UBC Theses and Dissertations

UBC Theses Logo

UBC Theses and Dissertations

Regulation of intracellular calcium concentration in vascular endothelial cells and valvular myofibroblasts Liang, Willmann 2004

Your browser doesn't seem to have a PDF viewer, please download the PDF to view this item.

Item Metadata


831-ubc_2004-93148X.pdf [ 13.65MB ]
JSON: 831-1.0099762.json
JSON-LD: 831-1.0099762-ld.json
RDF/XML (Pretty): 831-1.0099762-rdf.xml
RDF/JSON: 831-1.0099762-rdf.json
Turtle: 831-1.0099762-turtle.txt
N-Triples: 831-1.0099762-rdf-ntriples.txt
Original Record: 831-1.0099762-source.json
Full Text

Full Text

REGULATION OF INTRACELLULAR CALCIUM CONCENTRATION IN VASCULAR ENDOTHELIAL CELLS AND VALVULAR MYOFIBROBLASTS by WILLMANN LIANG B.Sc. (Hons.), The University of British Columbia, 2000 A T H E S I S S U B M I T T E D IN P A R T I A L F U L F I L M E N T O F THE REQUIREMENTS FOR THE D E G R E E OF DOCTOR OF PHILOSOPHY in T H E F A C U L T Y OF G R A D U A T E STUDIES Department of Pharmacology and Therapeutics We accept this thesis as conforming to the required standard  THE UNIVERSITY OF BRITISH C O L U M B I A August 2004 © Willmann Liang, 2004  ABSTRACT Background Some aspects of Ca  2+  signaling in vascular endothelial cells (ECs) and cardiac valvular  myofibroblasts (VMFs) were examined in this study. Over the last decade, the relationship between endothelial dysfunction, smooth muscle proliferation, and development of vascular diseases has been relatively well elucidated. Although the specific mechanisms remain unclear, it is generally agreed that alterations in endothelial Ca  regulation play an important role in  vascular pathophysiology. However, information regarding the underlying causes of valvular heart diseases is very limited, despite the large number of clinical cases reported. In the cardiac valve, ECs serve as a physical barrier between the VMFs underneath and the circulating blood. In addition, ECs secrete vasoactive substances in response to the enormous hemodynamic forces generated by the cardiac cycle. The endothelial secretions may have a general effect on the whole body or they may act locally on the cardiac valve.  The VMFs, being the most  predominant cells in the cardiac valve, perform a variety of functions to maintain normal valvular physiology. These functions, such as contraction, proliferation, and wound repair, are all directly or indirectly mediated by intracellular Ca concentrations ([Ca ]i). Thus, knowing 2+  2+  how [Ca ]i is regulated by vasoactive agents in VMFs becomes a critical step towards 2+  understanding valvular biology in both health and diseases.  Methods Both VMFs and ECs were loaded with Ca -sensitive fluorescent indicators fiira-2 and/or 2+  fluo-4. The cells were visualized with a fluorimeter-coupled microscope system. Measurements of [Ca ]i upon different pharmacological stimulations were done at room temperature (23 °C). 2+  Raw [Ca ]i data were analyzed with respect to i) their amplitudes and curve areas (as for the 2+  ii  VMF experiments) and ii) their decline rates (as for the EC experiments). Also in the VMF experiments, the Mn -quenching method was used to study divalent cation entry. Quantitative 2+  data were subjected to the appropriate statistical tests including Student's /-tests and one-way ANOVA. Results and Conclusions Part I: Ca Mobilization bv Pharmacological Agents in Valvular Myofibroblasts 2+  The fundamentals of Ca signaling properties in cultured human VMFs were studied. In 2+  VMFs, two agonist-induced and one store-operated Ca signaling pathways were identified, and 2+  observations of spontaneous Ca  2+  releases were made. The main findings are listed below.  Histamine, upon binding to Hi receptors, elicited [Ca ]i increase solely from ER Ca release in 2+  normal VMFs.  2+  In rheumatic VMFs, however, histamine also stimulated Ca  2+  influx.  The  purinergic agonists ATP and UTP activated P2Y2 receptors and induced both ER Ca release and 2+  Ca  2+  influx. The ER Ca  2+  emptying stimulated by histamine and ATP/UTP was limited to an  IP3-sensitive Ca store. A second ER compartment, the IP3-insensitive Ca store, released Ca 2+  2+  in response to SERCA blockade, which depletes the ER Ca  2+  2+  content and stimulates store-  operated Ca entry. There was also evidence for the presence of RyRs in VMFs, as shown by 2+  the effect of RyR modulation on spontaneous Ca releases. 2+  Data in support of the above findings are summarized in brief below. The selective Hi antagonist pyrilamine, but not the selective H2 antagonist cimetidine, abolished the histamineinduced [Ca ]j response, which showed no difference in the presence or absence of extracellular 2+  Ca or following treatment of SKF-96365, a blocker of Ca entry. In a Ca -free environment 2+  2+  2+  (or in the presence of SKF-96365), the duration of ATP/UTP-induced [Ca ]i response was 2+  shorter than in normal Ca -containing solution. This suggested a Ca 2+  2+  influx component  iii  regulated by purinergic receptor stimulation, as confirmed by accelerated M n entry as well. / +  The purinergic receptor subtype was characterized based on the following results: i) [Ca ]; 2+  response elicited by the selective P2Y2 agonist UTP; and ii) the lack of [Ca ]i response in VMFs 2+  challenged with the selective P2Y1 agonists ADP(3S and 2-Me-S-ATP. The presence of the IPsinsensitive ER Ca store was revealed by additional Ca release stimulated by CPA, following 2+  2+  repeated applications of histamine and ATP.  Store-operated Ca  application of CPA which increased the rate of M n  2+  entry was activated by  2+  entry. Unlike in normal VMFs, the curve  areas of histamine-elicited [Ca ]i responses in rheumatic VMFs showed a significant increase 2+  between Ca -containing and Ca -free environments, indicating that in the diseased cells 2+  2+  histamine also induced Ca  2+  entry. Finally, in a small number of VMFs spontaneous Ca  2+  releases in localized areas were observed. Blockade of the RyR elongated the latency period between each Ca releasing event, demonstrating the presence of functional RyRs in VMFs. 2+  Part II: Mechanisms of Ca Removal in Vascular Endothelial Cells 2+  How endothelial Ca homeostasis is maintained is still an unresolved issue, an important 2+  one though since cardiovascular diseases often prevail in the absence of controlled [Ca ]i 2+  regulation. In contrast to most published studies that investigated Ca the Ca  2+  entry pathways in ECs,  2+  removal mechanisms, which have equally vital roles in Ca  2+  homeostasis, were  examined in this study. In an effort to study cells that resemble physiological conditions as much as possible, a preparation of freshly isolated ECs was used. It was found that two pathways of extruding cytosolic Ca  2+  were present after agonist stimulation in ECs. The  sarco(endo)plasmic reticulum Ca -ATPase (SERCA), ryanodine receptor (RyR), and Na /Ca 2+  +  2+  exchanger (NCX) were components of the first pathway. The SERCA actively transported cytosolic Ca  2+  into the endoplasmic reticulum (ER). The RyR is a Ca  2+  release channel on the  iv  ER membrane. Ca exited the ER via the RyR and diffused across a subplasmalemmal restricted 2+  space to the plasmalemmal NCX, where Ca was extruded to the extracellular space. In parallel 2+  to the SERCA-RyR-NCX pathway, Ca extrusion also occured via the plasma membrane Ca 2+  2+  ATPase (PMCA), constituting the second Ca removal pathway in ECs. 2+  Data supporting the above findings are summarized as follows. Inhibitors of the SERCA, RyR and NCX, which respectively were cyclopiazonic acid (CPA), ryanodine (at the high concentration of 100 pM) and Na -free solution (ONaPSS), each slowed Ca removal rate to the +  2+  same extent. Combinations of these treatments, e.g. CPA+ONa and ryanodine+ONa, did not reduce Ca removal rate any further, indicating that the SERCA, RyR, and NCX are arranged in 2+  series. When the RyR was activated with caffeine or the low concentration of ryanodine (1 pM), Ca extrusion was facilitated. On the contrary, stimulation of RyR (with 1 pM ryanodine) and 2+  inhibition of SERCA (with CPA) together slowed down Ca extrusion, showing the sequential 2+  delivery of Ca  2+  from SERCA to RyR. When the SERCA-RyR-NCX pathway was blocked,  Ca extrusion could be further inhibited by blocking the PMCA with carboxyeosin, suggesting 2+  the contribution of the plasmalemmal Ca pump in removing cytosolic Ca . 2+  2+  v  TABLE OF CONTENTS ABSTRACT  ii  TABLE OF CONTENTS  vi  LIST O F T A B L E S  ix  LIST O F F I G U R E S  x  ABBREVIATIONS  xiii  LIST O F P U B L I C A T I O N S A N D A B S T R A C T S  xvi  ACKNOWLEDGEMENTS  xviii  C H A P T E R I: I N T R O D U C T I O N  1  1.1. O R G A N I Z A T I O N O F T H E C A R D I A C V A L V E  2  1.2. F U N C T I O N A L R O L E S O F V A L V U L A R M Y O F I B R O B L A S T S  5  1.3. O V E R V I E W O F V A L V U L A R H E A R T D I S E A S E S  7  1.4. C I R C U L A T I N G V A S O A C T I V E S U B S T A N C E S A N D T H E I R P H A R M A C O L O G I C A L A S P E C T S  12  1.5. P A T H O P H Y S I O L O G Y O F E N D O T H E L I A L C E L L S - I M P L I C A T I O N S O N V A L V U L A R H E A R T D I S E A S E S . 15 1.6. P H A R M A C O L O G Y A N D E N D O C R I N O L O G Y OF E N D O T H E L I A L C E L L S  16  1.7. E N D O T H E L I A L C A  20  2 +  TRANSPORTERS: C H A N N E L S , PUMPS, E X C H A N G E R S  1.8. E X A M P L E S O F I N T E R A C T I O N S B E T W E E N E N D O T H E L I A L C E L L S A N D M Y O F I B R O B L A S T S  23  C H A P T E R II: R A T I O N A L E O F S T U D Y , S P E C I F I C A I M S , A N D H Y P O T H E S I S  25  Specific aim #1: Characterization Mediated Ca  of Plasmalemmal  i) Histaminergic  Specific aim #2: Elucidation Contribution  Reticular  Receptor-  Signaling Pathways in Valvular Myofibroblasts  2+  Store-Operated  and Endoplasmic  & Purinergic Ca  Receptor Subtypes and ii)  Identifying  Functional  Channels and Ryanodine Receptors  2+  of Ca  Extrusion Pathways  2+  of Sarco(Endo)plasmic  Receptor, and Na -Ca +  -  2+  Exchanger  25  in Vascular Endothelial  Reticulum Ca -ATPase,  Cells -  Ryanodine  2+  and Plasma Membrane Ca -ATPase  C H A P T E R III: M A T E R I A L S A N D M E T H O D S  2+  26 28  3 . 1 . P R E P A R A T I O N OF V A L V U L A R M Y O F I B R O B L A S T S  28  3.2. P R E P A R A T I O N O F V A S C U L A R E N D O T H E L I A L C E L L S  29  3.3. M E A S U R E M E N T S OF I N T R A C E L L U L A R C A  30  3.3.1.  Conventional  Fluorescence  2 +  Microscopy  CONCENTRATION  30  vi  3.3.3. Rapid Laser-Scanning  Confocal Microscopy  35  3.4. M N - Q U E N C H [ N G E X P E R I M E N T S  35  3.5. F L U O R E S C E N T L A B E L I N G O F R Y A N O D I N E R E C E P T O R S  36  3.6. D A T A A N A L Y S I S A N D STATISTICS  36  2 +  3.6.1.  Ca  2+  Contents in Valvular Myofibroblasts  3.6.2. Spontaneous Ca  Release Rates and Duration in Valvular Myofibroblasts  2+  3.6.3. Ca  2+  37  Removal Rates in Vascular Endothelial  3.6.4. Three-Dimensional  Cells  38  Images of Ryanodine Receptors in Endothelial  Cells  38  3.7. S O L U T I O N S A N D C H E M I C A L S  C H A P T E R IV: C A  2 +  37  39  M O B I L I Z A T I O N B Y P H A R M A C O L O G I C A L A G E N T S IN  V A L V U L A R M Y O F I B R O B L A S T S (VMFS) - E R C A  2 +  STORES  AND M E M B R A N E RECEPTORS  40  4.1. O V E R V I E W  40  4.2. RESULTS  42  4.2.1.  Comparable [Ca ]j Responses in VMFs Originated from Different Patients 2+  4.2.2. Histamine-Induced  [Ca ] 2+  t  Increase is Independent of Extracellular  4.2.3. Evidence for Hi Receptor-Mediated 4.2.4. ER Ca  2+  Ca  Ca  2+  Signaling in VMFs  2+  Ca  Release from the ER  2+  4.2.6. Two Compartments of ER Ca 4.2.7. Activation ofCa  60  (and Mn ) Entry by SERCA Blockade  2+  66  2+  4.2.8. [Ca ]i Responses Elicited by A TP and UTP  70  2+  4.2.9. Ca  2+  Influx Component of A TP- and UTP-Induced  4.2.10. More Evidence for  P2Y2 Receptor-Mediated  4.2.11.  and A TP/UTP-Sensitive  Sizes of Histamine-  4.2.12. Selected Parameters of Ca  2+  4.2.13. Spontaneous Ca  [Ca ] 2+  Ca  t  Responses  ER Ca  2+  Stores  84 87  2+  Transporters  in VMFs  4.3. DISCUSSION  94 96  Histamine as an Intracellular  4.3.2. Intracellular  78 81  Signaling in Normal and Rheumatic VMFs  4.2.14. Schematic Model of Membrane Receptors and Ca  4.3.1.  73  Signaling in VMFs  2+  Release in VMFs  2+  53 57  Stores in VMFs  2+  47 50  Refilling is Essential in Regenerative Histamine Responses  4.2.5. Histamine-Insensitive  42  Ca  Ca  Release and Ca  2+  2+  4.3.3. Distinction between lP -Sensitive 3  4.3.4. Store-Operated  Mobilizing Agent in VMFs  2+  Ca  2+  96  Influx Stimulated by Purinergic Agents in VMFs  and IP -Insensitive 3  Channel Activity in VMFs  ER Ca  2+  Compartments  97 100 103  4.3.5. [Ca ]t Responses of Normal and Rheumatic VMFs  104  4.3.6. Spontaneous Ca  105  2+  2+  Releases and Functional  C H A P T E R V: MECHANISMS O F C A  2 +  Evidence for RyRs in VMFs  R E M O V A L IN V A S C U L A R  E N D O T H E L I A L C E L L S (ECS) - R O L E O F C Y T O S K E L E T O N AND C A  2 +  TRANSPORTERS  106  5.1. O V E R V I E W  106  5.2. R E S U L T S  109  5.2.1. Sarco(endo)plasmic (NCX)  Reticulum Ca -ATPase 2+  Contribute in Series to Ca  2+  (SERCA) and Sodium-Calcium  Exchanger  Removal in ECs  109  5.2.2. Serial Arrangement of SERCA and NCX is Maintained by Intact Cytoskeleton  115  5.2.3. Ca  122  2+  Removal is Facilitated  by RyR Opening and Inhibited by RyR Blockade  5.2.4. RyR Opening Accelerates ER Ca  2+  Loss in an Extracellular  5.2.5. Ryanodine Receptors and NCX Are Functionally  Ca -Free 2+  Coupled in Extruding  Environment Ca  2+  130 132  5.2.6. Ryanodine Receptors Act As a Link Between SERCA and NCX  135  5.2.7. Fluorescent Labeling of Ryanodine Receptors  138  5.2.8. Ca  2+  Removal via Plasma Membrane Ca -A 2+  TPase (PMCA)  after NCX (and RyR)  Blockade  141  5.2.9. Schematic Model of Ca  2+  Removal Pathways in ECs  144  5.3. DISCUSSION  146  5.3.7. Structural Arrangement of SERCA and NCX in Removal of Ca from 2+  5.3.2. Modulation  of RyR Activity by Selective Pharmacological  ECs  Agents  5.3.3. Other Potential RyR Modulators 2+  Ca  2+  and Depleting ER Ca  150  Removal Pathway  151  2+  5.3.6. Visualization of Ryanodine Receptors in Fresh Endothelial 5.3.7. Effect of Combined PMCA-  148 149  5.3.4. Role of RyR in Removing Cytosolic Ca 5.3.5. Position of RyR in the SERCA-NCX  146  and NCX-Inhibition  on Ca  2+  Cells  152  Extrusion  753  C H A P T E R VI: G E N E R A L C O N C L U S I O N S A N D F U T U R E D I R E C T I O N S  155  BIBLIOGRAPHY  157  LIST OF TABLES T A B L E 4 . 2 . 1 2 . 1 . C O M P A R I S O N OF H I S T A M I N E - , ATP-, A N D C P A - E L I C I T E D [ C A IN N O R M A L A N D R H E U M A T I C V A L V U L A R M Y O F I B R O B L A S T S  ], RESPONSES  LIST OF F I G U R E S FIGURE 1.1.1. O R G A N I Z A T I O N O F T H E C A R D I A C V A L V E  4  FIGURE 1.3.1. I M A G E O F A C A L C I F I E D M I T R A L V A L V E  9  FIGURE 1.3.2. I M A G E OF A N I M P R O P E R L Y C L O S E D A O R T I C V A L V E  10  F I G U R E 1.6.1. E N D O T H E L I A L SECRETIONS A N D THEIR A C T I O N S O N TISSUE C O N T R A C T I L I T Y  17  FIGURE 3.3. l . l . I M A G E O F F U R A - 2 - L O A D E D V A L V U L A R M Y O F I B R O B L A S T S ( V M F S )  33  FIGURE I M A G E O F F U R A - 2 - L O A D E D E N D O T H E L I A L C E L L S (ECs)  34  F I G U R E 4.1.1. F 4o/F o I M A G E S O F F U R A - 2 - L O A D E D V M F S B E F O R E A N D A F T E R H I S T A M I N E 38  3  STIMULATION  41  VMFs S A M P L E C P A - I N D U C E D [ C A ] , RESPONSES IN VMFs S A M P L E A T P - I N D U C E D [ C A ] , RESPONSES IN VMFs H I S T A M I N E - I N D U C E D [ C A ] , T R A N S I E N T IN VMFs IN OCAPSS H I S T A M I N E RESPONSE O F VMF IN T H E P R E S E N C E O F SKF-96365  F I G U R E S A M P L E H I S T A M I N E - I N D U C E D [ C A ] , RESPONSES IN  44  F I G U R E 4.2. l .2.  2 +  45  2 +  46  2 +  F I G U R E FIGURE 4.2.2. l . F I G U R E  48  2 +  49  VMFs RESPONSE IN VMFs  F I G U R E E F F E C T S OF P Y R I L A M I N E O N H I S T A M I N E - I N D U C E D [ C A ] , R E S P O N S E IN  51  F I G U R E E F F E C T S OF C I M E T I D I N E O N H I S T A M I N E - I N D U C E D [ C A ] ,  52  2 +  2 +  F I G U R E R E G E N E R A T I V E H I S T A M I N E RESPONSES IN  VMFs  54  FIGURE S E C O N D H I S T A M I N E A P P L I C A T I O N DID N O T ELICIT A R E S P O N S E IN OCAPSS FIGURE S E R C A B L O C K A D E A B O L I S H E D R E G E N E R A T I V E H I S T A M I N E RESPONSES IN F I G U R E 4.2.5. l . HISTAMINE-INSENSITIVE E R C A  2 +  C O M P A R T M E N T IN  55  VMFs  VMFs  58  FIGURE A C O N T R O L E X P E R I M E N T S H O W I N G 3 H I S T A M I N E RESPONSES IN NPSS FIGURE H I S T A M I N E - S E N S I T I V E E R C A  FIGURE F I G U R E 4.2.7. l . F I G U R E FIGURE FIGURE  C O N T E N T I N VMF  AFTER BASAL C A  2 +  59 LOSS  VMFs A F T E R B A S A L E R C A LOSS A C T U A L E R C A C O N T E N T IN VMFs (WITHOUT B A S A L E R C A LOSS) R E L A T I V E SIZES O F E R C A C O M P A R T M E N T S IN VMFs S T O R E - O P E R A T E D C A E N T R Y IN VMFs S T O R E - O P E R A T E D D I V A L E N T C A T I O N E N T R Y IN VMFs M N E N T R Y R A T E S B E F O R E A N D A F T E R C P A A D D I T I O N TO VMFs A T P - I N D U C E D [ C A ] , RESPONSES IN VMFs W I T H A N D W I T H O U T E X T R A C E L L U L A R  F I G U R E T O T A L E R C A F I G U R E  2 +  2 +  C O N T E N T IN  2 +  2 +  56  2 +  2 +  2 +  2 +  62 63 64 65 67 68 69  2 +  CA  71  2 +  F I G U R E U T P - I N D U C E D [ C A ] , RESPONSES IN 2 +  CA  VMFs WITH  A N D WITHOUT E X T R A C E L L U L A R 72  2 +  F I G U R E E F F E C T O F SKT-96365 O N A T P R E S P O N S E IN  VMFs  74  x  F I G U R E T I M E T A K E N FOR A T P (+/-SKF-96365)-INDUCED [ C A ] , R E S P O N S E TO D E C A Y / +  BY HALF  75  FIGURE M N  2 +  Q U E N C H I N G D A T A OF A T P / U T P A P P L I C A T I O N TO V M F S  76  FIGURE M N  2 +  E N T R Y R A T E S U N D E R B A S A L A N D A T P / U T P - S T I M U L A T E D CONDITIONS  77  FIGURE L A C K OF [ C A ] , R E S P O N S E U N D E R 2 +  ADPps  STIMULATION  79  F I G U R E L A C K OF [ C A ] , R E S P O N S E U N D E R 2 - M E - S - A T P S T I M U L A T I O N  80  FIGURE 4.2.1 l . l . A T P A N D H I S T A M I N E S H A R E D T H E S A M E E R C A  82  2 +  F I G U R E P A R T I A L ER C A  2 +  COMPARTMENT  2 +  EMPTYINGBY ATP  83  F I G U R E P S E U D O C O L O R E D F L U O - 4 - L O A D E D I M A G E S OF SPONTANEOUS C A  2 +  VMFs S H O W I N G V A R I O U S  ( S P C A ) R E L E A S E SITES R E C O R D E D O V E R T I M E  FIGURE E F F E C T S O F C A F F E I N E O N S P O N T A N E O U S C A  2 +  FIGURE E F F E C T S O F R Y A N O D I N E O N S P O N T A N E O U S C A F I G U R E DISTRIBUTION O F S P C A  89  2+  2 +  R E L E A S E S IN V M F S 2 +  90  R E L E A S E S IN V M F S  91  R E L E A S E D A T A AS A F U N C T I O N O F [ C A ] ,  F I G U R E L A T E N C Y PERIOD B E T W E E N S P C A F I G U R E S C H E M A T I C M O D E L OF C A  92  2+  2 +  2 +  RELEASE EVENTS  93  S I G N A L I N G IN V M F S  95  FIGURE 5.1.1. F 4o/F o I M A G E S O F F U R A - 2 - L O A D E D ECs B E F O R E A N D A F T E R A C E T Y L C H O L I N E 3  38  STIMULATION  108  FIGURE A C E T Y L C H O L I N E ( A C H ) - I N D U C E D [ C A ] , E L E V A T I O N S IN ECs  Ill  2 +  F I G U R E S U M M A R I Z E D D A T A O F [ C A ] , D E C L I N E R A T E S A T G I V E N R A N G E S O F [ C A ] ,  112  F I G U R E S A M P L E O N E - C O M P O N E N T E X P O N E N T I A L FITS O F [ C A ] , D E C L I N E PHASES IN ECs  113  2 +  2+  2 +  F I G U R E M E A N FITTED C A  2 +  D E C A Y R A T E C O N S T A N T S AS A P E R C E N T A G E O F T H E  CONTROL V A L U E  114  FIGURE 5.2.2. l . A C H - I N D U C E D [ C A ] , E L E V A T I O N S A N D D E C L I N E S IN C Y T O C H A L A S I N D 2 +  . (CYTD)-TREATED ECS  117  F I G U R E S U M M A R I Z E D D A T A O F [CA ], D E C L I N E R A T E S IN C Y T D - T R E A T E D ECs 2+  118  F I G U R E S A M P L E O N E - C O M P O N E N T E X P O N E N T E N T I A L FITS OF [ C A ] , D E C A Y P H A S E S 2 +  IN C Y T D - T R E A T E D ECs FIGURE C O M P A R I S O N O F T H E M E A N C A  119 2 +  R E M O V A L R A T E C O N S T A N T S IN C Y T D -  TREATEDECS  120  F I G U R E S A M P L E [ C A ] , RESPONSES IN L A T R U N C U L I N A (LATA)-TREATED ECs  121  F I G U R E E F F E C T S OF C A F F E I N E O N A C H - I N D U C E D [ C A ] , RESPONSES IN ECs  124  2 +  2 +  FIGURE E F F E C T S OF 1 u M R Y A N O D I N E - T R E A T E D A C H - I N D U C E D [ C A ] , RESPONSES IN E C S . . . . 125 2 +  FIGURE E F F E C T S OF 100 u M R Y A N O D I N E - T R E A T E D A C H - I N D U C E D [ C A ] , RESPONSES 2 +  IN  ECs  126  xi  F I G U R E R Y A N O D I N E R E C E P T O R (RYR) M O D U L A T I N G E F F E C T S O N C A  / +  REMOVAL  R A T E S IN ECs  127  F I G U R E S A M P L E O N E - C O M P O N E N T E X P O N E N T I A L FITS O F R Y R M O D U L A T O R - T R E A T E D [ C A ] , D E C A Y I N G P H A S E S IN E C S  128  2 +  FIGURE FITTED C A  2 +  R E M O V A L R A T E C O N S T A N T S IN R Y R - M O D U L A T E D E C S  F I G U R E E F F E C T S OF R Y R M O D U L A T I O N O N E R C A  129  CONTENT OF ECS  131  F I G U R E E V I D E N C E O F F U N C T I O N A L N C X A N D R Y R C O U P L I N G IN E C S  133  F I G U R E S U M M A R I Z E D D A T A O F C A  2 +  2 +  R E M O V A L R A T E S O F R Y R - & / O R N C X - I N H I B I T E D E C S . ..134  FIGURE E F F E C T S OF S E R C A B L O C K A D E A N D R Y R O P E N I N G O N C A FIGURE S U M M A R I Z E D D A T A OF C A  2 +  2 +  E X T R U S I O N F R O M E C S . . 136  R E M O V A L R A T E S O F C P A (+/-1 u M R Y A N O D I N E ) -  T R E A T E D ECS  137  F I G U R E B O D I P Y T R - X - R Y A N O D I N E L A B E L I N G O F R Y R S IN E C S  139  F I G U R E T H R E E - D I M E N S I O N A L COMPOSITES OF T H E B O D I P Y T R - X - R Y A N O D I N E - L A B E L E D ECS  140  FIGURE C O N T R I B U T I O N OF P M C A TO C A FIGURE S U M M A R I Z E D D A T A OF C A  2 +  2 +  R E M O V A L IN E C S  R E M O V A L R A T E S O F ONA ( + / - C A R B O X Y E O S I N ) -  TREATEDECS F I G U R E S C H E M A T I C M O D E L O F C A  142  143 2 +  R E M O V A L P A T H W A Y S IN E C S  145  xii  ABBREVIATIONS %F/s oc-nPSS  2+  [Ca ]i 2+  2+  OCaPSS ONaOCaPSS ONaPSS; ONa 2-D 2-Me-S-ATP 5-HT 5-HT  2  ACh ADPpS ANOVA anti-PCNA ATP AUC AV BODIPY TR-X Ca cADPR Ca-free PSS cAMP CE cGMP Cim COX-1 COX-2 CPA CVD CytD EC ECM EDCF EDHF EDRF EET EGTA eNOS ER ET-1 ET R; E T 2+  A  ET R; E T B  unit of divalent cation (or M n ) entry rate; F 3 6 0 per second antibiotic-containing normal physiological salt solution cytosolic C a concentration zero-Ca physiological salt solution zero N a zero C a physiological salt solution zero N a physiological salt solution two-dimensional 2-methyl-thio-adenosine 5 '-triphosphate serotonin serotoninergic (subtype) 2 receptor acetylcholine adenosine 5 '-0-(2-thio-diphosphate) analysis of variance anti-proliferating cell nuclear antigen adenosine 5'-triphosphate area under curve aortic valve 4,4-difluoro-4-bora-3a,4a-diaza-5-indacene Texas Red calcium ion cyclic adenosine 3,5-diphosphate ribose nominal Ca -free physiological salt solution cyclic 3',5'-adenosine monophosphate carboxyeosin cyclic 3',5'-guanosine monophosphate cimetidine cyclo-oxygenase-1 cyclo-oxygenase-2 cyclopiazonic acid combined valvular disease cytochalasin D endothelial cell extracellular matrix endothelium-derived contracting factor endothelium-derived hyperpolarizing factor endothelium-derived relaxing factor epoxyeicosatrienoic acid ethyleneglycol-bis((3-aminoethyl ether)-N,N,N ' N '-tetraacetic acid endothelial nitric oxide synthase endoplasmic reticulum endothelin-1 endothelin (subtype) A receptor endothelin (subtype) B receptor  A  B  2+  +  2+  +  2+  xiii  F340/F380 F36O  fGF-2 G protein H,R; Hi H R; H HEPES His hVMF ICCD IL-1 iNOS Ion IPs 2  2  IP3R  Kca channel Kd  LA LatA LSCM LuEry MCDB-131 MDMA Mn Mn MV Na NAADP NCX NHA NMDG NO nPSS NSCC Px 2+  +  2  P 2 Y 1 R ; P2Y1 P 2 Y 2 R ; P2Y2  PGI PLB PLC PM PMCA PMT PPADS Pyr 2  ratio of emitting fluorescence at 510 nm from Ca -bound over Ca -free fura-2 excited at 340 nm and 380 nm fluorescence intensity at 510-nm emission following excitation at 360 nm fibroblast growth factor 2 guanosine 5'-triphosphate binding protein histaminergic (subtype) 1 receptor histaminergic (subtype) 2 receptor 4-(2-hydroxyethyl)piperazine-l -ethanesulfonic acid histamine human valvular myofibroblast intensified charge-coupled device interleukin-1 inducible nitric oxide synthase ionomycin inositol 1,4,5-triphosphate inositol 1,4,5-triphosphate receptor calcium-dependent potassium channel dissociation constant local anesthetic latrunculin A rapid laser-scanning confocal microscope lupus erythematosus Molecular and Cellular Developmental Biology-131 3,4-methylenedioxymethamphetamine manganese chloride manganese ion mitral valve sodium ion nicotinic acid adenine dinucleotide phosphate Na /Ca exchanger sodium-hydrogen antiporter N-methyl-D-glucamine nitric oxide normal physiological salt solution non-selective cation channel purinergic (subtype) 2X receptor purinergic (subtype) 2Y1 receptor purinergic (subtype) 2Y2 receptor prostacyclin phospholamban phospholipase C plasma membrane plasma membrane Ca -ATPase photomultiplier tube pyridoxal-phosphate-6-azophenyl-2',4'-disulfonic acid pyrilamine 2+  +  2+  2+  2+  xiv  Rs RhMVD ROC ROI ROS RyR SBB SEM SERCA SKF-96365; SKF SOC  2+  2+  2+  2+  spCa release to TNFoc TRP channel TV UTP UV VMF 5  unit of area under curve; F 3 4 0 / F 3 8 0 ratio x seconds rheumatic mitral valve disease receptor-operated Ca channel region of interest reactive oxygen species ryanodine receptor superficial buffer barrier standard error of the mean sarco(endo)plasmic reticulum Ca -ATPase l-{a-[3(4-methoxyphenyl)propoxy]-4-methoxy-phenethyl}-lH-imidazole hydrochloride store-operated Ca channel 2+  spontaneous subcellular Ca release time required for peak F 3 4 0 / F 3 8 0 (or [Ca ]i level) to decay by half tumor necrosis factor-oc transient receptor potential channel tricuspid valve uridine 5'-triphosphate ultraviolet valvular myofibroblast 2+  xv  LIST O F P U B L I C A T I O N S A N D A B S T R A C T S Material from this dissertation has been published or accepted for publication: 1. X Wang, S Reznick, P Li, W Liang, C van Breemen. 2002. Ca removal mechanisms in freshly isolated rabbit aortic endothelial cells. Cell Calcium 31(6): 265-277. 2+  2. W Liang, P McDonald, B McManus, C van Breemen, X Wang. 2003. Histamine-induced Ca signaling in human valvular myofibroblasts. Journal of Molecular and Cellular Cardiology 35(4): Cover, 379-388. 2+  3. X Kuang, L Chan, W Liang, I Laher, C van Breemen, X Wang. 2003. The role of Kc in endothelial cell hyperpolarization and endothelium-dependent relaxation in the rabbit aorta. a  Endothelium-Dependent Hyperpolarization Factors 2002. Edited by P.M. Vanhoutte, Taylor  & Francis, New York, pp. 274-282. 4. W Liang, M Buluc, C van Breemen, X Wang. 2004. Vectorial Ca release via ryanodine receptors contributes to Ca extrusion from freshly isolated rabbit aortic endothelial cells. 2+  2+  Cell Calcium, in press.  Material from this dissertation is currently under preparation for submission: 1. W Liang, P McDonald, B McManus, C van Breemen, X Wang. 2004. Evidence for purinergic receptor-mediated Ca signaling in human valvular myofibroblasts. 2+  Material from this dissertation has been presented in oral form at the following meetings: 1. W Liang, P McDonald, B McManus, C van Breemen, X Wang. 2002. Current research in the mechanism of Ca signaling in human cardiac valves. 2 Annual Whistler Workshop on 2+  nd  Cardiovascular and Pulmonary Biology, Whistler, Canada.  2. W Liang, C van Breemen, X Wang. 2003. Role of ryanodine receptors in Ca extrusion in fresh endothelial cells. Frontiers in Cardiovascular Science, Vancouver, Canada, (also in poster form) 2+  3. W Liang, C van Breemen, X Wang. 2003. Ca extrusion in vascular endothelium - roles of IP3 and ryanodine receptors.  3  ,d  Annual Whistler Workshop on Cardiovascular and  Pulmonary Biology, Whistler, Canada. 4. W Liang, P McDonald, B McManus, C van Breemen, X Wang. 2004. Evidence for purinergic receptor-mediated Ca signaling in human valvular myofibroblasts. Experimental Biology 2004, Washington DC, USA. (also in.poster form) 2+  Material from this dissertation has been presented in poster form at the following meetings: 1. W Liang, P McDonald, B McManus, C van Breemen, X Wang. 2002. Ca compartments 2+  xvi  in the endoplasmic reticulum of human mitral valvular myofibroblasts.  XlVth World  Congress of Pharmacology, San Francisco, USA.  2. W Liang, C van Breemen, X Wang. 2002. Ca extrusion via ryanodine-mediated C a release channels in rabbit aortic endothelial cells. 10 International Symposium on Vascular Neuroeffector Mechanisms, Lake Tahoe, USA. 2+  2+  th  3. W Liang, C van Breemen, X Wang. 2003. Ca extrusion pathway involving ryanodine receptors and sodium-calcium exchanger in fresh rabbit aortic endothelial cells. 2+  Experimental Biology 2003, San Diego, USA.  4. W Liang, C van Breemen, X Wang. 2003. Ryanodine-mediated Ca extrusion pathway in 2+  fresh endothelial cells.  46 Annual Meeting of the Canadian Federation of Biological th  Sciences, Ottawa, Canada. 5. W Liang, P McDonald, B McManus, C van Breemen, X Wang. 2003. Regulation of intracellular calcium by purinergic receptors in human valvular myofibroblasts. 43 Annual rd  Meeting of the American Society for Cell Biology, San Francisco, USA.  6. W Liang, P McDonald, B McManus, C van Breemen, X Wang. 2004. Regulation of intracellular calcium in normal and rheumatic valvular myofibroblasts. 47 Annual Meeting th  of the Canadian Federation of Biological Sciences; P' Northern Lights Summer Conference,  Vancouver, Canada. Material from this dissertation has also been presented orally at the Graduate Student Seminar Series in the Department of Pharmacology and Therapeutics, University of British Columbia, and at the Research in Progress Seminars at the James Hogg iCAPTURE Centre for Cardiovascular and Pulmonary Research.  xvii  ACKNOWLEDGEMENTS I am most grateful to my supervisors, Dr. Casey van Breemen and Dr. Xiaodong Wang, for their wisdom and patience in guiding me through the adventures of my PhD journey. Casey and Xiaodong have put in tremendous efforts in introducing me to a wide variety of experimental techniques, engaging me in inspiring research discussions, and providing me with insightful advices on life experiences and career options. Despite the occasional obstacles I faced during the course of my degree program, it is a wonderful experience overall.  I also owe this  memorable experience to the members of my supervisory committee: Dr. Ismail Laher, Dr. Chun Seow, and Dr. Glen Tibbits, for their valuable inputs to my study. I would like to thank all the graduate students and postdoctoral fellows whom I have had a chance to work with in the lab. Thanks to their often words of encouragement and helpfulness when I first began postgraduate study. In particular, thanks to Dr. Bruce McManus and Dr. Paul McDonald for their help with the harvest of cardiac valves and isolation of valvular myofibroblasts. Also many thanks to Dr. Mesut Buluc for assisting me in conducting some of the experiments with endothelial cells. Finally, I would like to thank my parents, Kien Kong Liang and Rossana Liang, for their persistent support of my educational pursuit and for providing me with a comfortable learning environment. And to my friends who habitually but still willingly listen to me talking about calcium ions, thanks for all your patience.  XVlll  C H A P T E R I: INTRODUCTION Myofibroblasts and endothelial cells are the two most prevalent cell types in the cardiac valve. Endothelial cells act as a barrier between the myofibroblasts and the circulating blood. With an average 50 mL stroke volume and 70 to 80 heartbeats per minute, the cardiac valves, and especially ECs, are consistently subjected to enormous hemodynamic forces. In response to different physiological requirements, ECs secrete various vasoactive substances to the surrounding tissues and circulation. Valvular myofibroblasts (VMFs), located beneath the ECs, are direct recipients of different endothelial secretions. These secretions may regulate numerous functions of VMFs including contraction and wound repair, etc. These processes likely relate to interactions between VMFs and ECs. In cases of valvular heart diseases, damages to ECs may expose VMFs to the circulating substances, altering the valvular biology at the same time. On the other hand, VMFs may proliferate, migrate, and attempt to remodel the functions of a healthy valve. Thus, ECs and VMFs are perhaps independently and cooperatively responsible for the maintenance of valvular physiology in both health and disease. However, many of the cellular signaling events involved are currently unknown, in spite of the growing incidence of valvular heart diseases in the world. The research field of signaling mechanisms in the cardiac valve is therefore a novel one, with it requires fundamental understanding of how ECs mediate the synthesis of vasoactive substances and how VMFs may respond to the endothelial secretions. This study will first look in detail at the agonist-induced Ca Then the Ca  2+  2+  signaling properties of VMFs.  removal mechanisms in ECs, which play significant roles in intracellular Ca  2+  homeostasis and consequently regulating releases of secretory agents, are investigated. This introductory chapter will provide information relevant to the background, design, and outcomes of the current study.  1  In the following sections, the anatomical features of the cardiac valve are introduced first. Valvular myofibroblasts (VMFs) are multi-functional cells making up the bulk of the cardiac valve, and their various roles in valvular physiology, in both health and disease, will be summarized.  Also discussed are the pharmacological characteristics of major vasoactive  substances potentially modulating valvular function.  Another type of valvular cells, the  endothelial cells (ECs), lining the surface of cardiac valves, serves many functions: protective barrier for underlying tissues, control of valvular tone, and maintenance of blood fluidity. These functions of endothelial cells (ECs) are made possible by a number of secretory substances. Precise regulation of the amount and type of endothelial secretions is in large part mediated by controlled Ca  2+  fluxes via various Ca  2+  transporters. An overview will thus be given on the  substances released by ECs and the entities responsible for Ca homeostasis in ECs. Effects of 2+  damaged ECs on tissue physiology will also be discussed. Finally, the introductory chapter will close with a discussion of some examples of interactions between endothelial cells and myofibroblasts in other tissues, which provide supportive evidence for similar cell-cell communications in the cardiac valve.  1.1. Organization of the Cardiac Valve During embryonic development, mesenchyma, descended from endocardial cells, grow out of the cardiac cushion to become the cardiac valve (Taylor et al. 2003). The cardiac valve is a multi-layered structural entity composed of four main cell types embedded in connective tissue matrix. The outermost valvular layers are the atrialis facing the atrial side and the ventricularis facing the ventricular side (Mulholland and Gotlieb 1996). Semi-lunar valves, also known as aortic and pulmonary valves, lack the atrialis layer that is only present in atrio-ventricular, or mitral and tricuspid, valves (Ferrans and Rodriguez 1991). Elastic fibres and smooth muscle  2  cells make up the atrialis layer, which only covers the proximal end of the valve. The free or distal end of the valve consists mainly of the spongiosa layer, and it is where most of the extracellular matrices are (Mulholland and Gotlieb 1996).  Collagen is also present in the  spongiosa, but most is located in the fibrosa, which is the thickest layer in the valvular leaflet (Mulholland and Gotlieb 1996). Chordae tendineae extend from the fibrosal collagen and into the endocardium. Four types of cells are found in the cardiac valve. Figure 1.1.1 shows an illustration of a cross-sectional view of a cardiac valve. In the figure, bright-field images of enzymatically dissociated ECs and VMFs are also shown. The surface is lined with a continuous layer of ECs that extends along the atrial and ventricular endocardial surfaces (Mulholland and Gotlieb 1996). Cardiac myocytes are often present at the bases of atrio-ventricular valves (Mulholland and Gotlieb 1996). The base of the valvular leaflet contains blood vessels, and thus smooth muscle cells are always found in that region (Mulholland and Gotlieb 1996). Myofibroblasts are the most prominent cells in the valve and are present in all tissue layers (Taylor et al. 2000). VMFs are mostly arranged loosely in vivo, with much intercellular space filled with extracellular matrices (ECMs) (Mulholland and Gotlieb 1996). Integrins form links between VMFs and ECMs and mediate cell proliferation and cell motility (Taylor et al. 2003). Communications among VMFs also occur where there are close contacts between cells, via adherens junctions (Lester et al. 1988) and gap junctions (Filip et al. 1986).  3  The diagram shows the main components of a cardiac valve. The cell types of interest in this study are the endothelial cells (ECs) and valvular myofibroblasts (VMFs), which are the most predominant cells in the valve. Cardiac and smooth muscle cells may be present near the valvular root. Brightfield microscopic images of enzymatically-dissociated ECs and VMFs are shown as reference. VMFs are arranged loosely in vivo and where there are close contacts, gap or adherens junctions form links between the cells. The majority of the space between VMFs are filled with extracellular matrices (ECMs), the synthesis of which are one of the important functions of VMFs. Figure 1.1.1. Organization of the cardiac valve.  4  1.2. Functional Roles of Valvular Myofibroblasts Staining and functional studies on VMFs have revealed the various functions of these cells. Characteristics of smooth muscle cells are found in VMFs. Fluorescent labeling with anticGMP-dependent protein kinase, usually used as a smooth muscle marker, stains VMFs, but not fibroblasts and endothelial cells (Filip et al. 1986). Moreover, VMFs contains a-smooth muscle actin, although not as much as in smooth muscle cells (Zacks et al. 1991). Contractility of VMFs was first proposed when actin microfilaments, anchored in electron-dense bodies (Filip et al. 1986), colocalized with myosin in microfilament bundles (Lester et al. 1988). When VMFs are grown on a silicone rubber substratum, application of vasoactive substances results in wrinkling of the substratum, indicating contraction of VMFs (Filip et al. 1986; Messier et al. 1994). Studies of whole valvular leaflets have also demonstrated isometric force generation upon agonist stimulation (Filip et al. 1986; Taylor et al. 2000). Thus, VMFs probably contract in vivo to counter the enormous hemodynamic forces (Mulholland and Gotlieb 1997). The structure and function of the cardiac valve are maintained by ECMs, and their secretion is another function of VMFs (Mulholland and Gotlieb 1997). The main constituents of valvular ECMs are collagen, elastin, and proteoglycans.  The proteoglycans provide an  attachment base for collagen and elastin (Mulholland and Gotlieb 1996).  There is also  suggestion that the proteoglycans alleviate friction between the fibrosa and ventricularis (Tamura et al. 1995). Types I and III collagens are present in the greatest amounts, but traces of Type V collagen are also found (Bashey and Jimenez 1988; Lis et al. 1987). Collagen helps the valve to maintain its shape in response to pressure. Elastin, on the other hand, provides flexibility to the valve so that it can distend accordingly to the pressure. Thus, the collagen-rich fibrosa, being the thickest layer in the valve, is able to provide strength while the elastin-rich atrialis and  5  ventricularis gives elasticity on the free ends of the valve. The ECMs, via regulating growth factors, mediate valvular growth and differentiation (Flaumenhaft and Rifkin 1991; Carey 1991). The distribution and organization of ECMs are altered in disease conditions, and these are reflected in valvular dysfunction. For example, ECM remodeling as a result of increased matrix metalloproteinase activities, is observed in valves of patients with Marfan syndrome (Segura et al. 1998). Elsewhere, Lis et al. reported that both rheumatic and floppy valves have higher collagen contents than normal tissues (Lis et al. 1987).  The increase in collagen has different  consequences between the two pathological conditions, however. In floppy valves, interactions between proteoglycans and collagen cease as well as cross-linking within core collagens, resulting in fragility of the tissue (Lis et al. 1987). Fibrosis due to overproduction of surface collagen is often observed in floppy but not rheumatic valves (Lis et al. 1987). In contrast to floppy valves, rheumatic valves contain a wealth network of core collagen that results in tissue thickening (Lis et al. 1987). The modifications to valvular anatomy mentioned above are potential outcomes of valvular diseases, and the developments of which are triggered by endocardial injury. The injury may arise from surgical interventions in the treatment of cardiac and valvular diseases (Mulholland and Gotlieb 1996). As the immediate cells beneath the endocardial or endothelial layer, VMFs participate actively in valvular wound repair. The repair process does not end up with the normal endothelial monolayer but overlapping of cells is observed (Lester et al. 1988). It is the property of the newly formed valvular surface that suggests that VMFs, and not ECs, are involved in injury repair.  A study used an organ culture model with the dissection site  resembling the edge of the wound (Lester et al. 1992). Proliferating cells were stained with antiProliferating Cell Nuclear Antigen (anti-PCNA), since PCNA accumulates during active mitosis  6  (Kurki et al. 1988). Lester et al. found that only VMFs were positively stained with anti-PCNA and that the immunolabeling only occurred near the dissection site, i.e. where the wound was located (Lester et al. 1992). Therefore, it is concluded that VMFs proliferate and migrate in the event of valvular injury.  1.3. Overview of Valvular Heart Diseases Since many functions of VMFs revolve around disease conditions, it will be of interest here to discuss the indications of the most clinically relevant valvular heart diseases, with references to structural and cellular modifications. For detailed explanation on all types of valvular pathologies, the readers are advised to refer to Alpert et al. (2000). The occurrence of valvular heart diseases is much less often than coronary artery disease, but the former still contributes significantly to the cause of heart failure and sudden deaths (Wilson 1997; Mangion and Tighe 1995; Grigioni et al. 1999). Both valve-associated hospitalizations and surgical interventions in the New York State from 1983-2000 have seen a three-fold increase (Supino et al. 2002). The incidences of degenerative, drug-induced, and microorganism-induced valvular heart diseases are all on the rise (Soler-Soler and Galve 2000). People in the developed world are most seriously affected by age- and lifestyle-related valvular conditions whereas in developing countries, people are hit hardest by valvular problems arisen from hygienic issues. In brief, valvular heart diseases may be classified according to their sites of occurrence. In the mitral valve (MV), prolapse and rheumatic disease are two common conditions. M V prolapse is a result of degeneration of the fibrosal tissue, and in severe cases can cause valvular thickening and chordal elongation, leading to poor structural support of the valvular leaflet (Farb et al. 2000). Calcification is also a symptom of MV prolapse, as well as in chronic rheumatic MV disease (RhMVD) (Farb et al. 2000). Figure 1.3.1 shows an image of a calcified mitral  7  valve from a 58-year-old male (Manabe and Yutani 1998).  In chronic RhMVD, valvular  scarring due to fusion of valvular structures results in mitral stenosis (Farb et al. 2000). Inflammatory cells and VMFs are present concurrently with capillary formation (Farb et al. 2000). Secondary effects of PvhMVD and stenosis include congestive heart failure, dyspnea, and atrial fibrillation (Farb et al. 2000). Chronic RhMVD mostly happens in individuals with acute RhMVD previously.  Acute RhMVD is usually a consequence of pancarditis, which is  inflammation of all three layers of the heart (Farb et al. 2000). Pancarditis is often a result of an altered immune response to Group A hemolytic Streptococcus infections, and thus acute RhMVD remains prevalent in developing countries (Farb et al. 2000; Soler-Soler and Galve 2000). Other valvular pathologies may arise indirectly from RhMVD. In both aortic valve (AV) and tricuspid valve (TV), post-rheumatic valvular disease is a frequent problem, leading to symptoms similar to those in mitral stenosis (Farb et al. 2000). Chordal thickening is usually less severe in TV than in MV and A V (Farb et al. 2000). In AV, calcification, inflammation, and neovascularization may occur. Calcification is also seen in degenerative A V stenosis, which is associated with coronary atherosclerosis, increasing age, smoking, hypertension, and high lowdensity lipoprotein levels (Farb et al. 2000). A V regurgitation may derive from both postrheumatic and degenerative A V diseases (Farb et al. 2000). Figure 1.3.2 shows an image of an aortic valve with fibrotic thickening causing it to close improperly (Manabe and Yutani 1998). Regurgitating valves of the left heart are particularly significant in causing dyspnea and fatigue.  8  Figure 1.3.1. Image of a calcified mitral valve. The valve was isolated from a 58-year-old male. There is prominent fibrotic thickening of the valvular leaflets (white portions near where the arrows are), in contrast to the transparent portions near the top of the figure. There are also obvious calcified deposits (yellow-appearing structures ponted by arrows), which are often  observed in valvular heart diseases. [Figure reproduced from Manabe and Yutani 1998]  calcified deposits  9  Figure 1.3.2. Image of an improperly closed aortic valve. The valve was isolated from a 54year-old female. Fibrotic thickening of the valvular leaflets is evident and fusion of structures are observed in the distal (free) ends of the valve. The opening in the middle of the figure indicates improper closing of the valve, resulting in aortic regurgitation. [Figure reproduced  from Manabe and Yutani 1998]  improper closing of the valve  fibrotic thickening  10  Besides valvulopathies specific to a particular valve, combined valvular disease (CVD) occurs in a small number of patients (Paraskos 2000). Rheumatic heart disease is the most common cause of CVD, but it may be associated with systemic and drug-induced diseases as well (Paraskos 2000). Conditions involving all four valves are extremely rare. Simultaneous MV stenosis and AV regurgitation/stenosis has much higher incidence than combined TV and MV stenosis (Paraskos 2000). There have been reports noting cardio-protective effects in CVD. In one example, MV stenosis protects the left ventricle from back pressure of A V regurgitation (Paraskos 2000). In another example, TV stenosis protects the right ventricle from the extensive effects of MV stenosis (Paraskos 2000). As mentioned above, systemic conditions such as metastatic carcinoid tumor and lupus erythematosus (LuEry) are likely to result in CVD. Carcinoid tumor is vaguely defined as a tumor with characteristics not distinguishable from gastro-entero-pancreatic neuroendocrine tumor (Quaedvlieg et al. 2002).  In both carcinoid tumor and LuEry-associated valvular  dysfunctions, EC injury plays a significant role in disease development (Farb et al. 2000; Quaedvlieg et al. 2002).  In carcinoid valvular disease, plagues of smooth muscle cells,  proteoglycans, and probably VMFs adhere to valvular surfaces where ECs normally are (Farb et al. 2000). The presence of plagues results in thickening of valvular leaflets and stenosis. Connolly et al. reported structural changes in valves, similar to those observed in carcinoid valvular diseases, in patients taking appetite suppressants (Connolly et al. 1997). This report shares a common aspect with studies that showed valvular dysfunction caused by ergot alkaloids (Redfield et al. 1992) and by 3,4-methylenedioxymethamphetamine (MDMA) in that the drugs tested in all three studies are serotonin (5-HT) agonists (Setola et al. 2003). These 5HT mimetic agents are believed to activate 5-HT2 receptors, eliciting their effects on migraine  11  headache and on appetite suppression (Fitzgerald et al. 2000; Xu et al. 2002). Complicated signaling pathways downstream of 5-HT receptor stimulation have been elucidated that involves phospholipase C (PLC), protein kinase C, mitogen-activated protein kinase and extracellular signal-related kinase pathways. These pathways regulate hundreds of cellular functions that require detailed discussion of each. Nevertheless, the fact that carcinoid tumors also releases 5HT may explain why Connolly et al. observed similar morphological changes in anorexigeninduced valvular disease. Despite the diverging signaling cascades induced by 5-HT, the PLC pathway raises particular interests.  This is partly due to the PLC-regulated intracellular Ca mobilization 2+  common to many pharmacological agonists. More importantly, many valvulopathies discussed in this section have no known 5-HT-related effects, but display structural modifications including calcification. No report has explored the relationship between calcified valves and Ca  2+  signaling properties in VMFs. However, there were studies showing evidence for the role  of Ca mobilization in mediating calcification in canine fibroblasts (Kim 1994; Kim et al. 1999). 2+  Therefore, associations between VMFs' intracellular Ca  2+  responses to agonists may provide  clues to the development of valvular heart disease.  1.4. Circulating Vasoactive Substances and Their Pharmacological Aspects Considering the many activities of VMFs in maintaining a healthy valve and in remodeling a diseased valve in the previous sections, it is unclear why research has not been emphasized in investigating the underlying signaling mechanisms. The finding that VMFs are contractile was rather significant because of its implications on structural support, cell motility and wound closing. However, there were only limited research efforts to examine agonistinduced contractions of valvular leaflets and VMFs. Filip et al. reported for the first time ever  12  the contractility of single VMFs under treatments of epinephrine and angiotensin II (Filip et al. 1986). Almost eight years later Messier et al. reported that bradykinin, carbachol, and KC1 also induced contractions in VMFs (Messier et al. 1994).  Neither study attempted to  pharmacologically characterize the receptors involved in contracting the cells though. It was until the year of 2000 that the first comprehensive study was conducted on agonist-induced valvular contractions (Chester et al. 2000).  A variety of vasoactive substances and their  respective receptor antagonists were applied to intact valvular leaflets. Their force generations were measured and concentration-response relationships were established.  In the study,  epinephrine, norepinephrine, endothelin-1, thromboxane A , 5-HT, and histamine, all of which 2  are important vaso-modulators, were used to elicit the contractions. However, by looking at the entire leaflet, the drug effects on VMFs alone were not examined, since it has been documented that smooth muscle cells might also be present near the valvular root (Mulholland and Gotlieb 1996).  In view of this shortfall, and the regulatory role of histamine and adenosine 5'-  triphosphate (ATP), respectively, in inflammation and ischemia, the following paragraphs will discuss about the pharmacological characteristics of these two agents. Three subtypes of histamine receptors have been identified, but only two, Hi and H , are 2  present in the heart. Hi receptor (HiR) activation reduces atrio-ventricular node conduction (Hattori 1999). Stimulation of H receptors (H R) increases heart rate (Hattori 1999). Increased 2  2  cardiac contractility is a result of combined effects of Hi and H receptors, depending on the 2  species (Hughes and Coret 1972; Verma and McNeill 1977). Both HiR and H R are coupled to 2  GTP-binding proteins (G proteins) : H)R with the G subunit, and H R with the G subunit. q  2  s  Stimulation of HiR leads to the activation of phospholipase C, production of 1P3 and increase in [Ca ]i (Hill 1990). H R-induced [Ca ]; increase is also present in certain cells (Chew 1985, 2+  2+  2  13  Mitsuhashi et al. 1989), but the most common effect of H2R activation is the stimulation of adenylate cyclase and production of cAMP (Hill 1990). It should be noted that a hypothesis for the presence of an intracellular histamine receptor is supported by some studies (Saxena 1989; Brandes 1990, 1992). The purpose of the proposed intracellular histamine receptor is in the mediation of tumor cell proliferation (Bartholeyns and Boucher 1984; Bartholeyns and Fozard 1985; Watanabe et al. 1981), although the existence of such a receptor has not been widely accepted. Noting the proliferating role of VMFs in the cardiac valve, there may be a function for the intracellular histamine receptor in these cells. ATP increases cardiac contractility via actions on both P2X and P2Y receptors (Vassort 2001). The lack of specific ligands has slowed the progress on the characterization of purinergic receptors and generated conflicting reports on receptor subtypes. In the heart,  P2X1-7  receptors  have been found and are all ionotropic, meaning the receptors function as nonselective cation channels, with permeability to Na , K , and Ca (Bean 1992, Dubyak and el-Moatassim 1993). +  +  2+  All P2Y receptors are coupled to G-proteins. Five of a total 11 P2Y receptor subtypes are present in the heart: P2Y1, P2Y2, subtypes except  P2Y4,  P2Y4, P2Y6,  and  P2Y11  (Vassort 2001). ATP is fully agonistic on all  and UTP is only active on  P2Y2  and  P2Y4  (Vassort 2001).  P2Y2  and  P2Y  P2Y4  were formerly known as P2U receptors because of their activation by UTP (Ralevic and Burnstock 1998).  It is possible to distinguish  P2Y2  from  P2Y4  receptors by the latter's  nonresponsiveness to ATP. Activation of P2Y2 receptors results in PLC-mediated and increased  [Ca ]i, 2+  IP3  production  although cAMP and cGMP production have also been reported (Post et al.  1996;Buvinic et al. 2002).  14  7.5. Pathophysiology of Endothelial Cells - Implications on Valvular Heart Diseases The discussion so far has been limited to the roles of VMFs in valvular (patho)physiology. Indeed VMFs are the key players in the progression of valvular heart diseases. However, it is often the ECs which become dysfunctional or injured that initiate signaling events leading to the activation and proliferation of VMFs in valvular heart diseases. Such interactions between ECs and VMFs are implied because of suggestive roles of excessive nitric oxide (NO), fibroblast growth factor-2 (fGF-2), and endothelin-1, all secreted by injured ECs, in repairing valvular and vessel damages (Durbin and Gotlieb 2002; Siney and Lewis 1993; Villaschi and Nicosia 1993). Specifically, the modified secretions from ECs are likely the results of dysfunctional Ca  2+  homeostasis. In a number of vascular abnormalities such as reperfusion injury, atherosclerosis, and post-operative grafts, there are associations with altered Ca  2+  signaling mechanisms in both  ECs and smooth muscle cells (Lounsbury et al. 2000; Irani 2000; Mehta et al. 1997). Direct evidence for modified endothelial Ca  2+  signaling properties has not yet been shown in valvular  heart diseases, but pathological changes to the structure and functions of ECs similar to those in vascular diseases are observed. A few examples are cited here. In endocarditis, thrombosis attracts adhesion molecules and valvular thickening and stenosis develop (Lopez et al. 1987). Inflammatory responses arisen from rheumatic valvular disease render the ECs antigenic and subject to attack by antibodies (Galvin et al. 2000). Floppy valves may lose ECs due to improper valvular closing and results in activation of cell proliferation signals and direct exposure of the sub-endothelial cells (i.e. valvular myofibroblasts) to vasoactive agents (Stein et al. 1989). In view of the damages to ECs in valvular heart diseases, modifications to endothelial Ca  2+  signaling and resultant secretory products may be detected in future studies. Meanwhile, it is  15  important to first understand the relationship between Ca homeostasis in ECs and their releases z+  of vasoactive substances, which will be discussed next. 1.6. Pharmacology and Endocrinology of Endothelial Cells  The vaso-modulatory function of ECs has been extensively studied and reviewed. Although there is very little information about endothelial influences on the VMFs, it is postulated that interactions similar to those between ECs and vascular smooth muscle also exist in the cardiac valve. In the vasculature, ECs secrete a variety of substances that bind to membrane receptors of smooth muscle cells or diffuse across the vessel wall with an ultimate effect on contractility and in in vivo conditions, result in a change in blood pressure. Secretions by ECs for this purpose may be classified into endothelium-derived contracting factors (EDCFs) and endothelium-derived relaxing factors (EDRFs). Each EDCF and EDRF not only elicits its own independent effects but also interacts with each other to mediate vascular smooth muscle function. Figure 1.6.1 summarizes the most common endothelial secretions and their actions on the underlying vascular smooth muscle or valvular myofibroblasts.  16  Figure 1.6.1. Endothelial secretions and their actions on tissue contractility. This schematic  diagram shows the most common secretions by the endothelial cell (EC) that contribute to the contraction or relaxation of the underlying vascular smooth muscle (VSM) or valvular myofibroblast (VMF). The EC synthesizes relaxing factors: i) nitric oxide (NO) by endothelial nitric oxide synthase (eNOS); ii) prostacyclin (PGI2) by cyclo-oxygenases 1 & 2 (COX-1,2); and iii) epoxyeicosatrienoic acid (EET) by cytochrome P450 (CYP). EET activates Ca -sensitive potassium (Kc ) channels on EC or VSM, allowing K efflux and membrane hyperpolarization. An alternative theory suggests that K efflux from EC diffuse to VSM and activates the inwardrectifying K (KIR) channels, causing relaxation. There is also evidence for the function of myoendothelial gap junctions between EC and VSM where hyperpolarizing signals (or electrical charges, q) are transmitted across the cellular layers. Contracting factors synthesized by EC are: i) excessive NO from eNOS and iNOS; ii) ROS including H2O2; iii) endothelin-1 (ET-1) from epinephrine, thrombin, interleukin-1, and angiotensin II (Angll) stimulations of EC - ET-1 then acts on ET receptor (ET R); and iii) autocrine release of Angll acting on ATi receptor (ATiR). 2+  +  a  +  +  A  A  VSM or VMF relaxation  17  Nitric oxide (NO) is a well-established example of EDRF.  Endothelial nitric oxide  synthase (eNOS) oxidizes Z-arginine to form NO and citrulline. In normal physiological conditions, a small amount of eNOS is constitutively expressed, contributing to basal NO release (Nishida et al. 1992; Weiner et al. 1994). Low levels of NO facilitates cyclic 3'-5'-guanosine monophosphate (cGMP) production via guanylate cyclase. cGMP-dependent protein kinases in vascular smooth muscle induce vasodilatation (Huang et al. 2000). It was mentioned in Section 1.2 that cGMP-dependent protein kinases are present in valvular myofibroblasts (VMFs). Thus, NO from the endothelium may influence the VMFs underneath in the cardiac valve. Both shear stress and pharmacological agents such as acetylcholine and histamine can elicit [Ca ]i increase z  in ECs. The associations between [Ca ]j and NO are strengthened by the elucidation of a 2+  negative feedback system which shows enhanced cytosolic Ca of cGMP (Lau et al. 2003).  2+  removal following application  Increase in endothelial [Ca ]i is followed by transient NO 2+  production in the same time frame, i.e. several seconds. However, continuous NO release is maintained by another mechanism. Studies have shown that activation of phosphatidylinositol3-kinase, serine kinases Akt, and protein kinase A leads to the phosphorylation of the reductase domain of eNOS, increasing its activity (Dimmeler et al. 1999; Go et al. 1998). Another NOS, the inducible NOS (iNOS), is expressed when ECs are stimulated with cytokines.  Large  amounts of NO are produced by iNOS. However, the excessive NO is also a source of reactive oxygen species, which are regarded as EDCFs. Besides inducing its own direct effects on vascular relaxation, NO also modulates the production of another EDRF - prostacyclin (PGI2) (Marcelin-Jimenez and Escalante 2001). Aside from NO regulation, PGI2 production is mediated by cyclooxygenases 1 and 2 (COX-1, COX-2).  In ECs, COX-1 is constitutively present while COX-2 is only expressed in  18  inflammatory reactions (Davidge 2001).  Similar to NO, PGI2 synthesis is dependent on  endothelial [Ca ]i, except with two differences. Firstly, higher [Ca ]i than in NOS activation is 2+  2+  necessary for the activation of phospholipase A2 and generation of arachidonic acid, which is the substrate of COX. Secondly, unlike NO release upon shear stress, cyclic stress of the vessel stimulates PGI2 production (Rosales et al. 1997). The third group of EDRFs is endothelium-derived hyperpolarizing factor (EDHF). The identity of EDHF(s) is still debatable, but three major theories have been developed with all showing relationships with endothelial Ca -dependent K (Kc ) channels. 2+  +  a  Campbell et al.  proposed that endothelial cytochrome P450 epoxygenase generates epoxyeicosatrienoic acids (EETs), activating K  C a  channels on either ECs or smooth muscle cells (Campbell et al. 1996).  Another theory claims K exiting endothelial K c channels diffuses to smooth muscle cells and +  a  hyperpolarizes the cells by opening inward-rectifying K channels (Edwards et al. 1998). Finally, +  Segal et al. proposed tightly coupled myo-endothelial gap junctions transmit the hyperpolarizing signal across the vessel wall (Emerson and Segal 2000). It was mentioned earlier that excessive NO could be a source of reactive oxygen species (ROS), which is an example of EDCF.  Though, the primary ROS released by ECs are  superoxide anions and H2O2 (Hishikawa et al. 1997). Although ROS synthesis is often related to oxidative stress-induced vascular diseases such as atherosclerosis, EC production of ROS occurs in normal conditions as well.  To further complicate the issue, ROS do not always cause  vasoconstriction. Matoba et al. suggested that H2O2 has vasodilatory effects and is a potential EDHF (Matoba et al. 2002). In addition, H2O2, by increasing endothelial [Ca ]i, can activate 2+  eNOS, producing NO that stimulates guanylate cyclase in smooth muscle cells, and the increased cGMP levels cause vasorelaxation (Yang et al. 1999; Iesaki et al. 1999).  19  Endothelin-1 (ET-1) is another main EDCF having vasodilatory effects.  ECs usually  release ET-1 when stimulated with angiotensin II, interleukin-1, thrombin, and epinephrine (Drexler 1997). When bound to E T receptors on smooth muscle cells, ET-1 causes potent A  vasoconstriction (Busse and Fleming 2003). However, ET-1 also binds to endothelial E T  B  receptors which, upon activation, have stimulatory effects on NO and PGI2 syntheses (Busse and Fleming 2003; Lavallee et al. 2001). Vasodilatation is undoubtedly caused by the increased NO and PGI2 production, as a consequence of the ET-1-mediated negative feedback (Ullrich and Bachschmid 2000; Wagner et al. 2001). Moreover, NO and PGI2 enhance, respectively, the production of cGMP and cAMP in ECs, and these cyclic nucleotides inhibit additional ET-1 synthesis and release (Boulanger and Luscher 1990). 1.7. Endothelial Ca  2+  Transporters: Channels, Pumps, Exchangers  It is clear from the above discussion of EDCFs and EDRFs that intracellular Ca plays a central role in either the synthesis or modulation of the secretory substances. In the following paragraphs, the main endothelial Ca  transporters are introduced, with an emphasis on those  2+  2~F  2"F  involved in unloading cytosolic Ca . Details on all Ca transporters are extensively reviewed in Nilius and Droogmans (2001), Brini and Carafoli (2000), and Tran et al. (2000). 2+  Membrane-bound Ca triphosphate receptors  (IP3RS)  •  entry channels and endoplasmic reticulum (ER) inositol 1,4,5are the two main endothelial Ca  2+  channels responsible for  generating [Ca ]i increases in response to physiological and pharmacological stimuli. Most 2+  stimuli bind to G-protein-coupled receptors and activate phospholipase C (PLC) with a production of IP3. The IP3 opens IP R and stimulates ER Ca 3  2+  release.  In ECs, the IP R3 3  isoform is most commonly expressed (Mountian et al. 1999). Slightly after or concurrently with IP3R activation, Ca  2+  entry is often facilitated via a variety of channels.  These include the 20  nonselective cation channels (NSCCs) and store-operated Ca  2+  channels (SOCs). Agonists-  induced Ca influx may occur via both NSCCs and SOCs, although the latter also transport Ca 2+  2+  when the ER store is depleted and is more Ca -permeable than NSCCs (Nilius and Droogmans 2+  2001). In some cells, however, there is not a clear distinction between the function of NSCCs and SOCs, as both are activated upon agonist stimulation (Wang and van Breemen 1997). The molecular identities of NSCCs and SOCs vary greatly among species and types of ECs. Transient receptor potential (TRP) channels are proposed as the major pathway via which Ca  2+  enters ECs, and TRP-1 to TRP-6 isoforms have been found in different species (Nilius and Droogmans 2001). A minor endothelial Ca  2+  entry pathway may be via the reverse-mode  Na /Ca exchanger (NCX) (Teubl et al. 1999). +  2+  The NCX and plasma membrane Ca -ATPase (PMCA) are the two main membrane2+  bound transporters that extrude Ca to the extracellular space. The NCX has an affinity to Ca 2+  2+  at K > 1 pM, compared to that of PMCA at K D < 0.5 pM. The K D difference between NCX and D  PMCA provides some insights to their localization and function. The PMCA, although very sensitive to Ca , is not the optimal machinery for Ca removal after agonist stimulation, which 2+  2+  generally results in [Ca ]i of several hundred nanomolars. Most of the elevated Ca 2+  2+  is thus  drawn towards the NCX for extrusion purposes. Because of the relative insensitivity to Ca , 2+  NCX is thought to cluster in parts of the plasma membrane (PM) where there is high subplasmalemmal local [Ca ]i (Philipson 1999). With reference to the superficial buffer barrier 2+  (SBB) theory proposed by van Breemen et al. (van Breemen et al. 1995), effective Ca  2+  sequestration by the ER is only possible when there is continuous Ca extrusion via NCX. Thus, 2+  large amounts of Ca pass from the ER to the NCX in any given period. The restricted space 2+  between the PM and ER, with a width of about 20 nm, is therefore a likely area in the cell with a  21  localized Ca  2+  influences Ca  concentration of a few micromolars.  2+  Indeed, modulation of NCX activity  release from the ER (Paltauf-Doburzynska et al. 1998), suggesting the close  proximity between NCX and the ER. If NCX and ER are located near each other, Ca uptake and release by the ER becomes 2+  important in ensuing that Ca  2+  is properly delivered to the exchanger. The sarco(endo)plasmic  reticulum Ca -ATPase (SERCA) on the ER takes up Ca 2+  2+  at a faster rate than Ca  2+  leaks out  spontaneously (Tran et al. 2000). Two isoforms, SERCA1 and SERCA3, are found in ECs and both are sensitive to blockade by cyclopiazonic acid (CPA) (Mountian et al. 1999). In the presence of CPA, SERCA stops pumping in Ca , and there is a net Ca  2+  causing [Ca ]; increase and activation of SOCs.  entry has also been  2+  2+  Store-operated Ca  2+  loss from the ER,  demonstrated in ECs with the opening of ryanodine receptors (RyRs) (Paltauf-Doburzynska et al. 1998). The presence of RyRs in ECs has been shown implicitly in several reports (Wang et al. 1995; Frieden and Graier 2000; Ziegelstein et al. 1994). These receptors, unlike the unable to elicit recordable [Ca ]i changes in ECs, despite their Ca 2+  2+  IP3RS,  are  releasing properties.  Recently the RyR3 isoform is found in human ECs (Kohler et al. 2001), but other studies have also shown endothelial RyRs having similar functions to the cardiac RyR2 in modulating Ca  2+  oscillations (Jacob et al. 1988; Neylon and Irvine 1990; Laskey et al. 1992). RyRs may have a variety of functions in different ECs. For example, besides having an effect on SOCs, RyR opening also activates Kc channels in human ECs (Frieden and Graier 2000). On the other hand, a  the role of RyRs in removing cytosolic C a from native rabbit ECs will be demonstrated in the 2+  Results Section.  22  1.8. Examples of Interactions Between Endothelial Cells and Myofibroblasts The ultimate goal of finding the link between endothelial Ca  2+  homeostasis and its  influences on the functions of VMFs is largely based on a wealth of information on endothelial cell-smooth muscle interactions.  One of the most investigated topics in cardiovascular  physiology is the regulation of vascular smooth muscle tone by endothelial cells (ECs). A recent example is the use of a bioassay system where ECs act as the donor of secretory agents, and the detection of nitric oxide-, prostacyclin-, and EDHF-mediated contractions in a de-endothelialized vessel (Kuang, et al. 2003). Myofibroblasts, which themselves possess smooth muscle-like contractile properties, are known to interact with various cell types. In the comea, injury to the epithelium results in keratocyte apoptosis mediated by interleukin-1 (IL-1) and tumor necrosis factor-a (TNFa) (Wilson et al. 2003).  The apoptotic events also promote myofibroblast  migration to the site of injury (Mohan et al. 2003), thus indicating potential communicative pathways between epithelial cells and myofibroblasts. Interestingly corneal endothelial cells also secrete IL-1 and TNFa, both of which are key players in the motility of myofibroblasts, suggesting possible interactions with ECs as well (Wilson et al. 1994). In another example, myofibroblasts and ECs lie in proximity in the portal circulation. In the healthy (or quiescent) state, myofibroblasts in the liver are more commonly referred as hepatic stellate cells (Dooley et al. 2000). In liver cirrhosis, the fenestrae between ECs are gradually lost, making diffusion across the endothelial layer more difficult (Ramadori and Saile 2002).  At the same time,  accumulation of cytokines stimulates proliferation and movement of myofibroblasts, in attempts to repair the injured tissue (Knittel et al. 2000). This EC barrier later becomes a basal membrane for the adhesion of more myofibroblasts, thus forming a septum between the hepatocytes and the circulation (Ramadori and Saile 2002). Although not investigated in detail, EC-myofibroblast  23  interactions are thought to partially trigger the series of events in the damaging liver (Ramadori and Saile 2002). Rather than isolating tissues from blood vessels, myofibroblasts faciliate neovascularization in tumor cells. In an ovarian carcinoma cluster, co-culture of ECs has no effects whereas in the presence of myofibroblasts, both cells invade the tumor (Walter-Yohrling et al. 2003). The EC-myofibroblast coupled invasion is prevented by angiogenesis inhibitors (Walter-Yohrling et al. 2003). It is speculated that myofibroblasts secrete growth factors and extracellular matrices that promote contacts with ECs and the migration of both cell types into the tumor (Walter-Yohrling et al. 2003). Yet interactions between ECs and myofibroblasts are not always only implicated in pathological conditions. In valvular transplant, immune responses elicited by the recipient's T-cells against the donor valvular ECs have long been known for their roles in graft rejection (Hengstenberg et al. 1990). A study by Batten et al. shows that although the surface antigens are similar on both valvular myofibroblasts and ECs, only the latter are immunogenic and a proliferation of T-cells is detected (Batten et al. 2001). A co-culture of valvular ECs and myofibroblasts also abolishes the T-cell response, suggesting that VMFs interact with and protect ECs from inducing an immune response (Batten et al. 2001). This finding will likely contribute positively to the design of improved preparative procedures for donor valves. From a developmental point of view, the argument for valvular EC-myofibroblast communication is strengthened by the way the heart tube is formed. The heart tube is the embryonic stage of the vascular system, and two endocardial cushions are believed to have significant roles in the looping of vessels and segmentation of the heart (Mulholland and Gotlieb 1997). The endocardial cushions are where protrusions occur later in development, eventually forming the valves (Moore 1988). In summary, despite limited evidence, interactions between ECs and myofibroblasts play significant roles in multiple areas of medicine.  24  C H A P T E R II: Rationale of Study, Specific A i m s , and Hypothesis As explained earlier, the cardiac valve is made up of mostly endothelial cells and myofibroblasts. Both normal functioning and diseased alterations of the valve likely depend heavily on endothelial cell-myofibroblast interactions.  Myofibroblasts possess contractile  properties, and their interactions with ECs may in part resemble those between smooth muscle and endothelium in the blood vessel. Decades of work has been devoted to the elucidation of signaling mechanisms within the vasculature, but with a significant clinical prevalence of valvular heart diseases, there is pressing need for the study of cardiac valvular cell physiology. Thus, the ultimate goal of research in valvular biology, in connection with the published articles, is to foster further investigation in the underlying causes of valvular heart diseases. In order to achieve this goal, the pharmacology and physiology of the myofibroblast, a major functional constituent of the cardiac valve, must be well understood first.  Unfortunately, information  regarding ionic (e.g. Ca ) signaling mechanisms in valvular myofibroblasts (VMFs) is seriously 2+  lagging behind the research on endothelial cells. Therefore, before designing experiments aiming at resolving myofibroblast-endothelial cell cross-talk in the cardiac valve, attempts are put in to investigate the fundamental signaling properties of VMFs. With that in mind, the first specific aim of this study is developed as follows: Specific Aim #1 Characterization of Plasma Membrane and Endoplasmic Reticular Receptor-Mediated Ca Signaling Pathways in Valvular Myofibroblasts - Identifying 2+  i) Histaminergic & Purinergic Receptor Subtypes and ii) Functional Store-Operated Ca Channels and Ryanodine Receptors 2+  25  The findings from Specific Aim #1 will yield basic but vital knowledge about VMF physiology. In the long run, follow-up studies will enrich the information database of VMFs. Only until then will studies aiming at examining valvular cell-cell interactions achieve their maximal potential, especially since much is already known about endothelial cells (ECs). Interesting enough, with over 100,000 publications ranging from single-cell to whole-tissue studies, there are still knowledge gaps in some areas of Ca ECs.  With growing interests in intracellular Ca  2+  2+  signaling and secretory pathways in  regulation and its correlation with  endothelium-related diseases, it becomes essential to contribute to the full understanding of endothelial Ca  2+  signaling. Ca  2+  homeostasis depends equally on ion influx and extrusion, and  the attention for the second part of this study is drawn to the removal mechanisms of cytosolic Ca  2+  after agonist stimulation of ECs. Freshly isolated ECs are used here since they resemble in  vivo physiology much closer than cultured ECs do. It is also noted that aortic ECs from rabbits are used because of the immense challenge in obtaining healthy human valvular endothelium. In spite of this, the findings here are readily applicable to ECs in general since an earlier publication from our laboratory has found that the physiological characteristics of rabbit valvular ECs (Li and van Breemen 1995) resembled those from the aorta. Having justified the use of freshly isolated aortic ECs, the second specific aim is developed as follows: Specific Aim #2 Elucidation of Ca Extrusion Pathways in Vascular Endothelial Cells 2+  Contribution of Sarco(Endo)plasmic Reticulum Ca -ATPase, Ryanodine Receptor, 2+  Na -Ca +  2+  Exchanger and Plasma Membrane Ca -ATPase 2+  It is evident from the specific aims that two seemingly distantly related research questions are being pursued at the same time. It should be emphasized again that the objective of  26  this study is to innovate further research on both ECs and VMFs, leading to the eventual understanding of the development of valvular diseases.  Keeping the objective in mind, the  working hypothesis also reflects different levels of investigation in both types of cells. With very little being known about VMFs other than their smooth muscle-like contractile functions, it is reasonable to propose that VMFs possess Ca signaling properties similar to those in smooth 2+  muscle. It has long been established that smooth muscle cells respond to vasoactive substances by eliciting [Ca ]i increases and the sources of Ca 2+  extracellular entry.  2+  are from intracellular releases and/or  Thus, this phenomenon of smooth muscle forms the basis of the first  hypothesis: Working Hypothesis #1 Ca mobilization in valvular myofibroblasts is regulated by ER Ca release 2+  2+  and extracellular Ca influx, with varying sensitivities to different agents. 2+  With regards to the endothelial cells, SERCA, NCX and PMCA are all known Ca  2+  transporters involved in removing cytosolic Ca  2+  be confirmed here. NCX, having a low Ca  affinity, is activated by high [Ca ]i and is thus  2+  in other cell types, and their roles in ECs will  probably situated near the ER where the majority of Ca  2+  2+  is. As a result, it is postulated that  SERCA and NCX function in one unit in removing Ca . 2+  Opening of RyR will provide  continual feeding of Ca from the ER to NCX for extrusion. In contrast, PMCA has a high Ca 2+  2+  affinity and will respond to small fluctuations in cytosolic [Ca ]j, apart from influences from the 2+  ER. In summary, the second working hypothesis is formulated as follows: Working Hypothesis #2 Two parallel Ca removal pathways are present in vascular endothelial cells: 2+  one consisting of SERCA, RyR and NCX in series, and the other involving PMCA.  27  C H A P T E R III: M A T E R I A L S A N D M E T H O D S 3.1. Preparation of Valvular Myofibroblasts Human cardiac valves were collected by the Cardiovascular Registry at St. Paul's Hospital, Vancouver, Canada, from explanted hearts obtained at the time of transplantation according to guidelines set forth by the UBC-Providence Health Care Care Research Ethics Board.  A total of five valve specimens (four mitral valves, one tricuspid valve) from five  patients ranging from age 45 to 64 years were used as sources of normal human valvular myofibroblasts (hVMFs). The clinical cause of heart failure was ischemic cardiomyopathy in three of five patients and dilated cardiomyopathy in the remaining two patients. None of the patients were suffering from valvular diseases. Nor were the patients receiving anti-migraine medications which, according to some studies can potentially cause valvular dysfunction. The valvular leaflets used to prepare the cellular preparations were examined by a pathologist and were determined to be grossly normal in that there was neither thickening of tissue nor evidence of calcium deposits. Valves were procured from the explanted hearts as soon as possible after transplantation and stored briefly in cold, sterile medium. A section of the valvular leaflet immediately adjacent to the piece taken for culture was fixed in 10 % neutral-buffered formalin, paraffin-embedded and histochemically stained for microscopic analysis. Only the distal two-thirds of the valvular leaflet was used to extract the hVMFs.  This was done to avoid contamination with cardiac  myocytes positioned toward the base or proximal end of the valve. In addition, valve chordae were removed prior to culture to prevent fibroblast contamination of the cultures. Endothelial cells on the surface of the valve were removed by gentle rubbing on filter paper. The valve tissue was then minced and placed in a sterile container with 1 % Type I collagenase at 37 °C for  28  4 hours. The hVMFs were dissociated from the valve tissue by gentle vortexing, and the celltissue mixture was separated using a 70-pm filter. The hVMFs were small enough to pass through the filter and were collected in Molecular and Cellular Developmental Biology-131 (MCDB-131) medium supplemented with 1.18 g/L sodium bicarbonate, 100 U/mL penicillin, 100 pg/mL streptomycin, and 20 % newborn calf serum. The hVMFs were grown to confluence in an incubator humidified with 95 % O2 / 5 % CO2 at 37 °C. Cell medium was changed every 48 hours. The hVMFs were subcultured for one to two passages to expand cell numbers, aliquoted into cryovials, and frozen in liquid nitrogen for long-term storage. At one week prior to the experiments, hVMFs were thawed and maintained in culture using standard tissue culture techniques. The hVMFs used in this study have undergone four to eight passages in secondary culture. At the time of the experiments, hVMFs were at 70 % confluence, mimicking the loose arrangement of these cells in vivo.  3.2. Preparation of Vascular Endothelial Cells Use of animals was governed by guidelines set forth by the University of British Columbia (UBC) Committee on Animal Care, UBC, Vancouver, Canada. Adult female New Zealand White rabbits weighing between 2.0 to 2.5 kg were sacrificed by CO2 asphyxiation. Pinching and blinking reflexes were checked before any surgical invasion. A surgical blade was used to make a cut at the rabbit's neck, allowing exsanguination via the carotid arteries. The thoracic cavity was cut open after all the blood has been removed from the rabbit. The heart and lungs were removed, exposing the thoracic aorta. A 2-inch segment of the aorta near the distal end was dissected out and immediately placed in warm (37 °C) normal physiological salt solution (nPSS). Using a dissecting microscope (Olympus SZ 30), all surrounding connective and fat tissues of the vessel segment were carefully removed.  29  When the vessel was thoroughly cleaned, it was placed in nominal Ca -free PSS (Ca 2+  z+  free PSS) containing the enzyme solution at 37 °C for 30 minutes. The enzyme solution used for dissociation of endothelial cells consisted of 0.01 % Type IV collagenase, 0.5 % Type I elastase, 1 % bovine albumin, and 1 % trypsin inhibitor. After the enzyme treatment, the vessel was first washed in nPSS a few times and then was placed in antibiotic-containing nPSS (a-nPSS). The a-nPSS consisted of 90 % nPSS, 9.99 % fetal bovine serum, and 0.01 % antibiotic mixture of penicillin, streptomycin and amphotericin B. A Pasteur pipette was used to disperse the endothelial cells by the method of trituration. During trituration, small force was applied to flush solution into and out of the vessel. As a result, clusters of endothelial cells (ECs) were separated from the vessel. The ECs were seeded onto glass-based experimental chambers and were left for attachment at room temperature (23 °C) for 2 hours. All ECs were used within 6 hours after preparation to ensure viability of cells and quality of data.  3.3. Measurements of Intracellular Ca Concentration 2+  3.3.1. Conventional Fluorescence Microscopy  Valvular myofibroblasts (VMFs) and endothelial cells (ECs) in glass-based chambers were loaded with 1 pM of the fluorescent Ca indicator fura-2-acetoxymethylester (fura-2/AM) 2+  and 1 pM pluronic acid (F-127) for 30 minutes at room temperature (23 °C). Figures and show sample images of fura-2-loaded VMFs and ECs. Upon entering the cells, the ester bond of Fura-2/AM is cleaved, trapping the fluorophore in the cytosol. Uncleaved fura-2 or fura-2/AM, i.e. in the ester form, emits maximal fluorescence when excited at 380 nm (Scanlon et al. 1987). As discussed later, Ca -free fura-2 also fluoresce at 380-nm excitation. Thus, fura2+  2/AM in the cytosol does not affect the measurement of net changes in [Ca ]j. Proper cleavage 2+  of ester bonds also prevents penetration of fura-2 into subcellular organelles such as ER and  30  mitochondria. Compartmentalization of fluorescent dyes into organelles present a source of experimental error in [Ca ]j measurements, since fluorescent signals are detected in locations 2+  other than the cytosol. In this study, potential influences from organellar Ca signals are greatly 2+  diminished also because of the relatively low K D (224 nM) of fura-2, compared to other dyes such as mag-fura-2 which, with a high K D of 25 pM, specifically binds to Ca in the ER. The 2+  high Ca  2+  affinity (or low K D ) of fura-2 enables detection of nanomolar changes in C a  2+  concentration in the cytosol. If small amounts of fura-2 are loaded into the ER and mitochondria, the dye would be over-saturated by the concentrated Ca in these compartments and would not 2+  detect changes of Ca levels in these locations. 2+  After the loading period, the chamber was mounted on an inverted microscope (Nikon, Diaphot) with a 20 phase/fluor and an 100* oil-immersion objective and washed with nPSS via x  a solution perfusion system for 15 minutes to remove any fura-2/AM remaining in the extracellular space. Solution was infused into the system via polyethylene tubing. The volume of the chamber was kept constant at 0.5 mL by suction. A total of 3 mL was used during each solution change to ensure that the chamber contained the designated solution only. A l l experiments were performed at room temperature (23°C). The cells were excited with alternating ultraviolet (UV) light of 340 nm and 380 nm at 1second intervals and fluorescence was recorded at the emission wavelength at 510 nm. The 340 nm / 380 nm wavelengths were chosen due to fura-2's fluorescent characteristics. When fura-2 is bound with Ca in the cytosol, maximal fluorescence is emitted when the cell is excited with 2+  340 nm light. On the contrary, maximal light is emitted under 380-nm excitation when fura-2 is free from Ca , i.e. in low [Ca ]j environment. 2+  2+  Thus, cytosolic Ca  2+  levels ([Ca ]i) were 2+  expressed as the fluorescence ratio of the excitation wavelengths: 340 nm and 380 nm (F340/F380).  31  Fluorescence intensities of EC clusters containing 5 to 10 cells were recorded by a PMT fluorimeter (Photon Technology International (PTI), London, ON) coupled to the microscope. The PMT fluorimeter was connected via an interface to a computer, and data were recorded on Felix® Fluorescence Analysis Software v. 1.21 (PTI, London, ON). For the hVMF experiments, the cells were exposed to 340- and 380-nm UV light, and images at 510 nm emission were taken with a digital camera (DVC-1300, Digital Video Camera Company, Austin, TX) that was connected to the computer via an interface. The fluorescence ratio  (F340/F380)  of individual  hVMF (by means of regions of interests (ROIs)) were recorded using the Northern Eclipse® software (Empix Imaging, Toronto, ON). Each ROI included the entire cellular area, with no distinction between cytosolic and nuclear areas. Using the method shown by Grynkiewicz et al. (1985) and the equation: [Ca ]i 2+  = K  D  (R - Rmi )/(Rmax n  R)(Sf38o/S 38o), b  absolute [Ca ]i values 2+  2_j_  were calculated from the maximal and minimal fluorescence values under treatment of the Ca ionophore ionomycin (10 pM) in nPSS and zero Ca  2+  PSS (OCaPSS), respectively. Baseline  [Ca ]i in hVMFs was around 25 nM while a typical agonist (e.g. 100 uM histamine) could elicit 2+  a peak [Ca ]i up to 980 nM. Although it is uncommon to record milli-molar levels of [Ca ]i in 2+  2+  most cells, this has been reported in hVMFs before (Taylor et al. 2000). Baseline [Ca ]i in ECs 2+  was approximately 35 nM and maximal [Ca ]i upon a typical agonist stimulation, i.e. 10 p M 2+  acetylcholine (ACh), could reach close to 760 nM. [Ca ]i values calculated by this method, 2+  however, were subjected to significant experimental uncertainties because the dissociation constant ( K D ) of fura-2 used by Grynkiewicz et al. (1985) corresponds to the dye in solution rather than in endothelial cells. Thus, for the purpose of this study, the fluorescence ratio was not converted to absolute [Ca ]i because of the uncertainty for in situ calibrations (Wang et al. 2+  1995).  32  Figure Image of fura-2-loaded valvular myofibroblasts (VMFs). VMFs were loaded  with the Ca -sensitive fluorescent indicator fura-2 acetoxymethylester (1 uM) for 30 minutes at 23 °C. This image was taken when the VMFs at rest were exposed to 380-nm ultraviolet light. 2+  33  Figure  Image of fura-2-loaded endothelial cells (ECs). ECs were loaded with the  Ca -sensitive fluorescent indicator fura-2 acetoxymethylester (1 uM) for 30 minutes at 23 °C. This image was taken when the ECs at rest were exposed to 380-nm ultraviolet light. +  3.3.2. Rapid Laser-Scanning Confocal Microscopy  Some hVMF experiments were performed using a rapid laser-scanning confocal microscope (LSCM) in order to capture subcellular Ca  2+  signals which occurred in millisecond  intervals. The LSCM consisted of the Olympus BX50WI upright microscope and a Nipkow confocal disc. The pinhole on the confocal disc filters the out-of-focus light and allows for maximal sensitivity of the fluorescence acquisition at a given focal plane. This is especially important in the detection of basal, subcellular Ca  signals that are usually of weaker amplitudes  than global [Ca ], increase elicited by stimuli. The high speed of the LSCM mechanics here 2+  also is an asset to capture [Ca ]j signals occuring rapidly. hVMFs were loaded with the Ca 2+  2+  sensitive fluorescent indicator fluo-4 (1 uM) and Pluronic F-127 (1 pM) for 30 minutes at room temperature (23 °C). Design of the experimental chambers and perfusion system was similar to that described above. A water-dipping 60 objective was used to visualize hVMFs which were x  excited by a Argon-Krypton laser at 488 nm. Images of hVMFs were captured at 525-nm emission, at a rate of 25-30 frames per second by an ICCD (PerkinElmer Olympix) controlled by the Ultraview® 4.0 software (PerkinElmer, NJ). Fluorescent intensities of selected ROIs were recorded on an Excel spreadsheet. 3.4. Mn -Quenching Experiments 2+  The Mn -quenching method was used occasionally to measure the rate of divalent cation 2+  entry (Wang and van Breemen 1997). The cells were exposed to UV light at 360 nm, which is the isobestic point of fura-2, MnCL. (50 pM) in nominal Ca -free PSS (Ca-free PSS) was 2+  perfused into the chamber. Upon entering the cells, M n quenches its fluorescence. The basal M n  2+  2+  binds to the intracellular fura-2 and  entry rate was determined for 200 seconds prior to  the addition of drugs. A more negative slope of fluorescent intensity at 360 nm  (F360)  during  35  stimulation indicates an increased rate of M n  2+  entry, which is a sign of Ca entry under normal z+  circumstances. At the end of each experiment, ionomycin (10 pM) was added to the cells to achieve maximal quenching, at which point the intensity was arbitrarily set as 0 % fluorescence. To express M n entry rate, the unit % F o/second (%F/s) was used. 2+  36  3.5. Fluorescent Labeling of Ryanodine Receptors The fluorescent indicator BODIPY TR-X ryanodine was used to specifically label ryanodine receptors. The cells were loaded with 1 pM BODIPY TR-X ryanodine and 1 p M pluronic acid (F-127) for 30 minutes at 23 °C. After the loading period, the cells were washed with nPSS for 15 minutes to remove any excessive dye remaining in the extracellular space. The chambers were then mounted on an inverted microscope (Nikon Eclipse TE300) with a 60 oilx  immersion objective, coupled to a pinhole confocal scanning head (BioRad Radiance 2000). A krypton laser was used to excite the cells at 589 nm and images were captured with an ICCD at 616 nm. To obtain an image stack for three-dimensional composition later, images were taken at the bottommost focal plane first and moved upward in 0.15-pm steps.  3.6. Data Analysis and Statistics All acquired data were exported to Microsoft® Excel where they were analyzed. Statistical tests were performed using GraphPad® Prism.  In figures where representative  tracings are shown, responses from an individual VMF or an EC cluster were illustrated. Data on line and bar graphs were shown as mean ± standard error of the mean (SEM). Where applicable, one-way AN OVA and Student's t-test were used to determine statistical significance. The Neumann-Keuls post-hoc test was used in cases of overall differences in one-way ANOVA. P values of less than 0.05 (P < 0.05) were considered to be statistically different.  36  3.6.1. Ca  z+  Contents in Valvular Myofibroblasts  When VMFs were stimulated in a Ca -free environment, the recorded Ca 2+  expressed as fura-2 fluorescence intracellular compartments.  F340/F380  ratio) indicated Ca  The amount of Ca  2+  2+  signals (i.e.  mobilized only from  2+  stored in these compartments could be  estimated by calculating the area under curves (AUCs) of the drug-induced [Ca ]i responses. It 2+  must be noted that the AUC may underestimate the true amounts of Ca released from the ER 2+  because the amplitudes of [Ca ]i responses may be suppressed by elevated Ca -activated Ca 2+  2+  2+  removal processes. An example of such is the activation of PMCA by the Ca -calmodulin 2+  complex (Berridge et al. 2003). In this study, enhanced Ca  2+  removal affecting the sizes of  [Ca ]j responses was implicated by [Ca ]j decaying below baseline after stimulation in several 2+  2+  occasions (some examples are illustrated in Figures and In contrast, when Ca  2+  removal was inhibited, as in Figures and, [Ca ]s elevations were much larger. 2+  Despite the shortcoming of using AUC as a measurement of Ca content, this method allows for 2+  a present a way of comparing the apparent sizes of different ER Ca compartments. 2+  Each AUC was the sum of individual sub-AUC in one time unit. A time unit was defined as the time between any two data points, and was assigned to be the height of the sub-AUC. The sub-AUC was in trapezoidal shape, and the lengths of the top and bottom surfaces of the trapezoid were represented by  F340/F380  ratios of each of the two data points. Thus, AUC was  expressed in terms of F 3 4 0 / F 3 8 0 ratio-seconds (Rs). 3.6.2. Spontaneous C a  2 +  Release Rates and Duration in Valvular Myofibroblasts  Two methods were used in the analysis of spontaneous Ca releases in VMFs. First, the 2+  percentage of time each Ca release site's fluorescence intensity spent below baseline (< 0 %) 2+  and at 0-25 %, 25-50 %, 50-75 %, and 75-100 % above baseline within a 30-second period were  37  calculated. The maximal [Ca ]j level achieved in a given cell was considered to be 100 % above 2+  baseline. The data were plotted as a histogram with % above & below baseline on the abscissa and % of 30-second period on the ordinate. The histogram would provide an indicator of the distribution of data under basal, unstimulated conditions and during pharmacological modulation. Taken into account the signal-to-noise relationship and consistency of all data, fluorescence intensities of > 25 % above baseline were further analyzed. Spontaneous Ca  2+  release that resulted in [Ca ]i increases of > 25 % above baseline were termed arbitrarily as 2+  substantial spontaneous Ca  2+  substansital spontaneous Ca  2+  releases in this study.  The peak-to-peak duration of each  release site provided a measurement of the frequencies of Ca  2+  release occurrence. 3.6.3. C a  2 +  Removal Rates in Vascular Endothelial Cells  As mentioned above, the  F340/F380  ratio was used to represent [Ca ]j levels. In order to  group data from different experiments, all  2+  F340/F380  ratios were normalized to the maximal  fluorescence achieved by ACh stimulation in the control experiments, or in the ONa experiments when comparing effects of simultaneous NCX + RyR and NCX + PMCA blockades. The relative rates of [Ca ]i decline were determined by comparing the downstroke of the [Ca ]; 2+  2+  responses measured under different experimental conditions. Two approaches were used to quantify the effects of Ca channel/pump modulators on Ca extrusion. Firstly, by dividing the 2+  2+  discrete normalized [Ca ]i values by time, we obtained instantaneous [Ca ]j decaying rates by 2+  2+  calculating between each data pair. The values were then binned into different groups: 0-5, 5.0110, 10.01-15, 15.01-20, 20.01-40, 40.01-60, 60.01-80, and 80.01-100 % of normalized [Ca ]i 2+  levels (Wang et al. 2002). [Ca ]j declining rates were then plotted against the binned % of 2+  normalized [Ca ]; levels. 2+  Secondly, decaying [Ca ]i responses were fitted with an one2+  38  component exponential decay function of the form y = ae (Wang et al. 2002). The C a m  /+  extrusion rate constants, b, were compared among different experimental conditions. 3.6.4. Three-Dimensional Images of Ryanodine Receptors in Endothelial Cells  Individual x-y slices (in 0.15 pm thickness) of BODIPY TR-X-ryanodine-labeled images of ECs were stacked into a two-dimensional (2-D) projection image using Image J® (National Institutes of Health, MD). The original gray-colored 2-D projection image was assigned with a red color. A duplicate of the 2-D projection image was created, rotated by 6° to the right and assigned with a green color. The two 2-D projection images were superimposed on each other using Adobe Photoshop® and a three-dimensional composite image was generated.  3.7. Solutions and Chemicals The Ca -sensitive fluorescent indicator fura-2/AM, the fluorescent label for ryanodine 2+  receptor BODIPY TR-X ryanodine, and the PMCA inhibitor carboxyeosin were purchased from Molecular Probes Inc. (Eugene, OR). All other drugs and chemicals used in this study were purchased from Sigma Chemical Co. (St. Louis, MO). The solutions used in this study were constituted as follows [in mM] at pH 7.4: 1)  normal physiological saline solution (nPSS): NaCl [126], KC1 [5], MgCl [5], HEPES 2  [10], D-glucose [10], and CaCl [1]; 2  2)  zero Ca PSS (OCaPSS): NaCl [126], KC1 [5], MgCl [5], HEPES [10], D-glucose [10], 2+  2  and EGTA [0.1]; 3)  nominal Ca -free PSS (Ca-free PSS): NaCl [126], KC1 [5], MgCl [5], HEPES [10], and 2+  2  D-glucose [10]; 4)  zero Na PSS (ONaPSS): N-methyl-D-glucamine [126], KC1 [5], MgCl [5], HEPES [10], +  2  D-glucose [10], and CaCl [1]; 2  5)  zero Na -zero Ca PSS (ONaOCaPSS): N-methyl-D-glucamine [126], KC1 [5], MgCl [5], +  2+  2  HEPES [10], D-glucose [10], and EGTA [0.1].  39  C H A P T E R IV: C A  2 +  MOBILIZATION B Y P H A R M A C O L O G I C A L A G E N T S  IN V A L V U L A R M Y O F I B R O B L A S T S (VMFs) - E R C A  2 +  STORES AND MEMBRANE RECEPTORS 4.1. Overview Despite evidence suggesting the importance of VMFs in regulating many of the cellular and molecular processes involved in valvular injury and remodeling, very few pharmacological studies of VMFs have been conducted to date. In one study, epinephrine- and angiotensin IIinduced contractions were examined in isolated rabbit VMFs (Filip et al. 1986). In addition, transient increases in [Ca ]; levels induced by serotonin (Hafizi et al. 2000), endothelin-1, 2+  angiotensin II, and U46619 were shown in human mitral VMFs (Taylor et al. 2000). However, little has been reported on the possible mechanisms involved in Ca signaling in VMFs. 2+  In the following sections, cultured human VMFs were examined with respect to the characteristics of their [Ca ]i responses to histamine, ATP & UTP, and cyclopiazonic acid 2+  (CPA). First, experiments were conducted on normal VMFs. Sample pseudocolored  F340/F380  images of fura-2-loaded VMFs before and after histamine stimulation are shown in Figure 4.1.1. Both histamine and ATP/UTP are important vaso-modulators in healthy and diseased tissues. Identifying the Ca -signaling pathways induced by these two agonists would provide valuable 2+  insights in the understanding of VMF physiology. On the other hand, CPA is a widely used, reversible inhibitor of SERCA, and its use in this study would reveal information regarding the distribution and size of intracellular Ca  stores in VMFs. Finally, a comparative study was done  where VMFs isolated from rheumatic valves were subjected to the above pharmacological agents and their responses were evaluated against those of normal VMFs.  40  Figure 4.1.1. F340/F380 images of fura-2-loaded V M F s before and after histamine 2+ stimulation. As explained in Section 3.3.1, intracellular Ca concentration ([Ca ]j) was 2+  expressed as the ratiometric fluorescent intensity at 340-nm and 380-nm excitation. The original grayscale images were converted to pseudocolored ones with references to the color scale shown in the lower right of each panel. White color represents high [Ca ]j while violet represents low [Ca ]i. The unstimulated VMFs (left panel) had [Ca ]i values towards the lower end of the scale. Upon stimulation with 100 pM histamine (right panel), [Ca ]i elevations were indicated by the color changes of the image. 2+  2+  2+  2+  41  4.2. Results 4.2.1. Comparable [Ca ]i Responses in V M F s Originated from Different Patients 2+  As mentioned in Section 3.1, grossly normal atrioventricular valves from 5 patients diagnosed with ischaemic or dilated cardiomyopathy were used as a source of normal VMFs. Because of the potential biovariability among human tissues, preliminary experiments with selected pharmacological agents were done to determine whether VMFs from different individuals produced similar [Ca ]j elevations upon stimulation. In particular, [Ca ]j responses 2+  2+  elicited by pharmacological agents 100 uM histamine & 100 p M ATP and by the reversible SERCA blocker cyclopiazonic acid (30 pM, CPA) were compared. Representative agonist- and CPA-induced [Ca ]i responses are shown in Figures 2+  to As shown in Figure, a typical histamine response in nPSS consisted of a rapid [Ca ]i 2+  increase followed by decay to baseline within 300 seconds. In most cases, there were  several Ca  2+  oscillations after the initial upstroke until the response eventually died out. The  inset table of Figure shows that peak  F340/F380  ratios elicited by histamine among the 5  valves tested were not statistically different. In Figure, typical CPA-induced gradual [Ca ]i increases in nPSS are shown. In 2+  about half of the VMFs tested, sustained [Ca ]i elevation was observed after several minutes of 2+  CPA stimulation.  In the remaining half, [Ca ]\ returned to baseline eventually.  This  heterogeneity, seen in VMFs from all 5 valves, was probably not due to variability among individual patients. The inset table of Figure shows that peak  F340/F380  ratios of CPA-  induced responses were not statistically different among valves from the 5 patients. Some variations in the ATP-induced [Ca ]j responses were also seen in VMFs from 2+  different origins. ATP increased [Ca ]i to similar maximal values in all VMFs but in some the 2+  42  [Ca ]i decay occurred slowly in the range of minutes. In other VMFs, [Ca ]j elevation was 2+  z+  maintained at a plateau phase with little sign of decay during the ATP treatment. Typical ATPinduced [Ca ]i responses mentioned above are shown in Figure The inset table of 2+  Figure shows that despite the ATP-induced [Ca ]; plateau was not present in all VMFs, 2+  the maximal F340/F380 ratios achieved were not significantly different among the 5 valves. The [Ca ]; responses shown in this section suggested that VMFs demonstrate heterogeneous Ca  2+  signaling upon ATP and CPA stimulation. The heterogeneity in VMF  responses was present in all of the 5 valves tested, and was not a property of any particular individual. Mulholland and Gotlieb (1996) discussed the two morphological states of VMFs in culture. Cultured VMFs may appear in spindle and cobblestone shapes, both of which were seen in this study. In the initial stage of the study, preliminary analysis comparing the two VMF morphologies revealed that shape is not a factor in the heterogeneity of ATP and CPA responses. Despite the noticeable differences in the geometry of [Ca ]j responses, all VMFs showed similar 2+  [Ca  ]i  elevations in their initial responses to the stimulus (i.e. peak  within errors). In the subsequent experiments where the Ca  2+  F340/F380  ratios were close  signaling mechanisms of the  various pharmacological agents were elucidated, only VMFs from 2 of the 5 patients were used.  43  100 pM histamine was applied to a VMF in either normal Ca -containing physiological salt solution (nPSS) (solid trace) or zero Ca PSS (OCaPSS) (dotted trace) for the duration of the response. The inset table shows the peak [Ca ]i levels (expressed in F 3 4 0 / F 3 8 0 ratio) of the histamine responses in nPSS and OCaPSS of VMFs from 5 patients. The average peak values indicated that VMFs from different individuals responded similarly to histamine stimulation, in both nPSS and OCaPSS. Figure Sample histamine-induced  [Ca ]j responses in V M F s . 2+  2+  2+  2+  44  Figure Sample CPA-induced [Ca % responses in V M F s . The sarco(endo)plasmic reticulum C a - A T P a s e ( S E R C A ) blocker cyclopiazonic acid ( C P A , 30 p M ) was applied to V M F s in nPSS. The inset table shows the peak [ C a ] i levels o f V M F s from 5 patients. Heterogeneity o f C P A responses was displayed among V M F s and patients. The solid trace shows the plateau phase o f the response in some V M F s that is absent from other V M F s (dotted trace). In spite o f this, the peak sizes among valves from different patients were generally the same. 2+  2+  45  Figure Sample ATP-induced [Ca ]; responses in V M F s . Adenosine 5'-triphosphate ( A T P , 100 p M ) was applied to V M F s in nPSS. The inset table shows peak [ C a ] i levels o f V M F s from 5 patients. In some V M F s , A T P elicited sustained [ C a ] i elevation (solid trace) whereas in other V M F s , [ C a ] i gradually decayed towards baseline levels (dotted trace). In any case, the average peak values among different valves were equal to each other, suggesting individual biovariability was rather insignificant in generating [Ca ] i responses. +  2+  2+  2+  +  46  4.2.2. Histamine-induced [Ca ]i Increase is Independent of Extracellular Caz+ 2+  Shown in Figure is a sample His-induced [Ca ]j response in OCaPSS 2+  (representative of n = 159). When compared with the response shown in Figure, both histamine responses with and without extracellular Ca characteristics. Blockade of receptor-operated Ca  2+  2+  shared similar upstroke and decay  channels (ROCs) and store-operated Ca  2+  channels (SOCs) with 50 p M SKF-96365 did not alter the shape and time course of the histamine response in nPSS (Figure, representative of n = 68 cells). Areas under the [Ca ]i responses elicited by histamine with and without SKF-96365 were compared and were 2+  not significantly different, ln support of the data that histamine did not induce Ca VMFs, it was also found that fura-2 quenching by M n  2+  2+  entry in  was not increased by histamine  stimulation (data not shown).  47 Histamine-induced [Ca h transient in V M F s in OCaPSS. In the absence of extracellular Ca (i.e. OCaPSS), the histamine (His, 100 uM)-induced [Ca ] response in VMFs (representative of n = 159 cells) was not distinguishable to that in nPSS (Figure Figure  2+  2+  ;  2.5 i  1.5  0.5 -I 0  1  1  1  '  100  200  300  400  Time (seconds)  48  Figure Histamine response of V M F in the presence of SKF-96365. Blockade of  receptor- and store-operated Ca channels by SKF-96365 (SKF) (50 uM), applied for 200 seconds in nPSS prior to histamine stimulation, had no effect on the shape and time course of the histamine response (representative of n = 68 cells). Together with Figure, the data suggested that histamine did not induce Ca entry, and only elicited [Ca2+n ]i increase via 2+  2+  l+  2_|_  activating intracellular Ca release.  SKF-96365 Histamine  o oo . _  £ 1.5 to  0.5 0  100  200  300  400  500  600  Time (seconds)  49  4.2.3. Evidence for Hi Receptor-Mediated C a  z +  Signaling in V M F s  Selective receptor antagonists were used to identify the subtypes of histamine receptors in VMFs.  Pyrilamine (selective Hi antagonist, 0.1 uM) completely abolished the histamine-  induced [Ca ]i response (Figure, representative of n = 77 cells). After 20 minutes of 2+  continuous washout in nPSS, the antagonizing effect of pyrilamine was reversed, as shown by the second histamine response in Figure Knockout of H 2 receptor function, however, did not alter the histamine-induced [Ca ]; response in any way. 2+  Figure shows a  representative trace of n = 74 VMFs under histamine stimulation, before and after the incubation of cimetidine (selective H 2 antagonist, 1 pM).  50  Figure  Effects of pyrilamine on histamine-induced [Ca ]; response in V M F s .  Pyrilamine (Pyr) (0.1 pM), a selective H i antagonist, completely abolished the histamine (His, 100 pM)-induced [Ca ]i response in nPSS (representative of n = 77 cells). The Hi blockade was reversible after 20 minutes of continuous perfusion with nPSS. 2+  51  Figure  Effects of cimetidine on histamine-induced  [Ca ]j response in V M F s . 2+  Cimetidine (Cim) (1 uM), a selective H antagonist, did not alter the histamine (His, 100 uM> induced [Ca ]j response (representative of n = 74 cells). This suggested that no functional H receptor-mediated Ca signaling is present in VMFs. 2  2+  2  2+  2.5 Cim His  His  o oo  2H  co  co  1.5  o  200  400  600  800  1000  Time (seconds)  52  4.2.4. E R C a  2 +  Refilling is Essential in Regenerative Histamine Responses  Two histamine stimulations in nPSS at 15 minutes apart produced consistent  [Ca ]i 2+  responses in VMFs, as illustrated in the representative trace of n = 78 cells in Figure The slight run-down effect, i.e. gradually diminishing responses after repetitive histamine stimulations in VMFs, was observed at times. Incomplete refilling of Ca into the ER and, to a 2+  lesser extent, receptor desensitization are possible causes for the run-down effect. In the absence of extracellular Ca , i.e. in OCaPSS, however, VMFs did not respond to the second histamine 2+  stimulation (Figure, representative trace of n = 66 cells). Based on the different results from nPSS and OCaPSS, it appears that refilling of the ER with Ca  2+  derived from the  extracellular space is essential for repetitive histamine responses. When VMFs were treated with the reversible SERCA blocker cyclopiazonic acid (CPA, 30 pM), [Ca ]i oscillations that usually followed the initial peak of a histamine response was 2+  abolished (Figure, representative of n = 58 cells). In this figure, the CPA and histamine responses can be distinguished by their kinetics. CPA caused an initial slow [Ca ]; increase. Subsequent application of histamine induced a more rapid [Ca ]i upstroke. In addition, the rapid [Ca ]i decay of the histamine response was different from the shoulder phase of the response 2+  attributed to CPA stimulation.  In the continuous presence of CPA, a second histamine  application failed to elicit [Ca ], elevation. In total, findings in this section suggested that a 2+  single pulse of histamine depletes ER Ca  2+  that depends on SERCA activity for replenishment  and for subsequent responses.  53  Figure Regenerative histamine responses in V M F s . Histamine (His) (100 uM) was  applied twice, 15 minutes apart, in nPSS (representative of n = 78 cells).  Figure  Second histamine application did not elicit a response in OCaPSS.  Histamine (His) (100 uM) was applied twice, 15 minutes apart, in OCaPSS (representative of n = 66 cells). Only the first stimuulation resulted in [Ca ]; increase. 2+  0.5 0  500  1000  1500  2000  Time (seconds)  55  Figure S E R C A blockade abolished regenerative histamine responses in V M F s . 30  pM cyclopiazonic acid (CPA), which elicited a slow [Ca ]j increase (shown between the dotted vertical lines) by inducing Ca release from the ER via SERCA blockade, was added 100 seconds prior to the first histamine (His) (100 uM) application in nPSS. With CPA present throughout the experiment, the second His application did not induce a Ca response (representative of n = 58 cells). Prolonged incubation with CPA revealed a small maintained [Ca ]i elevation above the dashed line, which denotes resting [Ca ]j. Upon removal of CPA, [Ca ]i returned to baseline. 2+  2+  2+  2+  2+  2+  56  4.2.5. Histamine-Insensitive Ca  Release from the E R  z+  Despite the failure to elicit repetitive histamine-sensitive [Ca ]j responses in OCaPSS, 2+  CPA was still able to induce a [Ca ]i transient, as shown in Figure (representative of n = 2+  112 cells). Here 5 minutes of washout (instead of 15 minutes as in previous experiments) were allowed in between histamine applications to minimize undesirable effects due to prolonged incubation in a Ca -free environment. As a control for possible receptor desensitization, VMFs 2+  were repeatedly stimulated with histamine in nPSS. Figure shows that histamine induced [Ca ]j responses in repeated stimulations in nPSS (representative of n = 80 cells), indicating that 2+  the lack of subsequent histamine responses in OCaPSS (Figure was the result of a depleted ER Ca store. After emptying the histamine-sensitive ER Ca content, additional ER 2+  2+  Ca release activated by CPA was likely related to a portion of the ER insensitive to histamine 2+  induced signaling cascades, i.e. generation of IP3 and opening of IP3 receptors. This histamineinsensitive ER compartment is probably also free of or possess only sparse amount of ryanodine receptors, since no [Ca ]i response was seen when caffeine (activator of ryanodine-mediated ER 2+  Ca release channels, 20 mM) was added to VMFs (data not shown). 2+  57  Figure Histamine-insensitive E R Ca  compartment in V M F s . After three histamine  (His) (100 uM) applications to completely deplete the histamine-sensitive C a store in OCaPSS, 30 p M C P A induced an additional transient [Ca ]i response (representative of n = 112 cells). 2+  2+  58  These traces were obtained in nPSS (representative of n = 80 cells), as opposed to OCaPSS in the previous figure. The fact that a [Ca ]; response was seen here with each histamine (His) (100 pM) stimulation indicated that receptor desensitization did not explain the lack of responses to second and third application of histamine in Figure Figure A control experiment showing 3 histamine responses in V M F s . 2+  2.5  n  His  His  His  2\  1 -I 0  ,  ,  ,  ,  500  1000  1500  2000  Time (seconds)  59  4.2.6. Two Compartments of E R Ca"* Stores in V M F s  It is clear from the data in Section 4.2.5 that there are histamine-sensitive and histamineinsensitive ER Ca stores in VMFs. As mentioned in Section 3.6.1, area under curves (AUCs) 2+  of histamine- and CPA-induced [Ca ]i responses were calculated to determine the sizes of the 2+  two ER Ca  2+  compartments.  In Figure, CPA revealed the histamine-insensitive ER Ca store after the VMFs were subjected to OCaPSS for 1400 seconds. In order to compare the size of the histamineinsensitive store with the histamine-sensitive store, VMFs must be exposed to OCaPSS for the same duration prior to the addition of histamine (Figure, representative trace of n = 69 cells). The initial OCaPSS treatment in Figure allowed direct comparison of histaminesensitive and histamine-insensitive ER Ca contents in the existing protocol because basal Ca 2+  2+  loss was taken into consideration. Similarly, after subtracting basal Ca loss, the sum of the two 2+  Ca compartments was represented by the AUC of the CPA-induced [Ca ]; response in Figure 2+  2+ (representative trace of n = 62 cells). Values of AUCs from Figures, and are as follows. The unit of AUC is expressed as F 3 4 0 / F 3 8 0 ratio-seconds (Rs) (as described in Section 3.6.1). The size of the histamine-sensitive ER Ca  2+  compartment was 66.30 ± 2.48 Rs. The size of the histamine-  insensitive compartment was 57.45 ± 4.63 Rs. The experimentally derived size of both Ca  2+  compartments was 93.45 ± 11.34 R s - this value was comparable to the arithmetic sum of 66.30 ± 2.48 R s and 57.45 ± 4.63 Rs, which equals 123.75 ± 7.11 Rs, within statistical error. The sizes of ER Ca lost ER Ca  2+  2+  compartments calculated thus far were valid after VMFs basally  in OCaPSS for 1400 seconds. It must be noted that the protocol design for the  purpose of the findings here makes the extended OCaPSS treatment inevitable. To precisely  60  determine the sizes of ER Ca stores in normal conditions, the amount of basal Ca loss in the 2+  2+  experiments shown in Figures, and was also calculated. Figure shows a sample trace of CPA-induced [Ca ]i response in OCaPSS (with only 100 seconds of 2+  OCaPSS pre-incubation) in n = 55 cells. The 100-second OCaPSS treatment was standard in all Ca -free experiments and its purpose was to ensure complete chelation of any free Ca 2+  extracellular space by EGTA, thereby eliminating possible Ca  2+  2+  in the  influx. The AUC of Figure was 126.12 ± 4.63 Rs, which represented the actual total ER Ca  2+  content, i.e. the total  ER Ca content without the effect of basal Ca loss. Expressing the AUC of Figure as a 2+  2+  percentage of 126.12 ± 4.63 R s (AUC of Figure would notice that 25.9 ± 19.6 % of Ca  2+  was lost from the ER basally during the long OCaPSS treatment in the protocol. Knowing the amount of non-stimulated Ca loss, it was possible to extrapolate the actual Ca content in each 2+  2+  compartment by adding a basal loss factor of 25.9 ± 19.6 % to the AUCs of Figure and Thus, the sizes of the revised Ca contents were: 89.47 ± 17.54 R s for the histamine2+  sensitive compartment and 77.53 ± 15.20 R s for the histamine-insensitive compartment. The relative Ca distribution in the two ER compartments is shown in Figure In summary, 2+  assuming basal Ca loss occurs at equal rates from both ER Ca stores, the histamine-sensitive 2+  2+  compartment makes up 53.6 % of total ER Ca , and the histamine-insensitive compartment 2+  makes up the remaining 46.4 %.  61  Figure  Histamine-sensitive E R C a  z +  content in V M F after basal C a ^ loss.  In  consideration of the basal ER Ca loss due to extended period of incubation in OCaPSS (as shown in Figures and, an experiment was done where histamine (His) (100 pM) was applied to VMFs that had been sitting in the absence of extracellular Ca for the same amount of time (representative of n = 69 cells). The area under curve (AUC), as explained in Section 3.6.1, was calculated from the histamine response, and constituted to the size of the histamine-sensitive ER Ca compartment after basal Ca loss. 2+  2+  2+  2.5  2+  -i  62 Total E R C a content in V M F s after basal E R C a loss. Similar to Figure, VMFs were first incubated in OCaPSS for 1400 seconds (representative of n = 62 cells). Based on Figure, cyclopiazonic acid (CPA) (30 pM) was able to deplete the entire ER Ca store. Thus, CPA was applied to VMFs here, and the AUC represented the size of the histamine-insensitive ER Ca compartment after basal Ca loss. Figure  2 +  2  2+  2+  2.5  2+  1  63  Figure  Actual E R C a  2 +  content in V M F s (without basal E R C a.2+" loss). z  The  cyclopiazonic acid (CPA, 30 uM)-induced [Ca ]i response obtained without the prolonged OCaPSS incubation represented the total Ca released from the ER (representative of n - 55 2+  2+  2"F  cells). The AUC of this response was the size of the actual ER Ca  content.  2.5  o oo  CPA  C O  o «* CO  1.5  0  500  1000  1500  2000  Time (seconds)  64  Figure Relative sizes of E R C a compartments in V M F s . The sizes of the histamine-sensitive and histamine-insensitive ER Ca compartments were expressed as a percentage of the total Ca content. The two compartments were about the same size within statistical error in a total of n = 112 cells subjected to the protocol illustrated in Figure 2+  2+  80  *- 60 c  a>  40 -  a-  20  0 Histamine-insensitive  Histamine-sensitive ER C a  2+  compartments  65  4.2.7. Activation of C a  2 +  (and M n ) Entry by S E R C A Blockade 2+  It was shown in both Figures and that CPA stimulation could induce maintained [Ca ]j elevation in VMFs. The [Ca ]j plateau suggested continuous Ca influx due 2+  2+  2+  to opening of SOCs. This speculation was further supported by the data in Figure (representative of n = 48 cells), where addition of extracellular Ca in place of OCaPSS in the presence of CPA caused a maintained [Ca ]i increase above the resting level (shown by the 2+  dotted line). It is also noted that when VMFs were treated with CPA for over 10 minutes, [Ca ]i 2+  eventually went below the baseline in most cases. This was due to removal of basal Ca  2+  influx  into the cell, and VMFs incubated in OCaPSS also showed a slightly depressed baseline [Ca ]i (n 2+  = 37 cells, data not shown). Effects of SERCA blockade were also determined using the Mn -quenching method. In 2+  56 of 75 cells tested, CPA increased the rate of M n  2+  entry significantly (Figure As  described in Section 3.4, the Mn -influx rate was expressed in terms of % F36o/second (%F/s). 2+  Basal Mn -influx rate was determined to be 0.0227 ± 0.0037 %F/s. M n 2+  2+  influx was increased  to a maximum of 0.0587 ± 0.0034 %F/s, i.e. a 260 % increase, after 300 seconds of CPA treatment. M n  2+  influx remained faster than baseline for at least another 300 seconds. The bar  graph in Figure compares the M n influx rates at different time points. 2+  66  Store-operated Ca entry demonstrated by restoring extracellular Ca after the initial Ca release by 30 pM cyclopiazonic acid (CPA) in OCaPSS (representative of n = 48 cells). The elevated [Ca ]i was maintained until the removal of CPA. The dashed line shows resting [Ca ]i level. Figure Store-operated C a 2+  entry in V M F s . 2+  2+  2+  67  Figure Store-operated divalent cation entry in V M F s .  The manganese-quenching method was used here to monitor M n entry from the extracellular space. Fluorescent intensities at 360 nm, which is the isobestic point of fura-2, were recorded. Manganese chloride (Mn) (50 u\M) was present throughout the experiment. 30 pM cyclopiazonic acid (CPA) accelerated M n influx, as shown by the increased negative slope of the trace, compared to the basal M n influx rate (dashed line) (representative of n = 56 cells). Maximal quenching was obtained with the addition of ionomycin (Ion) (10 )iM). 2+  2+  2+  68 M n entry rates before and after CPA addition to V M F s . The rate of M n entry was calculated from the experiment illustrated in Figure In a total of n = 56 cells, M n entry rate increased by a maximum of 257 ± 22.5 % (mean ± SEM) after addition of CPA for 300 seconds. M n influx was maintained for a total of 600 seconds in the presence of CPA. (*P < 0.05 compared to basal M n entry rate. P < 0.05 compared to M n influx rates at 0 and 600 seconds.) Figure  2+  2 +  2+  2+  2+  0.07 _  T3  #  2+  * #  0.06 -{  C  o  o u 0.05 o  CO co  C  0.04  H  (0  O 'SE 0.03  +  CN  n  E = 0.02 H  — 0.01 0 0  300  600  Time after CPA treatment (seconds)  69  4.2.8. [Ca ]i Responses Elicited by A T P and U T P z+  After resolving the two ER Ca  compartments in VMFs, it was further tested if the  histamine-sensitive Ca store is also responsive to other agonists that mobilize intracellular Ca 2+  via the IP signal transduction pathway.  2+  Purinergic receptor agonists, ATP and UTP, were  3  applied to VMFs to monitor [Ca ]; changes. ATP (P2 agonist, 100 pM) induced a longer-lasting 2+  [Ca ]j increase in nPSS than in OCaPSS (Figure, representative of n = 203 cells). 2+  Similarly, application of UTP (selective  P Y2 2  agonist, 100 pM) also resulted in [Ca ]j increase 2+  with longer duration in nPSS than in OCaPSS (Figure, representative of n = 78 cells). Qualitatively the wider [Ca ]i responses in the presence of extracellular Ca 2+  2+  indicated the role  of Ca influx during ATP/UTP stimulation. 2+  70  Figure ATP-induced [Ca ]j responses in V M F s with and without extracellular  C a . 100 uM adenosine 5'-triphosphate (ATP) induced a longer-lasting [Ca ]j response in nPSS than in OCaPSS (representative of n = 203 cells). The data suggested ATP-induced Ca influx in VMFs. 2+  2+  2+  0  100  200  300  400  500  Time (seconds)  71  Figure  UTP-induced [Ca ]j responses in V M F s with and without extracellular  C a . 100 u M uridine 5'-triphosphate (UTP) induced a longer-lasting [Ca ]j response in nPSS than in OCaPSS (representative of n = 78 cells). The data suggested UTP-induced C a influx in VMFs. 2+  2+  2+  0  100  200  300  400  500  Time (seconds)  72  4.2.9. C a  2 +  Influx Component of A T P - and UTP-Induced [Ca' ]i Responses +  Two methods were used to reveal the Ca -influx component of the ATP/UTP-induced 2+  [Ca ]i responses in VMFs. Treated with the ROC/SOC blocker SKF-96365 (50 uM), ATP2+  induced [Ca ]i increase decayed faster than control (Figure, representative of n = 47 2+  cells). The time required for the peak [Ca ]i level to decay to 50 % of the peak (t o) was 2+  5  calculated. According to the bar graph in Figure, t o was 73.3 ± 5.7 seconds for the 5  control (i.e. without SKF-96365) ATP-induced [Ca ]j response. 2+  The t o was significantly 5  shorter when Ca influx was blocked with SKF-96365, which was 48.0 ± 6.8 seconds. 2+  Secondly, Mn -quenching experiments were conducted as described in Section 3.4. 2+  Figure shows representative traces of Mn -quenched F 6o values during stimulation of 2+  3  VMFs with ATP (n = 90 cells), UTP (n = 146 cells), and UTP + SKF-96365 (n = 79 cells). In Figure, both lines [b] ATP and [c] UTP traces showed accelerated M n  2+  entry rates, as  illustrated by the faster F 6o decay when compared to the basal rate [a]. The dotted UTP + SKF3  96365 trace showed slower F 6o decay than the basal rate, suggesting that both UTP-stimulated 3  and basal M n  2+  influx was inhibited. M n  2+  influx rates were also calculated (as described in  Section 3.4) for the various experimental conditions (Figure The M n  2+  entry rate of  0.0374 ± 0.0011 %F/s at baseline was significantly increased to 0.0471 ± 0.0015 %F/s and 0.0530 ± 0.0019 %F/s during ATP and UTP stimulation, respectively. When M n abolished with SKF-96365, the rate of M n  2+  2+  influx was  entry was 0.0170 ± 0.0014 %F/s, significantly  slower than the basal rate of 0.0374 ± 0.0011 %F/s.  73  Figure Effect of SKF-96365 on ATP response in V M F s . Abolition of Ca  influx by SKF-96365 (50 uM) treatment shortened the duration of the ATP-elicited [Ca ], response in nPSS (representative of n = 47 cells). 2+  74  Figure Time taken for A T P (+/-SKF-96365)-induced [Ca ], response to decay by half. The data represented in Figure were compared with respect to t5o, which is the time 1  needed for [Ca ]; to decrease 50 % from the peak. In a total of n = 47 cells, tso was shorter when VMFs were treated with SKF-96365 during ATP stimulation. (* P < 0.05 vs. ATP) 2+  75  Figure M n quenching data of A T P / U T P application to V M F s . Basal MrT entry rate was indicated by the dotted line [a]. Stimulation of V M F s with either A T P (100 uM) (representative of n = 90 cells) and UTP (100 pM) (representative of n = 146 cells) accelerated the rate of M n entry [b, c]. In the presence of SKF-96365 (SKF) (50 pM), M n entry was reduced (representative of n = 79 cells). 2 +  2 +  0  2 +  100  200  300  400  500  Time (seconds)  76  Figure M n  entry rates under basal and ATP/UTP-stimulated conditions. MrT  entry rates from the data represented in Figure were calculated. Both ATP (in a total of n = 90 cells) and UTP (in a total of 146 cells) treatments significantly increased M n entry rates. On the contrary, SKF-96365 together with UTP (in a total of n = 79 cells) resulted in very little M n entry, the amount of which was even below the basal level. (* P < 0.05 vs. all bars) 2+  2+  77  4.2.10. More Evidence for P v2 Receptor-Mediated C a 2  / +  Signaling in V M F s  In Section 4.2.8, [Ca ]i responses elicited by the selective P y agonist UTP and the non2+  2  2  selective P agonist ATP were shown to have similar shapes and time courses. However, it is 2  still possible for the presence and subsequent activation of P YI receptors when they are 2  stimulated preferentially with ADPPS or 2-Me-S-ATP, both of which are selective P YI agonists. 2  As illustrated in the representative traces of Figures and, VMFs did not respond to either 100 pM ADPPS (n = 68 cells) or 100 pM 2-Me-S-ATP (n = 77 cells). To ensure viability of cells, VMFs were subsequently challenged with 100 pM ATP and [Ca ]; increases 2+  were observed.  78  Adenosine 5'-0-(2to VMFs. No [Ca ]; increase was observed (representative of n = 68 cells). ATP (100 pM) was applied afterward to ensure viability of the cells.  Figure Lack of [Ca ]i response under ADPpS stimulation. thio-diphosphate) (ADPPS) (100 pM), a selective P i agonist, was applied 2+  2+  2 Y  2.5  o oo CO  y-o  1.5  •<*  CO  LL  1^  0.5 0  100  200  300  400  500  600  700  Time (seconds)  79  Figure Lack of [Ca % response under 2-Me-S-ATP stimulation. 2-methyl-thio-  adenosine 5'-triphosphate (100 pM), another selective P2Y1 agonist, was applied to VMFs. Same as in Figure, no [Ca ]i increase was observed with P YI stimulation by 2-Me-S-ATP (representative of n = 77 cells). A T P (100 pM) was applied afterward to ensure viability of the cells. 2+  2  2.5 ATP  2-Me-S-ATP  o co CO  o  1.5  CO  1-  0.5 "I 0  1  1  1  1  1  100  200  300  400  500  1  600  1  700  Time (seconds)  80  4.2.11. Sizes of Histamine- and ATP/UTP-Sensitive E R C a ^ Stores  Having identified the histaminergic and purinergic receptor subtypes and the presence of separate ER Ca  2+  compartments in VMFs, the next step was to determine if the histamine- and  ATP/UTP-sensitive Ca  2+  stores are inclusive of each other. As shown earlier in Figure,  after exhausting the histamine-sensitive Ca additional Ca  2+  from the ER.  2+  store, CPA was able to activate the release of  Experiments were done where ATP was added after histamine  could no longer induce an [Ca ]; increase (Figure, representative of n = 102 cells). The 2+  purpose of these experiments was to investigate whether ATP and histamine share the same ER Ca  2+  compartment. Based on the data in Figure, ATP did not stimulate additional ER  Ca  2+  release after the abolition of the histamine response in OCaPSS, but application of CPA  afterward still induced a [Ca ]j response. Since both histamine and ATP induced intracellular 2+  Ca  2+  mobilization via activation of IP3RS, the CPA-induced [Ca ]j response in Figure 2+  can be further characterized as Ca  release from an IP3-insensitive ER Ca  2+  Using the same logic, the histamine-sensitive Ca  2+  Ca  2+  2+  compartment.  compartment described in Section 4.2.5  should more precisely be called the HVsensitive ER Ca It is now clear that the ER Ca  2+  compartment.  releasable by histamine is inclusive of the ATP-sensitive  store. The question remains whether repetitive ATP stimulation is able to deplete the entire  IP3-sensitive C a  2+  store, making subsequent histamine-induced [Ca ]j responses impossible. As 2+  shown in Figure (representative of n — 39 cells), after repeated ATP stimulations, application of histamine induced further ER Ca release from the IP -sensitive store. 3  2+  release.  ATP only stimulated partial Ca  2+  Therefore, despite both ATP and histamine are IP3-  mobilizing agents, only the latter was able to deplete the entire nVsensitive ER Ca  store.  81  Figure ATP and histamine shared the same E R C a compartment. Histamine (His) (100 uM) was applied for three times in order to deplete the histamine-sensitive ER Ca store. Subsequent application of adenosine 5'-triphosphate (ATP) (100 pM) failed to elicit a [Ca ]i response, suggesting that ATP and histamine, both IP -mobilizing agents, shared the same IP -sensitive Ca store (representative of n = 102 cells). Treatment of cyclopiazonic acid (CPA) (30 pM) stimulated Ca release from the IP -insensitive Ca2+ store. 2 +  2+  2+  3  2+  3  2+  ZT  3  2 His | ATP  His  His  1.8  CPA  1.6 co  ^1.4 CO  1.2 1 0.8 o  500  1000  1500  2000  2500  Time (seconds)  82  VMFs were first repeatedly stimulated with adenosine 5'-triphosphate (ATP) (100 pM) until [Ca ]i increases were no longer present (representative of n = 39 cells). Application of histamine (His) (100 uM) afterward induced additional ER Ca release. The data suggested that although histamine and ATP shared a Ca2+ compartment, the latter only partially depleted the Ca in that store. Figure Partial E R C a  2 +  emptying by A T P .  2+  2+  2+  2 1.9  His ATP  His  CPA  1.8 1.7  0  500  1000  1500  2000  2500  3000  Time (seconds)  83  4.2.12. Selected Parameters of Ca  i+  Signaling in Normal and Rheumatic V M F s  The data presented so far only dealt with VMFs isolated from grossly normal cardiac valves. It would be of interest to make a cursory comparison between some Ca -signaling 2+  properties in VMFs from normal and diseased valves. As indicated in Section 1.3, one of the most common valvular abnormalities is rheumatic valvular disease. In this part of the study, VMFs from 6 rheumatic and 5 normal valves were evaluated based on their responsiveness to pharmacological agents. In particular, peak [Ca ]i values (or peak 2+  F340/F380  ratios) and AUCs of  the histamine, ATP, and CPA responses were measured. For the CPA experiments, the [Ca ]i 2+  plateau was also compared between normal and rheumatic VMFs because SOC activity is implied when elevated [Ca ]; persists during SERCA blockade. 2+  Tables lists all the data and findings. In the table, experiments done in nPSS were indicated by "+Ca " and those done in OCaPSS were indicated by "-Ca ". In normal 2+  2+  VMFs, histamine did not induce Ca  2+  influx (see Section 4.2.2). This finding was confirmed  here by the equal AUCs in Ca -containing and Ca -free environments. In OCaPSS, the AUC 2+  represents the total amount of Ca  2+  2+  release from the ER whereas in nPSS, the AUC is equal to  the sum of Ca release and Ca influx. Thus, if the AUCs in nPSS and OCaPSS are the same, 2+  no Ca  2+  2+  influx is present, as in the case with histamine stimulation in normal VMFs.  In  rheumatic VMFs, however, the AUC in nPSS was significantly larger than that in OCaPSS, suggesting Ca influx elicited by histamine in diseased cells. 2+  Data in Section 4.2.9 showed that ATP induced Ca  2+  influx in normal VMFs. Also  shown in Table, the ATP AUC in nPSS was significantly larger than that in OCaPSS. The AUC difference was also detected in rheumatic VMFs. Moreover, in nPSS, the AUC of rheumatic VMFs tended to be larger than the normal VMFs (P = 0.187). Thus, rheumatic VMFs  84  may have stronger Ca  2+  influx machinery than normal VMFs, although the small sample size  could not reveal the difference here. According to Table, for either histamine or ATP responses, the peak sizes were not different between normal and rheumatic VMFs with or without extracellular Ca . However, 2+  CPA in OCaPSS elicited a significantly smaller peak than in nPSS. The CPA AUC in OCaPSS was also smaller than in nPSS. As a result, CPA differed from histamine or ATP in that the SERCA blocker induced Ca  2+  influx before the [Ca ]; response reached the peak. 2+  On the  contrary, both histamine (in rheumatic VMFs) and ATP (in both normal and rheumatic VMFs) induced Ca  2+  influx only after the [Ca ]; reached the maximum, as demonstrated by AUC 2+  differences and peak size equalities. Similar to ATP, CPA induced slightly more Ca rheumatic VMFs (P = 0.0734) than in normal VMFs. The stronger Ca  2+  2+  influx in  influx may in part be  associated with the marginally higher plateau level in rheumatic VMFs (P = 0.241).  85  Table  Comparison of histamine-, A T P - , and CPA-elicited [Ca ]; responses in  normal and rheumatic valvular myofibroblasts.  The table lists mean ± SEM values from  experiments on VMFs from 5 normal and 6 rheumatic valves.  Peak Level  Histamine Normal Rheumatic +Ca -Ca  2+  2 +  Area Under Curve  Plateau Level (% Peak)  # P tP j P &P  +Ca  -Ca  2+  2 +  CPA  ATP Normal  Rheumatic  Normal  Rheumatic  1.19 ± 0.10  1.16 ± 0 . 0 9  0.84 ± 0.05  0.84 ± 0 . 1 4  0.59 ± 0 . 0 9  0.76 ± 0 . 1 0  1.13 ± 0 . 1 0  1.19± 0.07  0.86 ±0.11  0.91 ± 0 . 1 4  0.39 ±0.04*  0.44 ± 0.08*  79.89 ± 6 . 8 8  90.47 ± 3 . 8 2  86.17 ± 1.07  86.79 ± 17.39  54.89 ±6.75*  39.68 ± 0.60*  ^fcli^liWlBiii  iiiiiiiiiiisliil iiliiiiiiiliiss IllBllSllllSlli  137.49 ±28.54  129.45 ± 2 2 . 2 3  79.38 ± 14.71  103.51 ± 2 0 . 9 5  112.6 ±28.52  96.66 ±20.77*  65.83 ± 14.14*  61.69 ± 12.11  #  T  &  < 0.05 vs. +Ca values; = 0.187 vs. Normal; = 0.0734 vs. Normal; = 0.241 vs. Normal l  86  4.2.13. Spontaneous C a  i +  Release in V M F s  In a small number of VMFs, spontaneous Ca any application of drugs. Subcellular Ca  2+  2+  (spCa ) releases were observed without 2+  signals from individual Ca release sites were visible 2+  using rapid scanning laser confocal microscopy. A total of 101 subcellular Ca release sites from 10 unstimulated VMFs were analyzed. These VMFs were treated with either 15 mM caffeine or 100 pM ryanodine because of their potential actions on ryanodine receptors (RyRs), which mediate Ca sparks in both cardiac and smooth muscles. Sample time-lapsed images of fluo-4-loaded VMFs displaying subcellular Ca signals are shown in Figure 2+  In Figure, sample traces of spontaneous [Ca ]; signals from one subcellular Ca 2+  release site in a VMF are shown. Spikes of Ca  2+  2+  release were present in the basal condition,  whereas spCa release was abolished during caffeine treatment. Figure shows sample 2+  traces from another spCa release site of a different VMF. The basal spCa release patterns 2+  2+  were similar in both Figures and However the baseline [Ca ]i level was 2+  depressed when VMFs were treated with ryanodine. The histogram in Figure shows the time distribution of [Ca ]i levels as a function of the baseline as described in Section 3.6.2. During the 30-second period when data were analyzed, [Ca ]j levels were near or below baseline (i.e. < 25 % above baseline) for over 2+  90 % of the time. Compare with the unstimulated condition, when VMFs were treated with RyR modulators (caffeine or ryanodine), significantly more data fell below the baseline - 63 % (unstimulated) vs. 98 to 99 % (modulated RyR). For approximately one-third of the 30-second period, [Ca ]; levels were < 25 % above baseline in the basal condition, compared to only 0.5 2+  1.6 % of data during caffeine or ryanodine treatment. Thus, a generally depressed [Ca ]i  87  baseline was observed when RyR activity was modulated, although caffeine may also suppress IP R activity. 3  The bar graph in Figure compares the peak-to-peak time between spikes of Ca  2+  releases. Under basal condition, the average latency period between Ca release peaks was 6.37 2+  ± 0.30 seconds.  When treated with ryanodine, the time between Ca  2+  release peaks was  significantly increased to 9.01 ±2.14 seconds. The ryanodine treatment data clearly showed that RyRs regulate spontaneous Ca  2+  releases in VMFs.  The suppression of spontaneous Ca  releases by caffeine, which has dual actions on RyRs and  IP3RS,  2+  suggested possible roles of  IP Rs in generating subcellular [Ca ]i signals that can only be confirmed with more extensive 2+  3  studies.  88  Figure Pseudocolored tluo-4-loaded V M F images showing various spontaneous 2+ C a (spCa ) release sites recorded over time. The top and bottom panels show spCa 2 +  2+  releases of two different VMFs. The VMFs here were not stimulated and were viewed under a rapid laser-scanning confocal microscope acquiring images at 25-30 frames per second. Only representative images showing spCa releases over the course of the experiments are illustrated here. The original grayscale images were converted with reference to the color scale according to the arbitrary [Ca ]i values. 2+  2+  89  releases in V M F s . The solid trace shows the basal spCa release events of one site in a VMF. The ryanodine receptor opener caffeine (15 mM) abolished the spCa releases and slightly depressed the baseline [Ca ]j (dotted trace). Figure Effects of caffeine on spontaneous C a  +  2+  2+  -50  I  0  +  1  1  1  1  1  5  10  15  20  25  1  30  Time (seconds)  90  Figure Effects of ryanodine on spontaneous Ca releases in VMFs. The solid trace shows the basal s p C a release events o f one site in an another V M F . The specific ryanodine receptor blocker ryanodine (100 p M ) preserved the s p C a releases but prolonging the time between each s p C a release while also slightly depressed the baseline [ C a ^ (dotted trace). 2+  2+  2+  - 5 0 "I 0  2  1  5  1  10  1  1  1  1  15  20  25  30  Time (seconds)  91  Figure Distribution of spCa release data as a function of [Ca [j. In experiments where spontaneous C a releases were examined (i.e. a total of 101 spCa release sites in n = 10 cells), data points from a 30-second period were grouped according to their [Ca ], values (as % of the peak). +  2+  2+  2+  %of Peak (0 %= Baseline)  92  The time between the peaks of each spCa release was calculated. For the purpose of analysis, a spCa release event was defined as [Ca ]i > 25 % above baseline (please refer to Section 3.6.2 for details). Only data from basal and ryanodine (100 uM) treatments were included for calculation of the peak-to-peak latency, since caffeine treatment completely abolished the spontaneous Ca releases. Blockade of the RyR with ryanodine signficantly increased the latency period between spCa releases. (* P < 0.05 vs. basal) Figure Latency period between spCa  release events.  2+  2+  2+  2+  2+  basal  ryanodine  93  4.2.14. Schematic Model of Membrane Receptors and C a  z +  Transporters in V M F s  The current understanding of both spontaneous and drug-induced Ca  2+  signaling  pathways in human VMFs is summarized in Figure Briefly, agonists binding to Hi and P2Y2  receptors stimulate ER Ca release from one of two Ca compartments while P2Y2 receptor 2+  activation also induces Ca  2+  2+  influx. Ca  2+  influx also occurs via SOC opening when both IPs-  sensitive and lP3-insensitive ER Ca compartments are deprived of Ca . Although no caffeine2+  2+  induced [Ca ]i response is present in VMFs, the presence of functional RyRs is implicated by 2+  their modulatory actions on spontaneous Ca  2+  releases.  94  Histamine, upon binding Hi receptor, activates intracellular Ca release from the ER. Stimulation of P2Y2 receptors also induces Ca release from the same store, albeit at a lesser extent. A secondary effect of P2Y2 receptor activation is the stimulation of Ca influx, a phenomenon not observed with histamine application. Both histamine and ATP fail to elicit Ca release from the entire ER, since inhibition of the SERCA reveals an additional ER Ca compartment that is free of IP3RS. By completely depleting the ER of Ca , store-operated Ca channel is activated, facilitating Ca influx to refdl the ER. Opening of RyRs, and possibly of IP3RS as well, are responsible for the fast, localized spontaneous Ca releases observed in some cells. Figure Schematic model of C a  2 +  signaling in V M F s .  2+  +  2+  2+  2+  2+  2+  2+  2+  95  4.3. Discussion Numerous reports have suggested that VMFs, which are the predominant cells in cardiac valves, are the principal targets in the development of valvular diseases (Roberts 1973; Rose 1996; Becker 1998; Virmani 1998; McDonald et al. 2002). Evidence points to the roles of VMFs in valvular contraction (Filip et al. 1986), injury repair (Lester and Gotlieb 1988), and ECM secretion (Lester and Gotlieb 1988), all of which may be extensively controlled by Ca  2+  signaling. There are a few reports on agonist-induced transient [Ca ]; increases in VMFs 2+  (Taylor et al. 2000; Hafizi et al. 2000), but no information is available regarding the mechanisms involved. Thus, the present study investigated drug-induced Ca signaling pathways in VMFs. 2+  4.3.1. Histamine as an Intracellular C a  Mobilizing Agent in V M F s  Histamine is one of the most important mediators of inflammatory and allergic reactions. The roles of histamine in the cardiovascular system have been well studied. Contractions in conduit arteries are governed by Hi receptors, while peripheral vessels are relaxed by activation of both Hi and H receptors (Novak and Falus 1997). In the heart, histamine is inotropic, 2  chronotropic, and arrhythmogenic, via activation of H] and H receptors (Novak and Falus 1997). 2  Little is known about the effects of histamine on cardiac valves, but with about 30 % of hospitalized cardiac patients suffering from valvular heart disease (Soler-Soler and Galve 2000) this topic is certainly relevant to cardiac medicine. In this study, hVMFs were stimulated consistently with 100 pM histamine due to the lack of reproducible responses at lower concentrations. At first glance, this histamine concentration seems high but its use was justified for two reasons. Firstly, the concentration of histamine in mammalian tissue ranges between 0.01 and 1 mM histamine (Babe Jr and Serafin 1996). Secondly, numerous studies of [Ca ]; regulation in vascular smooth muscle cells (Krsti et al. 2+  96  1996) and fibroblasts (Johnson et al. 1990; Niisato et al. 1996) have employed histamine concentrations in the 100 micromolar range to investigate Ca signaling mechanisms at maximal 2+  levels of response. It was shown in Figures and that the transient histamine-induced [Ca ]; 2+  increase in hVMFs is due to activation of Hi receptors, i.e. the [Ca ], increase was selectively 2+  blocked by pyrilamine (Hi antagonist) but not by cimetidine (Hi antagonist). This finding agrees with an earlier study which showed that activation of Hi receptors is responsible for generating valvular contractions in pigs (Chester et al. 2000). The histamine-induced [Ca ]i responses were 2+  indistinguishable when elicited in either Ca -containing or Ca -free solution, as shown in 2+  Figures and In addition, blockade of Ca Ca  2+  2+  2+  influx by SKF-96365 did not alter  signals elicited by histamine (Figure nor did histamine accelerate the rate of M n  2+  entry in hVMFs. It is possible that the cell-culturing process may cause hVMFs to lose the expression of membrane-bound Ca  2+  channels but this has not been the case in studies where  cultured human smooth muscle cells were used (L'Heureux et al. 2001; Stepien et al. 2002). Therefore, the evidence suggests that histamine activation of Hi receptors induces an increase in [Ca ]i solely by Ca release from the ER. 2+  2+  4.3.2. Intracellular C a  2 +  Release and C a  2 +  Influx Stimulated by Purinergic Agents in VIVIFs  Besides histamine, the other key vasoactive substances belong to the family of 5' nucleotide triphosphates. Representative examples of this class of agents include endogenous ATP and UTP. In response to physiological stimuli, endothelial cells release ATP (Bodin et al. 1992) and UTP (Saiag et al. 1995). The actions of ATP and UTP may be autocrine or on surrounding cells.  For example, activation of endothelial P y receptors results in [Ca ]j  increases and production of NO and EDHF (Marrelli 2001).  2+  2  Stimulation of P x and P y 2  2  97  receptors increases the contractility of cardiac myocytes as a result of ER Ca release and C a z+  z+  influx (Vassort 2001). The ionotropic properties of P x receptors (Vassort 2001) mean that they 2  open to allow influx of Ca  2+  (and other ions) but have no effects on intracellular Ca  release.  2+  On the contrary, P Y receptors are G-protein-coupled and are upstream of the IP signal 2  3  transduction cascade. As shown in Figures and, the purinergic agonists ATP and U T P induced ER Ca release in VMFs in the absence of extracellular Ca , suggesting minimal, 2+  2+  if any, contribution of P x receptors in intracellular Ca 2  microglia, opening of P x receptors prevents Ca  2+  2  2+  mobilization. In some cells such as  influx via P y receptors (Wang et al. 2000). 2  This phenomenon is not present in VMFs, since preliminary data showed unaltered ATP-induced Mn  2+  entry in the presence of pyridoxalphosphate-6-azophenyl-2',4'-disulfonic acid (PPADS), a  selective P x receptor antagonist. 2  Thus, the emphasis of purinergic receptor-mediated Ca  2+  signaling in VMFs is on the study of P Y receptors. 2  It has been reported that ATP is rapidly degraded by endothelial ecto-ATPases to adenosine in whole tissue preparations (Bernardi et al. 1997; Fleetwood et al. 1989; Kuzmin et al. 1998; Meghji et al. 1992). Adenosine has cardioprotective effects during myocardial ischemia and reperfusion (Ely and Berne 1992). Vasodilatory actions by adenosine are also observed in smooth muscle (Shryock and Belardinelli 1997). The generation of adenosine complicates the study of ATP actions on whole tissues but not in the experiments with VMFs here, since ectoATPases and endothelial cells are not present in the specimens.  The potential effects of  adenosine on VMFs represent an entirely new research area that is beyond the scope of this study, and thus are not discussed here. Readers are referred to reviews by Ralevic and Burnstock (1998) and Shryock (1997) for details about adenosine and its pharmacological actions on the cardiovascular system.  98  Several reports have documented the use of high concentration of ATP and UTP (i.e. 100 pM) that elicits maximal responses of [Ca  2+  ]i  and membrane potential (Mateo et al. 1996; Viana  et al. 1998; Wang et al. 2000; Moccia et al. 2001). Therefore, 100 uM ATP and UTP, were applied to VMFs throughout this study. Similar efficacies of [Ca ]j responses elicited by ATP 2+  and UTP were seen in VMFs, and clear Ca  2+  influx components were demonstrated in the  presence of both agonists. As shown in Figures and, the longer durations of [Ca ]j responses in nPSS than in OCaPSS first suggested P Y receptor-stimulated Ca 2+  2  Secondly, Figure showed acceleration of M n  2+  2+  influx.  entry rates during the ATP and UTP  treatments, indicating agonist-stimulated divalent cation influx. Lastly, incubating VMFs with the ROC/SOC blocker SKF-96365 significantly suppressed the P influx (and M n  2+  2Y  receptor-stimulated Ca  2+  influx).  The choice of pharmacological agents in the characterization of P y receptor subtypes in 2  VMFs depends largely on existing literature documenting studies with other cell types in various species.  According to a number of reviews (Ralevic and Burnstock 1998; Vassort 2001;  Williams and Jarvis 2000; Alexander and Peters 1999), there is great heterogeneity in the potencies and efficacies of purinergic drugs on receptor subtypes between animals and cell types. The general consensus after consulting the literature is that ADPPS and 2-Me-S-ATP are widely accepted as selective P YI receptor agonists whereas UTP is frequently used to stimulate P 2  receptors specifically.  As mentioned before, activation of  P Y 2  2Y2  receptors with UTP elicited  2  [Ca ]j responses similar to those with ATP. In addition, Figures and showed that neither ADPPS nor 2-Me-S-ATP induced a [Ca ]; response. Thus, the present data indicate 2+  that P  2 Y  2  receptors are responsible for both ER Ca release and Ca influx in VMFs. 2+  2+  99  With regards to purinoreceptor antagonists, the conclusion from literature sources is that no selective P2Y antagonists are commercially available. Suramin is one of the more commonly used broad-spectrum P2 receptor blockers (Dunn and Blakeley 1988).  However, its P2-  antagonistic property is overcome by non-specific activities (Ralevic and Burnstock 1998). A report has shown that suramin non-competitively blocked serotonin and thromboxane receptors in platelets (Hourani et al. 1992). Most importantly, suramin increases skeletal and cardiac RyR opening probabilities and conductances (Sitsapesan and Williams 1996). Knowing from Section 4.2.13 that RyRs may contribute to spontaneous Ca releases in VMFs, suramin was not used in 2+  this study to block P receptors. In fact, the use of suramin, minus its side effects, would not 2  provide additional information on P y receptors in VMFs, amid the lack of selective 2  purinoreceptor antagonists. 4.3.3. Distinction between IP3-Sensitive and IP -Insensitive E R C a  2 +  3  Both histaminergic (Bakker et al. 2002) and purinergic  P Y2 2  Compartments  receptors (Ralevic and  Burnstock 1998) are coupled to G-proteins which, upon activation, stimulates IP3 production and Ca release via IP Rs. There are other modes of Ca release from the ER - mediated by RyR 2+  2+  3  (or cyclic ADP-ribose) and by nicotinic acid adenine dinucleotide phosphate (NAADP). Evidence in various cell types indicates that different modes of ER Ca necessarily inclusive of each other. ACh-insensitive ER Ca  2+  2+  release are not  store has been shown in fresh  endothelial cells (Wang et al. 1995). In the pancreatic acinar cells, ACh-insensitive ER Ca  2+  store is prone to release by SERCA blockade (Camello-Almaraz et al. 2000), a phenomenon similar to the histamine- and ATP-insensitive ER Ca  2+  store in VMFs shown in Sections 4.2.5  and 4.2.11. Studies on smooth muscle and secretory gonadotropes have reported the existence of two independent, SERCA-containing ER Ca  2+  stores - one with IP3RS and RyRs and the other  100  with RyRs only (Johnson et al. 2000; Flynn et al. 2001). It is not unusual that ER Ca release 2+  via RyRs is not observed as easily as that mediated by IP3RS, as is the case in fresh endothelial cells (Wang et al. 1995).  In the present study, a direct, measurable [Ca ]i response from 2+  opening RyRs was not visualized in VMFs. However, the presence of functional RyRs could be demonstrated by their modulatory actions on spontaneous Ca  2+  releases (please refer to Section  4.2.13 and 4.3.6 for details). A series of experiments led to the finding of IP -sensitive and IP3-insensitive (or SERCA3  sensitive) ER Ca  2+  stores in VMFs. In Figure, it was shown that removal of Ca from 2+  the extracellular space had no effect on the histamine-induced [Ca ]i signal, but subsequent 2+  responses to histamine were abolished. In Ca -containing solution, repeated histamine-induced 2+  2+  •  •  [Ca ]i responses were seen, only interrupted by the application of CPA (Figure It is worth mentioning here that CPA was preferred to thapsigargin in the experiment due to the latter's irreversible blockade on the SERCA and subsequent cytotoxic events (Bai et al. 1999). Based on Figures and, it is clear that refilling of the ER via Ca  2+  influx and  SERCA-mediated sequestration is part of histamine-induced Ca signaling in VMFs. However, the fact that neither OCaPSS (Figure nor SKF-96365 (Figure had any effect on the first [Ca ]i transient suggested that histamine did not activate receptor-operated or voltage2+  gated Ca  2+  channels. Therefore, refilling from the extracellular space was dependent on the  presence of a basal Ca  2+  leak of the plasma membrane (Alderton and Steinhardt 2000). The 2_|_  observation that CPA increased the rate of decay of the histamine-induced [Ca ]; response and abolished the oscillatory component indicated in normal conditions, there is partial recycling of Ca from the cytosol to the ER. 2+  101  When Ca recycling is prohibited, not by SERCA inhibition, but by incubating VMFs in 2+  OCaPSS as in Figure, the histamine-insensitive ER Ca store is revealed. After VMFs no 2+  longer responded to histamine stimulation in OCaPSS, additional Ca  release was induced by  CPA (Figure Based on the computational results explained in Section, the conclusion of two ER Ca  2+  compartments in VMFs is reached. The histamine-sensitive C a  2+  compartment contains 53.6 % of total ER Ca content, and the remaining 46.4 % Ca makes up 2+  the histamine-insensitive Ca  2+  2+  compartment.  The previous paragraphs showed how histamine-insensitive (or CPA-sensitive) ER Ca  2+  release was unresponsive to repetitive histamine stimulations. It is not clear until after the following experiments that the Ca  2+  compartments (in)sensitive to histamine could be  generalized in terms of their sensitivity to IP3. Experiments in Figure illustrated that 2+  2"F  CPA, but not ATP (an IP - and Ca mobilizing agent), was able to stimulate additional ER Ca 3  release after exhausting the histamine-sensitive Ca ATP was applied first, however.  2+  store. A different result was seen when  Figure shows that following exposure to ATP,  histamine was able to induce more Ca  2+  release from the ER, with CPA stimulating the  remaining ER Ca release. It is paradoxical that both IP -mobilizing agonists (i.e. histamine and 2+  3  ATP) would generate a response depending on the sequence they were applied in. With no known cross-desensitizing effects between  Hi  and  PY 2  2  receptors, one explanation for the  observation in Figure may rest in the distribution and number of P For instance, if  P Y2 2  Y  2  receptors in VMFs.  receptors are localized to certain portions of the PM, the  probably diffuses only to the ER nearby and fails to activate all the P2Y2  2  IP3R.  IP3  produced  On the other hand, if  receptors are sparsely but evenly populated, globally only small amounts of IP3 is produced  upon ATP stimulation. The concentration of IP3 maybe too diluted to stimulate full release of  102  the IP3-sensitive Ca  2+  store. Nevertheless, the speculations above can only be verified by 1)  immunofluorescent studies where the HiR and  P2Y2R  are labelled and 2) comparing both global  and localized IP3 concentrations upon histamine and ATP application. To summarize, the data presented here are consistent with the notions of an IP -sensitive Ca store fully releasable upon 2+  3  stimulation by histamine, and an IP -insensitive Ca store that is susceptible to CPA. 2+  3  4.3.4. Store-Operated C a  Depletion of Ca  2+  2 +  Channel Activity in V M F s  from the IP3-sensitive ER Ca compartment alone is not sufficient to 2+  activate store-operated Ca  2+  entry, as demonstrated by the lack of Ca  2+  influx during histamine  stimulation. Application of hstamine only partially empties the ER of Ca . In VMFs, SOCs are activated when both IP3-sensitive and nvinsensitive ER Ca after SERCA blockade. SOCs, identified as Ca  2+  compartments are free of Ca  2+  channels which open in response to ER Ca  2+  2+  depletion (Clapham 1995), have been observed in many cell types, including vascular smooth muscle (Gibson et al. 1998; Zacks et al. 1991) and endothelium (Wang and van Breemen 1997). The slow rising phase of [Ca ]i (Figure elicited by CPA is the net result of basal ER 2+  Ca  2+  release and loss through SERCA locked in the open state. Prolonged CPA incubation  eventually depletes the ER Ca  2+  stores, and SOCs are activated subsequently.  Activation of  SOCs in VMFs is supported by three observations. Firstly, CPA caused a maintained elevation of [Ca ]j that is indicative of store-operated Ca entry (Figures and Secondly, 2+  2+  with CPA throughout the experiment, when OCaPSS was substituted with nPSS, an elevated [Ca ]j above baseline was seen, again representing continuous Ca influx (Figure The 2+  2+  last evidence of SOC activity is revealed by M n used in mimicking Ca  2+  2+  quenching experiments, which are commonly  influx (Wang and van Breemen 1997; Trepakova and Bolotina 2001;  Wang et al. 1995b). The rate of M n  2+  influx was significantly increased shortly after CPA was  103  added (Figure The slight delay between CPA application and increase in M n  z+  influx  rate maybe best explained by the time necessary for depletion of ER Ca , which is a prerequisite 2+  for the activation of SOCs. 4.3.5. [Ca ]i Responses of Normal and Rheumatic V M F s 2+  The characterization of intracellular Ca  2+  signaling mechanisms in the above sections  allows the understanding of the physiology of normal VMFs.  In response to the growing  incidence of valvular heart diseases and their correlation with VMFs, the logical next step was to investigate the Ca signaling properties of diseased VMFs. In this work of thesis, VMFs of the 2+  rheumatic origin were examined as a starting point towards more extensive and thorough studies on other valvular diseases in the future. As outlined in Table, comparisons between normal and rheumatic VMFs were made with respect to the peak sizes and AUCs of the histamine-, ATP- and CPA-induced [Ca ]j responses in nPSS and OCaPSS. The most notable 2+  characteristic of rheumatic VMFs was the evidence for Ca influx during histamine stimulation. 2+  In addition, there was marginally more Ca  2+  influx induced by ATP stimulation in rheumatic  VMFs (P = 0.187). Slightly stronger store-operated Ca  2+  influx (P = 0.241) and lower ER C a  2+  content (P = 0.0734) were detected in rheumatic VMFs. The data from rheumatic VMFs could be broadly interpreted as alterations in the diseased cells' handling of extracellular Ca . Ca 2+  2+  influx changes in rheumatic VMFs may have connections with reports 1) suggesting the alleviation of atrial fibrillations, associated with rheumatic heart disease, by Ca channel blockers (Levy 2001), and 2) showing Ca deposits in the myocardium of rheumatic hearts (Li 2+  1993). Nevertheless, limited sample size and individual bio-variability in the present study may have hampered the statistics of some of the findings but they provide valuable leads in future experiments.  104  4.3.6. Spontaneous C a  Releases and Functional Evidence for RyRs in V M F s  z +  Spontaneous, subcellular Ca  2+  releases were visualized in a number of VMFs in this  study (Figure The functional role of these Ca  2+  releases in VMFs has yet to be  determined, and it was unclear why not all the VMFs fire spontaneous [Ca ]i signals. However, 2+  the presence of Ca  2+  sparks in cardiac (Eisner et al. 1998) and smooth muscles (Jaggar et al.  2000) may shed some light on the importance of spontaneous Ca releases in VMFs. Ca spark 2+  2+  is a localized [Ca ]i increase caused by spontaneous opening of RyRs. It is believed that Ca 2+  2+  sparks mediate excitation-contraction coupling in cardiac myocytes and modulate vasorelaxation via the activation of Ca -sensitive K channels (Imaizumi et al. 1999). In VMFs, there is 2+  +  evidence for Ca sparks based on the data shown in Figures and These Ca 2+  2+  sparks probably contribute to the pulsatile movements of valvular leaflets in each cardiac cycle. 2_j_  Both caffeine and 100 p M ryanodine treatments suppressed the [Ca ]; baseline and spontaneous [Ca ]i signals. Although known for its positive action on RyRs, caffeine has also 2+  been shown to inhibit IP Rs in some cells (Bezprozvanny et al. 1994). The lack of a caffeine3  induced [Ca ]i response in VMFs may suggest that the number or density of RyRs is relatively 2+  low. Thus, in VMFs the RyR-activating effect of caffeine may not overcome its potential IP R3  inhibitory effect. The abolition of spontaneous Ca releases during caffeine treatment in Figure 2+ implicitly suggests a role of  IP3RS  in generating subcellular [Ca ]; signals. 2+  Experiments with selective IP3R modulators are required to confirm this speculation. In contrast, the ryanodine effect was straightforward since RyR blockade by 100 pM ryanodine inhibited RyR-mediated Ca  2+  release, increasing the latency period of Ca  2+  sparks (Figure  Therefore, the ryanodine data not only illustrate Ca sparks via RyR opening, but also reveal the 2+  presence of functional RyRs in VMFs, previously unknown from global [Ca ]i measurements. 2+  105  C H A P T E R V: M E C H A N I S M S O F C A  2 +  R E M O V A L IN V A S C U L A R  E N D O T H E L I A L C E L L S (ECs) - R O L E O F CYTOSKELETON AND C A  2 +  TRANSPORTERS  5.1. Overview Having discussed several aspects of Ca signaling in VMFs in the previous chapter, the 2+  following will concentrate on the maintenance of intracellular Ca  2+  homeostasis in ECs, which  are most likely to interact with VMFs in the cardiac valve. Numerous reports and reviews have discussed Ca entry mechanisms in endothelial cells (ECs). One example is a review by Nilius 2+  and Droogmans (Nilius and Droogmans 2001). In contrast, only a handful of studies focused on how Ca is removed from ECs. The lack of documentation on endothelial Ca extrusion does 2+  2+  not undermine the significance of this study. This is because a few studies have correlated abnormal Ca  2+  removal in the endothelium with transplant vascular disease (Skarsgard et al.  2000; Demers et al. 2001) and oxidative stress-related conditions such as atherosclerosis (Grover and Sampson 1997). Even in the studies where endothelial Ca  2+  removal was investigated, the  conclusions were based on findings in cultured ECs (Paltauf-Doburzynska et al. 1999; Goto et al. 1996; Sedova and Blatter 1999). It has long been shown that cultured cells generally do not reflect in vivo cell physiology as well as freshly isolated cells or intact tissues do. Using intact valvular endothelium may be ideal in this study; however, physiological influences by the underlying myofibroblasts, which to date are not well understood at all, may interfere with attempts to fully understand how endothelium functions on its own. Thus, a native preparation of enzymatically-dissociated ECs was used to elucidate mechanisms of cytosolic Ca removal in 2+  this study. This native EC preparation enabled the study of single cell physiology without changes in expression of receptors and ion transport molecules so often seen during tissue culture. 106  In this study, although aortic ECs were used owing to the already established cell isolation protocols (Wang et al. 1995), the findings here would be applicable to ECs in general (i.e. valvular ECs) since an earlier report from our laboratory showed similar Ca  2+  signaling  properties between aortic and valvular ECs (Li and van Breemen 1995). In all experiments, acetylcholine (ACh) was used as the physiological stimulus on the freshly isolated ECs. Figure 5.1.1 shows sample  F340/F380  images of fura-2-loaded ECs before  and after ACh stimulation. The acquired data supported the idea of an in-series SERCA-NCXlinked Ca  2+  extrusion pathway. The importance of an intact cytoskeleton in facilitating this  pathway was implicated. RyRs were shown to act as an intermediate component of the SERCANCX pathway.  Functional couplings between SERCA & RyR, and NCX & RyR were  demonstrated by simultaneous inhibition of both Ca transporters. Fluorescently labelled RyRs 2+  were visualized as additional evidence for the presence of functional RyRs in ECs. Lastly, the role of carboxyeosin as a PMCA blocker was observed. The use of carboxyeosin on top of NCX blockade effectively inhibited two parallel Ca  2+  removal pathways in ECs, one involving  SERCA-RyR-NCX and the other involving PMCA.  107  Figure 5.1.1. stimulation.  images of fura-2-loaded E C s before and after acetylcholine explained in Section 3.3.1, intracellular Ca 2 + concentration ([Ca ]i) was  F340/F380  As expressed as the ratiometric fluorescent intensity at 340-nm and 380-nm excitation. The original grayscale images were converted to pseudocolored ones with references to the color scale shown in the lower right of each panel. The [Ca ]j values of the unstimulated ECs (left panel) increase upon stimulation with 10 uM acetylcholine (right panel). 2+  2+  unstimulated  + acetylcholine  108  5.2. Results Note: Sections 5.2.1 and 5.2.2 reflected parts of a collective work (Wang et al. 2002) and represented integral components of this thesis. 5.2.1. Sarco(endo)plasmic reticulum Ca -ATPase (SERCA) and Sodium-Calcium 2+  Exchanger (NCX) Contribute in Series to C a  2 +  Removal in ECs  In the control condition, freshly isolated ECs were stimulated with the physiological agonist acetylcholine (ACh, 10 pM) in nPSS. When [Ca ]j level reached a plateau, both ACh 2+  and extracellular Ca were removed and replaced with OCaPSS. [Ca ]i decline rates were used 2+  2+  as a parameter of measuring Ca extrusion in ECs. Besides the control, ECs were subjected in 2+  random order to three other treatments: SERCA inhibition, NCX inhibition, and simultaneous SERCA and NCX inhibition. Cyclopiazonic acid (CPA, 15 uM) was used to inhibit SERCA. Inhibition of NCX was achieved by substituting nPSS with ONaPSS, which consisted of equimolar of 7V-methyl-£)-glucamine (NMDG) in exchange of NaCl. Both CPA and ONaPSS had no known adverse effects and their actions on SERCA and NCX were completely reversible. [Ca ]j decline rates were compared among the control and CPA- &/or NCX-treated experiments. 2+  Figure shows representative traces of ACh-induced [Ca ]j increases in control and 2+  treated conditions (as reproduced from Wang et al. 2002). In this figure, the [Ca ]i decaying 2+  phase of the control response was superimposed on the subsequent responses as dashed traces, demonstrating that ECs extrude Ca  2+  slower when SERCA or NCX was inhibited. The rate of  [Ca ]i decay with combined CPA-ONa treatment was the same as that with CPA alone (superimposed as long dashed trace). Binned [Ca ]i decline rates from all experiments were 2+  plotted against [Ca ]j levels in Figure Samples of exponentially fitted [Ca ]i decaying 2+  2+  phases are shown in Figure and the average Ca removal rate constants, as a percentage 2+  109  of the maximum, i.e. the control rate constant, are shown in Figure Both the raw [Ca ]i decline rates and calculated Ca removal rate constants supported the finding in Figure 2+  that SERCA and NCX handle Ca in series for extrusion since blockade of either or both Ca 2+  2+  transporters reduces Ca extrusion rate to the same extent. 2+  110  Figure Acetylcholine (ACh)-induced [Ca ]j elevations in ECs. ACh (10 uM) was 2+  applied to ECs in nPSS. Both ACh and nPSS was removed and substituted with Ca -free solution (OCaPSS) once [Ca ]; has reached a plateau. Traces from control and 3 treatment conditions are shown below (representative of n = 6 experiments). The 3 treatments were: Na free solution (ONa), cyclopiazonic acid (CPA), and a combination of both. ONa was used to inhibit the activity of Na /Ca exchanger. CPA was used to block the SERCA. The [Ca ]i decline rates from different experiments were compared. The control [Ca ]; decline phase was reproduced in the subsequent traces (in short dashed form). The long dashed trace on top of the CPA+ONa-treated [Ca ]i decline phase was reproduced from the CPA experiment. 2+  2+  +  +  2+  2+  2+  2+  Ill  Figure Summarized data of [Ca" ]i decline rates at given ranges of [Ca ],. Instantaneous slopes of the raw traces (as exemplified in Figure were calculated and binned into groups according to the % normalized [Ca ]j. The [Ca ]i groups were 0-5 %, 510 %, 10-15 %, 15-20 %, 20-40 %, 40-60 %, 60-80 %, and 80-100 % normalized [Ca *],. From a total of n = 6 experiments in each treatment, data within each group were averaged and plotted as follows. Detailed explanation of the analytical method was given in Section 3.6.3. (* P < 0.05 vs. all treatments) i+  2+  2+  2+  2  ONaCPA - © - ACh control -B- ONa: -A- CPA  I 09  2  c o  '55  5  % of maximal response of [Ca ] 2+  112  Figure Sample one-component exponential fits of [Ca ]j decline phases in ECs. 2+  The kinetics of [Ca ]; declines in ECs was arbitrarily set to follow a l -order exponential decay: Normalized % [Ca ]i = e where k is the rate constant. Based on the raw data, computational iterations were made to determine the fitted curve that best represented the data. As a result of the fitting, [Ca ]i decay rate constants were calculated, and examples of which are shown in the inset table below. 2+  st  2+  k(tlme)  2+  40 Rats Const,  o ACh control 0.1528 30  ••  ONa  0.0806  A  CPA  0.0720  <>  o 20 to co a.  ONa-CPA  0.0651  to Q>  CC "CJ  10.  I  as £  o z  -10 20  40  SO  80  Time (seconds)  113  Figure Mean fitted C a  decay rate constants as a percentage of the control value.  Fitted ONa-, CPA-, and ONa+CPA-treated Ca decay rate constants from different experiments were normalized to the control values (at 100 %). In a total of n = 6 experiments for each treatment, the control rate constant was significantly greater than the ones under NCX and/or SERCA inhibition. (* P < 0.0003 vs. control) 2+  114  5.2.2. Serial Arrangement of S E R C A and N C X is Maintained by Intact Cytoskeleton  The functional, serial arrangement of SERCA and NCX described above contributed significantly - about one-half - to Ca extrusion in ECs, as shown by the 50 % reduction of Ca  2+  removal rate constants in Figure  2+  2+  It is unlikely that such organization of Ca  transporters occurs completely by chance. Betz (1983) has shown that in brain capillary ECs the cytoskeleton may play a role in maintaining the functional linkage between IP3 receptors and the plasma membrane (PM). Cytochalasin D (CytD) is an actin-depolymerizing agent and was used here to disrupt the cytoskeleton in order to elucidate the mechanism of SERCA-NCX apposition. The same control and (CPA &/or NCX) treated conditions were used as in Section 5.2.1, except the ECs were incubated with 50 pM CytD for 90 minutes prior to the experiments. It is noted that only 3 ACh responses could be obtained consistently after the CytD treatment, as opposed to the 4 responses in ECs without CytD incubation. The disruption of the cytoskeleton may render the ECs less responsive to repetitive agonist stimulation associated with altered spatial PM-ER arrangement. Due to this limitation, data from different experiments were pooled together for analysis. Figure shows representative traces from one experiment where the control, CPA-treated, and ONa-CPA-treated protocol was done. Binned Ca  2+  decline rates are  shown in Figure Similar to untreated ECs, inhibition of either SERCA or NCX in CytD2+  treated ECs showed reduction in Ca  removal rates when compared to control. However,  simultaneous SERCA and NCX inhibition resulted in further slowing of Ca finding was supported by the Ca  2+  2+  extrusion. This  removal rate constants (Figure calculated from the  exponentially fitted [Ca ]i decaying phases (Figure Another agent that disrupts the 2+  cytoskeleton via a different mechanism was also used.  Latrunculin A (LatA, 30 pM) (De  Oliveria and Mantovani 1988) works by inhibiting microfilament processes.  Representative 115  traces from a separate experiment where the ECs was treated with LatA also showed that combined SERCA-NCX blockade slowed Ca removal more than individual blockade of NCX 2+  or SERCA (Figure Thus, it is evident that by dissociating the cytoskeleton, the serial arrangement of SERCA and NCX in fresh ECs is lost.  116  Figure ACh-induced [Ca ]j elevations and declines in cytochalasin D (CytD)treated ECs. CytD is an actin-polymerizing agent that disrupts the cytoskeleton of ECs. ECs 2+  were pretreated with 50 pM CytD for 90 minutes prior to ACh stimulation. In the sample shown below, CPA- and ONa+CPA-treated [Ca ]i responses were obtained after the control (representative of n = 4 experiments). This is in contrast to the total of 4 responses (1 control + 3 treatments) in ECs without prior CytD treatment (as in Figure The CytD treatment might structurally alter the ECs in a way such that only 3 consecutive ACh responses could be recorded in the same experiment. Of the 3 responses in each experiment, the ONa+CPA treatment was always present; the remaining responses were obtained from control, ONa, and CPA, in random order. The peak of the ONa+CPA-treated [Ca ]i response in each experiment represented 100 % of the normalized % [Ca ]j. This enabled data from all the experiments to be pooled together for analysis. In this figure, the dotted trace was reproduced from the control response, and the long dashed trace from the CPA-treated response. 2+  2+  2+  117  ]j decline rates in CytD-treated ECs. Data were analyzed in a similar manner as in Figure for a total of n = 4 experiments. Figure Summarized data of [Ca  118  Figure Sample one-component exponentential fits of [Ca ]j decay phases in CytD2+ treated ECs. The inset table shows the fitted Ca removal rate constants, determined in the  same manner as in Figure  119  Figure Comparison of the mean C a  2 +  removal rate constants in CytD-treated ECs.  Fitted Ca removal rate constants from different treatments were normalized to the control values in a total of n = 4 experiments. As in Figure, the control rate constant was significantly larger than those under ONa or CPA treatment. However, a disrupted cytoskeleton further reduced the Ca removal rate constant under combined NCX and SERCA blockades. (* P < 0.05 vs. control; # P < 0.05 vs. all bars) 2+  2+  ioo i  £  80-  1 fi  60/  I  •  a O  o  #  40-  *  *  T  T  mm mm  mm Wmm  ill 20 A  m  mm  111  —T' ~  A C h control  ONa  CPA  OlfeCPA  120  LatA is another cytoskeleton dissociating agent. LatA (30 pM) was applied to ECs 90 minutes prior to the experiments. This figure shows representative control, ONa-treated, and ONa+CPA-treated ACh-induced [Ca ], responses after the LatA treatment (in a total of n = 3 experiments). The dotted trace was reproduced from the control response, and the thin solid trace (superimosed on the CPA+ONa response) was reproduced from the ONa-treated ACh response. Figure  Sample [Ca ]j responses in Latrunculin A (LatA)-treated ECs. 2+  2+  T  0  i 1 1 r r 200 400 600 800 1000 1200 1400 Time (seconds) J  1  121  5.2.3. C a  2 +  Removal is Facilitated by RyR Opening and Inhibited by RyR Blockade  After identifying the SERCA-NCX pathway of Ca removal in ECs, the next step was to 2+  determine the ER Ca -release channel in between the two Ca transporters. The two major ER 2+  Ca  2+  release channels in ECs are  2+  IP3RS  and RyRs.  IP3RS  are involved in intracellular Ca  2+  mobilization during agonist stimulation and thus, the role of these receptors in removing cytosolic Ca  is probably minimized. On the contrary, no known effects of RyRs have been  2+  found before although there have been reports of the presence of RyRs in ECs (Ziegelstein et al. 1994; Wang etal. 1995). [Ca ]i decline rates of control and ryanodine- or caffeine-treated ECs were compared. 2+  The control 10 pM ACh response was obtained first, and the treated response was done after 15 minutes of nPSS perfusion. The 15-minute washout allowed the ECs to fully recover from the previous stimulation, as was confirmed by two identical ACh responses obtained in 15 minutes apart in separate time control experiment (data not shown). Both 15 mM caffeine and 1 p M ryanodine were used as RyR activators. In Figures to, the black solid trace denotes the control ACh response while the gray dotted trace denotes the caffeine- or ryanodinetreated ACh response. Caffeine (15 mM) facilitated the [Ca ]i decline rate, as shown by the 2+  more rapid [Ca ]i downstroke (Figure, representative of n = 8 experiments). The 2+  specific RyR ligand ryanodine exerts its activating effect at low concentrations, i.e. between 0.1 to 10 pM, depending on the tissue (Fill and Copello 2002). In the present study, 1 uM ryanodine increased [Ca ]i decay rates in ECs (Figure, representative of n = 12 experiments). The 2+  data in Figures and showed that by increasing the RyR opening probability, cytosolic Ca is removed more effectively. 2+  122  Besides acting as a RyR agonist at low concentrations, ryanodine also blocks RyR at high concentrations (Fill and Copello 2002). RyRs in ECs were blocked by 100 pM ryanodine here. By comparing the ryanodine-treated [Ca ]i decay rates to those of the control cells, Ca 2+  2+  removal was slower when the RyR was blocked (Figure, representative of n = 8 experiments). As mentioned in Section 3.6.3, two approaches were used to quantitate the [Ca ]i decline 2+  rate data. Average [Ca ]i decline rates from different experimental conditions: control, caffeine 2+  (15 mM), and ryanodine (1 and 100 pM) were plotted as a function of binned % normalized [Ca ]i levels, as described in Section 3.6.3 (Figure At 15, 20 and 40 % normalized 2+  [Ca ],, [Ca ]i declines were significantly faster in the presence of 15 mM caffeine or 1 pM 2+  2+  ryanodine than in the control experiments (P < 0.05). On the other hand, Ca extrusion in the 2+  100 pM ryanodine treatment was significantly slower than control values (P < 0.05). The experimental data were also analyzed by fitting the decaying phase of the [Ca ]i 2+  responses with the one-component exponential fit equation: y — ae where b is the Ca removal bt  2+  rate constant. Sample exponential fits are shown in Figure In Figure, the bar graph shows average fitted Ca removal rate constants. Under control conditions, Ca removal 2+  2+  rate constant after ACh stimulation was 0.063 ± 0.003 s". The rate constants of the 1 pM 1  ryanodine and 15 mM caffeine treatments were 0.090 ± 0.014 s" and 0.096 ± 0.008 s", 1  1  respectively, and were both significantly larger than control values (P < 0.05). When RyRs were blocked by 100 uM ryanodine, the rate constant was 0.028 ± 0.004 s", significantly smaller than 1  control values (P < 0.05). Based on both raw (Figure and fitted (Figure data, it can be concluded that RyR is an intermediate component of a cytosolic Ca extrusion pathway 2+  in ECs.  123  Figure Effects of caffeine on ACh-induced [Ca ]i responses in ECs. A control :+  ACh-induced [Ca ]; response was first obtained, and [Ca" ]; decay was monitored in OCaPSS after removal of the agonist (representative of n = 8 experiments). The protocol was repeated except that the ryanodine receptor (RyR) activator caffeine (15 mM) was added together with OCaPSS. The solid line superimposed on the caffeine-treated response was reproduced from the control response.  124  Figure Effects of 1 11M ryanodine-treated ACh-induced [Ca ]j responses in ECs. 2+  As in Figure, a control ACh-induced [Ca ]j response was first obtained, and [Ca ]; decay was monitored in OCaPSS after removal of the agonist (representative of n = 12 experiments). ECs were pre-incubated with the specific RyR activator 1 pM ryanodine before repeating the protocol. The solid line superimposed on the 1 pM ryanodine-treated response was reproduced from the control response. 2+  2+  125  Figure Effects of 100 p M ryanodine-treated ACh-induced [Ca h responses in ECs.  The experiment was identical to that shown in Figure The only difference was that ECs were pre-incubated with the RyR-inhibiting concentration of 100 p M ryanodine here (representative of n = 8 experiments). The solid line superimposed on the 100 u M ryanodinetreated response was reproduced from the control response.  126  Figure Ryanodine receptor (RyR) modulating effects on Ca  z+  removal rates in ECs.  The summarized data were calculated as explained in Section 3.6.3. Data plotted below were obtained from treatments with caffeine (n = 8 experiments), 1 u M ryanodine (n = 12 experiments), and 100 uM ryanodine (n = 8 experiments). At any given [Ca ]t from 15 % to 40 %, Ca removal was facilitated when RyR was activated, and diminished when RyR was blocked. 2+  2+  127  Figure Sample one-component exponential fits of RyR modulator-treated [Ca ]; decaying phases in ECs.  -10  J  1  1  1  1  1  0  10  20  30  40  1  1  1  50  60  70  —  i  80  1  90  Time (seconds)  128  The data here again supported the claim that RyR mediated Ca removal. Opening of RyR with 15 mM caffeine (n = 8 experiments) or 1 pM ryanodine (n = 12 experiments) yielded Ca removal rate constants that were significantly greater than that of the control condition. On the contrary, control rate constant was larger than when RyR was inhibited with 100 uM ryanodine (n = 8 experiments). Figure Fitted C a  2 +  removal rate constants in RyR-modulated ECs. 2+  2+  0.12  3  i  P < 0.05 vs. control  0.10  re (O  c 0.08  o o 0  +•>  re  ± 0.06 re  > o E £  + CM  T  0.04  re O  -a 0.02 o 0.00  control  15 mM caffeine  1 pM ryanodine  100 uM ryanodine  129  5.2.4. RyR Opening Accelerates E R C a  2 +  Loss in an Extracellular C V - F r e e Environment +  Pharmacological actions of caffeine and ryanodine on RyRs were shown above. Using the same tools, RyR was again modulated and passive ER Ca  2+  loss was monitored. To ensure  that only Ca release from the ER was measured, experiments were conducted in OCaPSS. Data 2+  were acquired after 1, 5 and 15 minutes in OCaPSS and ECs were stimulated with 10 pM ACh, which has been shown previously to completely deplete the ER of Ca (Wang et al. 1995). The 2+  peak size of the ACh-induced Ca response in OCaPSS was used as a crude measurement of the 2+  amount of Ca in the ER, from which the rate of ER Ca loss could be inferred. 2+  2+  The graph in  Figure shows peak sizes at 5 and 15 minutes of each treatment. Values were expressed as percentages of the control ACh response after 1 minute in each experiment. The relatively horizontal control and 100 uM ryanodine treatment (n = 6 experiments) curves indicated that ER Ca  content remained constant over time. The curves for 1 p M ryanodine (n = 8 experiments)  and 15 mM caffeine (n = 3 experiments) treatments, however, showed much steeper slopes overall. Opening RyRs by either 1 pM ryanodine or 15 mM caffeine stimulated cumulatively a 30 % Ca loss from the ER in 15 minutes in OCaPSS. This finding suggested that in addition to 2+  increasing the Ca removal rate at an elevated [Ca 2+  2+  ]i  level (i.e. after ACh stimulation, as shown  in Section 5.2.3), RyR opening also promotes basal ER Ca depletion in OCaPSS. The data here 2+  also confirmed that ryanodine exerts its agonistic effects at 1 pM and antagonistic effects at 100 pM.  130  Figure Effects of RyR modulation on E R C a  2 +  content of ECs. ECs were stimulated  with acetylcholine (ACh) in OCaPSS with and without pre-treatment of caffeine or 1 pM / 100 pM ryanodine in OCaPSS for 1,5, and 15 minutes. The [Ca ]i peak was used as an indication of the relative ER Ca content. For each drug treatment, [Ca ]i peak levels were expressed as percentages of the ACh response after 1 minute of incubation. 100 pM ryanodine treatment (n = 6 experiments) had no significant effect on ER Ca content while 1 pM ryanodine (n = 8 experiments) or 15 mM caffeine (n = 3 experiments) treatments induced a total of about 30 % Ca loss from the ER over 15 minutes. 2+  2+  2+  2+  2+  10  5  i  i  is  _i  i  15 i  100  90  80  70  60 0  T  —•—  control ••<>•• 1 \M ryanodine — T " 100 nM ryanodine 15 mM caffeine  —v~  * P < 0.05 vs. control & vs. ryanodine 100 nM - < — i —  i  10  5  15  Time (minutes)  131  5.2.5. Ryanodine Receptors and N C X Are Functionally Coupled in Extruding Ca''*  The data thus far showed that RyR (Section 5.2.4) and NCX (Section 5.2.1) are both involved in removing cytosolic Ca after agonist stimulation. The next question was whether or 2+  not RyR and NCX handle Ca  2+  in series for eventual extrusion. [Ca ]j decline rates were thus 2+  compared under control, RyR-inhibited, NCX-inhibited, and RyR+NCX-inhibited conditions. Sample traces of ACh-induced [Ca ]j responses in nPSS (black solid trace), ONaPSS (light gray 2+  dashed trace), and 100 pM ryanodine-ONaPSS (dark gray dotted trace) from a total of 7 experiments are shown in Figure For the control trace shown in Figure, sample [Ca ]i decay under 100 pM ryanodine treatment from an earlier experiment was superimposed for comparison (shown as gray solid trace). Results of these experiments were summarized in Figure The [Ca ]; levels indicated in Figure were normalized to the peak [Ca ]i 2+  2+  obtained in ONaPSS. This was done to ensure that ECs were subjected to two ACh stimulations only, i.e. control vs. ONa, ONa vs. ryanodine, or ONa vs. ryanodine + ONa. When NCX was inhibited, [Ca ]; decline was slower than control. This finding agreed with the data shown in 2+  Section 5.2.1. Also in Figure, 100 pM ryanodine treatment alone showed the same degree of [Ca ]i decline rate reduction as the ONa treatment. This indicated that by inhibiting 2+  RyRs, the same effect on Ca  2+  removal rate was achieved as if NCX were blocked instead.  Moreover, [Ca ]i decline rates under ONa treatment completely overlapped with those under 100 2+  uM ryanodine + ONa treatment, indicating that combined NCX and RyR blockades did not inhibit Ca  2+  extrusion in an additive fashion. As a result, it may be concluded that RyR and  NCX are coupled in series, sequentially transporting Ca  2+  to be extruded to the extracellular  space.  132  Figure Evidence of functional N C X and RyR coupling in ECs. Representative traces  (from left to right) of control (black solid trace), ONa-treated (light gray dashed trace), and 100 p M ryanodine + ONa-treated (dark gray dotted trace) ACh-induced [Ca ]j responses (representative of n = 7 experiments). At the control trace, the slower [Ca ]; decline under 100 p M ryanodine treatment (gray solid trace) from another experiment is shown here as a reference. The downstroke of the control response was superimposed on the ONa- and 100 u M ryanodine + ONa-treated responses for comparison. 2+  2+  133  Figure Summarized data of C a  removal rates of RyR- &/or NCX-inhibited E C s .  Data from experiments illustrated in Figure were pooled together and were normalized to the maximal [Ca ]i achieved in ONa treatment. Compared to vontrol, [Ca ]i removal rates were reduced to the same extent under R y R &/or NCX blockade (total of n = 7 experiments for each treatment). 2+  2+  134  5.2.6. Ryanodine Receptors Act As a Link Between S E R C A and N C X  Having identified the relationship between RyR and NCX in extruding Ca  2+  from ECs,  the next step was to confirm whether RyR is a component of the SERCA-NCX Ca extrusion 2+  pathway reported in Section 5.2.1. More specifically, experiments were conducted to determine if SERCA serves as the Ca transporter upstream of RyR, which then delivers Ca to NCX for 2+  2+  extrusion. The reversible SERCA blocker cyclopiazonic acid (CPA, 15 uM) was added to ECs and [Ca ]i decline rates with and without additional treatment of the RyR activator ryanodine (1 2+  pM) were compared. In Figure (representative of n = 10), the CPA-treated response (light gray dashed trace) showed slower [Ca ]i decay when compared to control (black solid 2+  trace). Despite opening RyRs (dark gray dotted trace) by 1 uM ryanodine, Ca  2+  removal was  slower when SERCA was inhibited altogether. Summarized data were shown in Figure The finding in this section suggested that the proposed RyR-mediated Ca extrusion pathway is 2+  effectively blocked once SERCA is inhibited. In addition to the data in Section 5.2.5 which states that RyR and NCX are part of the same Ca extrusion pathway, it can be concluded that 2+  this pathway also consists of SERCA.  135  Figure Effects of S E R C A blockade and RyR opening on C a extrusion from ECs. Representative traces (from left to right) of control (black solid trace), CPA-treated (light gray dashed trace), and 1 p M ryanodine + CPA-treated (dark gray dotted trace) ACh-induced [ C a ] i responses (representative o f n = 10 cell clusters). For the CPA-treated responses, the C P A induced gradual [Ca J! increases (shown between the thin dotted vertical lines) were achieved prior to addition o f A C h . The downstroke o f the control A C h response was superimposed on the C P A - and C P A + 1 p M ryanodine-treated responses for comparison. 2+  2+  136  Figure Summarized data of C a removal rates of C P A (+/- 1 u M ryanodine)2+ treated ECs. Blockade of SERCA with CPA significantly reduced Ca removal rate, as also 2 +  shown earlier in Figure In the presence of 1 pM ryanodine, although RyR was activated, the SERCA-inhibited Ca removal was still slower than control. 2+  —  o a > (A  3  (0  o •a  control CPA C P A + 1 n M ryanodine  P < 0.05 vs. control  +  CM  # ••O-  2 ^  a> N  o c  1 H  Rt &-  75 > o  E  a> + CM  ro O  i  0  — i —  — i —  10  20  30  % normalized control [Ca  40  50  2+, ]j  137  5.2.7. Fluorescent Labeling of Ryanodine Receptors  Ziegelstein et al. (1994) and Wang et al. (1995) have reported evidence for the presence of RyRs in ECs. In the above sections, data for the functional roles of RyRs have been presented. Up until now, RyR localization in freshly isolated ECs have not been visualized fluorescently. In this study, ECs were loaded with the fluorescent RyR indicator BODIPY TR-X-ryanodine (1 pM for 15 minutes, n = 4 experiments). Images of BODIPY TR-X-ryanodine-loaded ECs were taken with an ICCD-coupled confocal microscope at 0.15-pm horizontal sections, and for each stack of images the middle slice is shown (please refer to Section 3.5 for more details on the microscope system). Sample images of BODIPY TR-X-ryanodine-loaded ECs were shown in Figure (left panels). As a negative control (n = 4 experiments), ECs were pretreated with an inhibitory concentration of ryanodine (100 pM) for 15 minutes prior to the application of BODIPY TR-X-ryanodine. At identical confocal microscope settings (e.g. laser power, black level, gain, iris size), prior treatment of 100 uM ryanodine prevented BODIPY TR-X-ryanodine from binding to RyRs and emitting fluorescence (Figure, right panels), demonstrating the binding specificity of the RyR fluorescent indicator. Three-dimensional composites of the same BODIPY TR-X-ryanodine-loaded ECs were shown in Figure  138  ECs were treated with the specific fluorescent RyR ligand (1 pM BODIPY TR-X ryanodine) for 15 minutes with or without prior incubation of 100 pM ryanodine (representative of n = 4 experiments). These images were captured with an ICCD-coupled confocal microscope at a slice thickness of 0.15 pm. The images on the left illustrate BODIPY TR-X ryanodine fluorescence on RyRs. On the right are negative controls; ryanodine pre-treatment prevented BODIPY TR-X ryanodine binding to RyRs, thus no fluorescence was visible. All images were captured with the same microscope settings. Figure BODIPY TR-X-ryanodine labeling of RyRs in ECs.  BODIPY TR-X  B O D I P Y T R - X + 100 tiM ryanodine  139  Figure  Three-dimensional  composites of the BODIPY TR-X-ryanodine-labeled  ECs. The images shown here were compiled from the stack of images taken from the same cells in Figure Details on the preparation of the three-dimensional images were explained in Section 3.6.4.  140  5.2.8. C a  2 +  Removal via Plasma Membrane Ca -ATPase ( P M C A ) after N C X (and RyR) 2+  Blockade  It has been shown earlier that significant amount of Ca was extruded, albeit at a slower 2+  rate, from ECs even after blockade of the SERCA-RyR-NCX pathway. The NCX-independent Ca extrusion mechanism is probably via PMCA. As described in Section 5.2.5, the reduction 2+  of [Ca ]i decline rates in ONa, 100 pM ryanodine, and ONa + 100 pM ryanodine treatments were 2+  not distinguishable. The 0Na environment is sufficient in abolishing the entire SERCA-RyR+  NCX pathway.  Thus, for this part of the experiments, ONaPSS was used as the tool to  investigate non-NCX-associated Ca  2+  extrusion.  ACh-induced [Ca ]i responses were first 2+  recorded in ONaPSS. Subsequently ECs were treated with the PMCA inhibitor carboxyeosin (CE, 25 pM) in the continual absence of extracellular Na . Figure shows representative +  traces (from n = 5 experiments) of the inhibition of Ca removal by CE on top of NCX blockade. 2+  It is clear that ACh-induced [Ca ]i increase was higher in the presence of CE, indicating a 2+  compromised Ca removal system when PMCA is blocked. Average Ca removal rates, binned 2+  2+  as in the previous sections and summarized in Figure, showed marked inhibition of Ca extrusion by simultaneous NCX and PMCA blockades.  141  Figure  Contribution of P M C A to C a  2 +  removal in ECs. Representative traces  showing ACh-induced [Ca ]j responses in ONaPSS and the slower [Ca ]i decay phase under 25 pM carboxyeosin treatment in ONaPSS (representative of n = 5 experiments). Carboxyeosin is an inhibitor of the PMCA. Only ONa treatment was used here to compare to the actions of carboxyeosin since it has been established in the earlier experiments that ONaPSS effectively 2+  2+  2"1"  blocked the RyR-NCX Ca extrusion pathway.  0  200  400  600  800  1000  Time (seconds)  142  Figure Summarized data of Ca  removal rates of ONa (+/-carboxyeosin)-treated  ECs. By inhibiting the NCX, Ca removal rate was significantly reduced. Treatment of carboxyeosin on top of ONa resulted in further slowing of Ca removal in a total of n = 5 experiments. Note: Ca removal rates from control experiments were reproduced from Figure and shown here for comparison. 2+  2+  2+  143  5.2.9. Schematic Model of C a  z +  Removal Pathways in ECs  The current understanding of how elevated Ca  2+  is removed from the cytosol of freshly  isolated endothelial cells is shown in Figure In brief, the ER and the PM are tightly associated by an intact cytoskeleton. The cytoskeletal network is essential in maintaining an inseries Ca removal pathway after agonist stimulation. This pathway involves the following Ca 2+  2+  handling sequences: 1) Ca uptake into the ER by SERCA; 2) ER Ca release via RyR; and 3) 2+  2+  Ca extrusion via NCX to the extracellular space. PMCA functions in a parallel mechanism to 2+  extrude Ca when the SERCA-RyR-NCX pathway is blocked. 2+  144  Figure  Schematic model of C a  2 +  removal pathways in ECs. Cytosolic C a  2+  is  removed by sarco(endo)plasmic reticulum Ca -ATPase (SERCA) into the endoplasmic reticulum (ER), released from the E R via ryanodine receptors (RyRs), and extruded into the extracellular space via the Na /Ca exchanger (NCX). This mode of C a removal is dependent on an intact cytoskeleton. When the SERCA-RyR-NCX pathway is inhibited, the plasma membrane Ca -ATPase (PMCA), which acts in parallel to extrude C a , becomes the sole C a transporter to deliver C a to the extracellular space. 2+  +  2+  2+  2+  2+  2+  2+  145  5.3. Discussion The importance of Ca  2+  extrusion in endothelial Ca  emphasized enough until recently.  2+  homeostasis has not been  Much effort has been devoted in examining Ca  entry  mechanisms, but relatively poor understanding of the mechanisms of removing cytosolic Ca in 2+  the endothelium remains. Known Ca transporters in ECs, including SERCA, NCX and PMCA, 2+  were evaluated with respect to their contribution to Ca removal in this study. ER Ca 2+  channels such as  IP3R  2+  release  and RyR also function to regulate [Ca ]i, although the former mainly 2+  mediate agonist-induced [Ca ]i increase. 2+  Elevations in cytosolic [Ca ]i are generally not 2+  detected by RyR opening in ECs. In bovine ECs, RyRs have been shown to localize in the ER membrane facing the subplasmalemmal space, mediating store-operated Ca  2+  entry and  endothelial nitric oxide synthase activity (Paltayf-Doburzynska et al. 1998). The localization of RyRs near the PM probably coincides with the dependence of the SERCA and NCX on the intact cytoskeleton in facilitating Ca  2+  extrusion.  Thus, the roles of various endothelial Ca  2+  transporters in removing cytosolic Ca were thoroughly investigated in this study. 2+  5.3.1. Structural Arrangement of S E R C A and N C X in Removal of C a  2 +  from E C s  One mechanism via which elevated Ca is removed from the cytosol in ECs is through 2+  the NCX, as shown by the slower [Ca ]i decline in the ONaPSS treatment in Figure 2+  Blockade of NCX activity by removing extracellular Na (and substituting with equimolar of +  NMDG to maintain a constant osmolarity), despite having non-specific effects, is preferred over other more selective agents.  Bepridil and benzamil are two examples of selective N C X  inhibitors; however, reports have documented the use of both drugs to block K channels +  (Yumoto et al. 2004; Su et al. 2000). In contrast, the only side effect of ONaPSS is its potential inhibition of the Na /H antiporter (NHA). +  +  It has been shown in another study on rabbit  146  endothelium that NHA blockade has no effect on intracellular pH and [Ca ]i (Li and van Breemen 1995). Thus, resulting [Ca ]i decline rate reduction from ONaPSS treatment in this 2+  study was solely attributed to the inhibitory effect on the NCX. The NCX is the final structure where Ca  2+  passes through before being extruded to the  extracellular space. The route of Ca transport before reaching the NCX from the cytosol was 2+  resolved by experiments manipulating SERCA activity. CPA constitutes a better choice for blocking SERCA than thapsigargin because of the latter's irreversible binding to SERCA and the induction of apoptotic events (Bai et al. 1999). As shown in Figures and, the sizes of [Ca ]i decline rate decrease were the same in ONaPSS, CPA, and ONaPSS + CPA treatments. 2+  This finding implies that the amount of Ca passing through either or both of SERCA and NCX 2+  is equal. The only explanation for this phenomenon is that SERCA and NCX are arranged in series, sequentially handling Ca  2+  to be eventually extruded. When one component of this in-  series arrangement is taken away, the entire pathway fails to function properly, thus slowing Ca extrusion. In order for the SERCA-NCX Ca  2+  removal pathway to be effective, the two Ca  2+  transporters must lie relatively close to each other. It is clear that SERCA is located on the ER membrane while NCX is situated on the PM. The mechanism underlying the correct alignment of the two independent membranes is worthy of investigation. During Ca  2+  influx in smooth  muscle, the superficial sarcoplasmic reticulum sequesters considerable amounts of Ca Breemen et al. 1995). The SBB relies on the proximity between Ca  2+  2+  (van  influx channels and the  SERCA, very much analogous to the proposed apposition of SERCA and NCX in ECs. Thus, a similar SBB model may be applicable to endothelial Ca regulation, with partial sequestration of 2+  cytosolic Ca into the superficial ER prior to extrusion via NCX. The distribution of superficial 2+  147  and central ER in the cell is unlikely a result of occurrence by chance. Subcellular organelles are known to be held in their respective locations by means of a cytoskeletal network, consisting of microtubules and actin filaments (Alberts et al. 1998). Experiments in Section 5.2.2 showed that an intact cytoskeleton maintains the SERCA-NCX alignment in ECs. Both cytochalasin D and latrunculin A, disrupting the cytoskeletal components via different mechanisms, broke apart the sequential linkage of SERCA and NCX. As a result, [Ca ]i decline rate was reduced further 2+  when SERCA and NCX were blocked simultaneously. With the modified cytoskeleton, SERCA and NCX no longer act in series but remove Ca independently of each other. 2+  5.3.2. Modulation of RyR Activity by Selective Pharmacological Agents  The SERCA-NCX Ca  2+  extrusion pathway is not complete without a Ca -release 2+  channel that exports the Ca from the ER. In this study, RyR was proposed as the link between 2+  SERCA and NCX. Before presenting data supporting this claim, the pharmacology of RyRs is first discussed. Caffeine and ryanodine were used here to modulate RyR activity. Caffeine has been extensively used to stimulate Ca -induced Ca release via RyRs in both skeletal, cardiac, 2+  2+  and smooth muscle (Copello et al. 2002; Kettlun et al. 2003). However, the effect of caffeine is not limited to RyRs, since IP R activity is also inhibited (Bezprozvanny et al. 1994). Despite 3  caffeine's IP3-inhibitory effects, its use did not pose any problem in this study.  In the  experiments, the IP3-mobilizing agonist ACh was removed after [Ca ]i reached a maximum. 2+  Extracellular Ca  2+  was also removed at the same time. Theoretically Ca  2+  release and influx  were both abolished soon, if not immediately afterward. As illustrated in Figures and, the caffeine-induced increase in [Ca ]j decline rate occurred towards the lower 2+  intracellular Ca concentrations, i.e. when [Ca ]; has been decaying for some time, and [Ca ]i 2+  2+  has almost returned to baseline level. By that time, it was speculated that  2+  IP3RS  and IP3-  148  mediated Ca release contributed minimally to the measured [Ca ];. Besides, 1 uM ryanodine 2+  2+  and caffeine treatments shared a similar pattern in increasing [Ca ]j decline rates (Figure 2+ Since ryanodine is a highly selective RyR modulator (see the following paragraph) with no known IP R effects, it can be assumed that the common effects of ryanodine and caffeine on 3  Ca clearance is due to the same RyR activating effects in ECs. 2+  Ryanodine was the other drug used to modulate RyR activity in this study. Despite its specificity at RyRs, ryanodine has opposite effects on the RyR, owing to the complicated pharmacology of the receptor.  Several reports and review articles have documented the  concentration dependency of ryanodine's actions in different tissues (Paltauf-Doburzynska et al. 1998; Fill and Copello 2002; Meissner 1986; Buck et al. 1992). It is generally agreed that ryanodine in the micromolar range tends to increase RyR opening probability. configuration, the RyR remains active and consistently releases ER Ca . 2+  In this  At higher  concentrations, e.g. 100 pM, ryanodine initially opens RyR, subequently locks it in a lowconductance or closed state, and Ca  2+  release is inhibited eventually (Fill and Copello 2002).  This characteristic of ryanodine was also revealed in the data shown in Section 5.2.3 and is discussed in Section 5.3.5. 5.3.3. Other Potential RyR Modulators  There are many other commercially available pharmacological agents that elicit specific effects on RyRs. However their use was not practical in this study because of various reasons. Cyclic-ADP-ribose (cADPR) is a physiological RyR activator, but its inability to stimulate skeletal and cardiac RyRs has also been demonstrated, thus raising the possibility of multiple physiological stimuli for RyRs (Copello et al. 2001).  Besides, cADPR is membrane-  impermeable and its administration requires permeabilised cells, which will not allow the  149  measurement of [Ca ]i decline. Local anesthetics (LAs) such as tetracaine and procaine are not 2+  membrane impermeant, but are probably very poorly diffusible across the PM. The poor permeability may be the result of the LA's cationic properties in solution. In order to reach the cytosol, the LA mustfirstbecome nonionic. Thus, a charged-uncharged equilibrium governs the permeability of LAs. However, after getting across the PM the LA still needs to bind to the RyRs in the ER. According to several reports using LAs to inhibit ER Ca  2+  release in various  cell types (Lukyanenko et al. 2001; Lilly and Gollan 1995; Inoue et al. 2003; Turner et al. 2001), the effective concentrations of tetracaine and procaine are, respectively, 0.1 - 0.5 mM and 5-10 mM.  The poor permeability of LAs is not only suggested by the use of millimolar  concentrations in these studies, but is also illustrated by the fact that permeabilized cells were used in the above cited reports. It is highly questionable that similar concentrations of tetracaine or procaine would be effective in blocking RyRs in the intact ECs in this study.  Most  importantly, the LAs may induce non-specific side effects at such high concentrations. Another drug, ruthenium red was shown by Hoogduijn et al. to block RyRs in intact embryonic kidney cells (Hoogduijn et al. 2002). Unfortunately ruthenium red also blocks mitochondrial Ca  2+  transport and requires membrane permeabilization in most other cells. 5.3.4. Role of RyR in Removing Cytosolic C a  2 +  and Depleting E R C a  2 +  In Figures and, 1 pM ryanodine treatment, by opening RyRs, was shown to result in a faster Ca  2+  removal rate while 100 pM ryanodine inhibited Ca  2+  extrusion by  blocking RyRs. Low and high concentrations of ryanodine also produced different extents of ER Ca  2+  depletion when ECs were left in OCaPSS for a 15-minute period (Figure Both 15  mM caffeine and 1 pM ryanodine activated RyRs, but the higher Ca and occurred before significant ER Ca  2+  2+  removal rates (Figures  loss was detected (Figure The  150  different onset times of caffeine or ryanodine effects may be attributed to two main factors: 1) different parameters were being measured and 2) measurements were done under different conditions. The effect of caffeine or ryanodine was seen quickly when the Ca removal rate was 2+  measured, and for these measurements [Ca ]j was elevated as a result of ACh stimulation with 2+  RyRs actively handling ER Ca . On the contrary, when caffeine or ryanodine was incubated in 2+  OCaPSS in the measurement of ER Ca loss, RyRs were activated under basal [Ca ]j conditions, 2+  2+  i.e. ECs were not stimulated with ACh in the process. Thus, the difference in observed effect times of 1 pM ryanodine and 15 mM caffeine in Figures, and did not contradict each other, but rather converged to the same conclusion that open RyRs promote both ER Ca depletion and Ca extrusion. It is interesting to note that the concentration range of the 2+  2+  biphasic ryanodine effects in the fresh rabbit ECs differed somewhat from those previously reported. For example, Paltauf-Doburzynska et al. (1998) showed that 25 pM ryanodine blocks RyRs in cultured bovine ECs whereas Turner et al. (2001) reported that in cultured guinea pig neurons, 1 pM ryanodine is already an inhibiting dose. It is possible that heterogeneity of RyR isoforms underlies this tissue- and species-dependent variability in ryanodine sensitivity. 5.3.5. Position of RyR in the S E R C A - N C X C a  2 +  Removal Pathway  The relationships between RyR & SERCA and RyR & NCX in Ca removal were shown 2+  in Figures and Before these experiments were done, all is known is that both SERCA-NCX and RyR contribute to Ca extrusion in ECs. Although the data so far agree with 2+  the proposed SERCA-RyR-NCX pathway, no concrete evidence has been shown yet. ECs were treated with 100 pM ryanodine and ONaPSS so that both RyR and NCX were blocked. If RyR and NCX were not functionally coupled in an in-series manner, similar to that between NCX and SERCA, the result in Figure should indicate a further slowing of [Ca ]i decline. The fact 2+  151  that [Ca ]i decline rate was reduced to the same degree in treatments of ONaPSS, 100 uM 2+  ryanodine, and ONaPSS + 100 uM ryanodine suggests that RyR and NCX are components of the same Ca removal pathway. 2+  The next issue is between SERCA and RyR - whether these two Ca  2+  transporters  function in series. Instead of blocking RyRs here, RyRs were activated by 1 uM ryanodine. The purpose of combining RyR activation and SERCA blockade was to determine if SERCA is the first component of the proposed pathway. From Section 5.2.1, it is clear that SERCA inhibition decreased Ca  2+  removal rate while in separate experiments RyR activation facilitated C a  2+  removal. If, during SERCA blockade, active RyR opening still increases Ca removal rate, then 2+  either SERCA is not the only ER Ca uptake mechanism or RyR does not belong to the same 2+  SERCA-NCX pathway. Figure shows that SERCA inhibition with or without actively 2_|_  opening RyRs resulted in the same reduction of [Ca ]\ decline rate. Thus, the conclusion is that SERCA, RyR and NCX 1) remove cytosolic Ca in this order; 2) are arranged in series; and 3) 2+  are components of the same Ca extrusion pathway in ECs. 2+  5.3.6. Visualization of Ryanodine Receptors in Fresh Endothelial Cells  Prior to this study, RyRs in fresh ECs have not been visualized with fluorescence microscopy. In order to gain more information related to the localization of these receptors, RyRs were labelled with BODIPY TR-X-ryanodine. In other cells, BODIPY TR-X-ryanodine has been documented as a selective RyR ligand (Varadi and Rutter 2002). The specificity of BODIPY TR-X-ryanodine in fresh ECs is demonstrated in Figure, where pre-incubation of 100 pM ryanodine completely prevented receptor binding of the RyR label.  The main  conclusion from these micrographs is that the ECs do possess RyRs and that they may well be located peripherally. However to prove this point in these relatively small cells would require a  152  much better spatial resolution as could be obtained with immunogold electron microscopy. Despite the evidence for RyRs in ECs, caffeine failed to induce a [Ca ]; transient as shown by 2+  Wang et al (1995). This apparent paradox could be explained by the fact that most RyRs are located on the peripheral ER. Most of the Ca released via RyRs is probably directed towards 2+  the NCX and extruded before reaching the cytosol. In another study, Lesh et al. (1993) showed extensive staining of anti-RyR antibody in the cytosol of guinea pig aortic endothelium. The variations in endothelial RyR distribution among different species may be the reason for tissuespecific caffeine-induced [Ca ]i responses, e.g. in bovine (Buchan and Martin 1991) and 2+  cultured human ECs (Neylon and Irvine 1990). Based on existing data, it may be concluded that RyR distribution varies among different tissues and species. 5.3.7. Effect of Combined P M C A - and NCX-Inhibition on C a  2 +  Extrusion  In addition to demonstrating the in-series arrangement of SERCA, RyR and NCX in a common Ca  2+  removal pathway, another ER-independent Ca  2+  extrusion mechanism was also  uncovered. This mode of Ca extrusion acts in parallel to NCX and is undoubtedly the PMCA. 2+  No specific PMCA blocker is available at present, but some studies have reported PMCAinhibitory effects of carboxyeosin (Moccia et al. 2002; Bassani et al. 1995) and caloxin (Chaudhary et al. 2001). Carboxyeosin (CE) was the choice of PMCA blocker in this study. As shown in Figure, CE further inhibited Ca  2+  removal on top of NCX blockade. This  marked inhibition of Ca extrusion after blockade of NCX is consistent with Ca extrusion via 2+  2+  two parallel pathways: the PMCA and the composite of SERCA-RyR-NCX. The gradual [Ca ]i 2+  decay seen in the ONaPSS + CE treatment could be due to incomplete blockade by CE or may be complicated by cell mortality after this extreme intervention (unpublished observations). It is also possible that mitochondria become more active in Ca  2+  removal, compensating for the  153  prolonged [Ca ]\ elevation. Future experiments where only the PMCA blocker (CE or other potential PMCA inhibitory agents) is used will be necessary in order to evaluate the percent contribution of PMCA alone in extruding Ca from ECs. 2+  154  C H A P T E R VI: G E N E R A L C O N C L U S I O N S A N D F U T U R E DIRECTIONS The current work represented the first attempt to jointly study the Ca properties in endothelial cells and valvular myofibroblasts.  2+  signaling  These two types of cells are  important regulators of a normal cardiac valve, and are modified significantly in a diseased valve. Much is known about the physiological and signaling aspects of ECs, but very few reports have examined the biology of VMFs.  The different levels of knowledge about ECs and VMFs  necessitated an experimental design with two foci. Without any previous work done on the signaling properties of the VMFs, the first focus of the study was to consider the fundamentals, i.e. the characteristics of receptor/channel-mediated Ca  2+  signals in these cells. In cultured  human VMFs, functional H]R, P2Y2R, and SOCs were identified pharmacologically and were found to elicit different Ca mobilizing patterns. For instance, P2Y R activation, but not that of 2+  2  HiR, induced Ca  2+  entry.  In addition, IP3-sensitive and IP3-insensitive intracellular C a  2+  compartments were identified. The second focus of the study was to elucidate the details of cytosolic Ca pathways.  2+  removal from ECs, building upon a wealth of existing literature on Ca  2+  entry  By using an established model of freshly isolated aortic ECs, which are  physiologically representative of ECs in general, two parallel Ca  2+  removal mechanisms were  elucidated. After agonist stimulation, cytosolic Ca was extruded from the ECs via the PMCA and the composite of SERCA-RyR-NCX. This study has thus contributed to our understanding of endothelial Ca  2+  homeostasis, as well as Ca  comprehensive investigation of Ca  2+  signaling mechanisms in VMFs.  A more  regulation in VMFs is certainly required in future valvular 2_|_  research. This can be achieved, for example, by exploring the Ca signaling characteristics of other vasoactive substances. Regarding the histaminergic and purinergic signaling pathways, efforts can be devoted in outlining the activation/deactivation of enzymes secondary to Ca 155  mobilization. It is interesting to note that what is now known about the VMFs is somewhat similar to the findings in smooth muscle cells a couple decades ago. Thus, future studies with VMFs may also follow some of the approaches used with smooth muscle cells before. A good method is to use a bioassay system to measure VMF functions (e.g. contractility) in response to endothelial secretions.  In the bioassay system, different endothelial secretions may be  synthesized by challenging the ECs with different agonists or by manipulating the activity of Ca  2+  transporters responsible for extrusion. A better insight into the effects of endothelial  releases on VMF responses may thus be gained. In addition to measuring contractile responses, the production of ECMs by VMFs (with or without endothelial influences) may also be determined by histochemical techniques. However, in vivo interactions between ECs and VMFs are resembled only when the intact valve is studied. With the advancement of imaging and electrophysiological techniques, simultaneous measurements of ionic concentrations and currents in ECs and VMFs in an intact valve should be a realistic goal in resolving the mystery around the development of valvular heart diseases.  156  BIBLIOGRAPHY Alberts B, Bray D, Johnson A, Lewis J, Raff M , Roberts K, Walter P. 1998. Cytoskeleton. In: Essential Cell Biology. Garland Publishing, New York, 513-546. Alderton JM, Steinhardt RA. 2000. Calcium influx through calcium leak channels is responsible for the elevated levels of calcium-dependent proteolysis in dystrophic myotubes. J Biol Chem 275: 9452-9460. Alexander SPH, Peters JA. 1999. Receptor and ion channel nomenclature supplement. Elsevier, Cambridge, 64-67. Alpert JS, Dalen JE, Rahimtoola SH (eds). 2000. Valvular Heart Disease, 3/e. Lippincott Williams and Wilkins, New York, 1-464. Babe Jr KS, Serafin WE. 1996. Histamine, bradykinin, and their antagonists. In: Goodman and Gilman's the pharmacological basis of therapeutics. Hardman JG, Limbird LE (eds). McGrawHill, Toronto, 581-582. Bai JZ, Saafi EL, Zhang S, Cooper GJ. 1999. Role of Ca amylin in pancreatic islet beta-cells. Biochem J 343: 53-61.  2+  in apoptosis evoked by human  Bakker RA, Timmerman H, Leurs R. 2002. Histamine receptors: specific ligands, receptor biochemistry, and signal transduction. Clin Allergy Immunol 17: 27-64. Bartholeyns J, Boucher M. 1984. Involvement of histamine in growth of mouse and rat tumors: antitumoral properties of monofluoromethylhistidine, and enzyme-activated irreversible inhibitor of histidine decarboxylase. Cancer Res 44: 639-645. Bartholeyns J, Fozard JR. 1985. Role of histamine in tumor development. Trends Pharmacol Sci 6: 123-125. Bashey Rl, Jimenez SA. 1988. Collagen in heart valves. In: Collagen, vol.1. Nimni ME (ed). Boca Raton, CRC Press, 273-292. Bassani RA, Bassani JW, Bers DM. 1995. Relaxation in ferret ventricular myocytes: role of the sarcolemmal Ca -ATPase. Pflugers Arch 430: 573-578. 2+  Batten P, McCormack A M , Rose ML, Yacoub MH. 2001. Valve interstitial cells induce donorspecific T-cell anergy. J Thorac Cardiovasc Surg 122: 129-135. Bean BP. 1992. Pharmacology and electrophysiology of ATP-activated ion channels. Trends Pharmacol Sci 13: 87-90. Becker AE. 1998. Acquired heart valve pathology. An update for the millennium. Herz 23: 415-419. Bernardi M , Galeazzi G, Lamura E, Piantelli F, Rendell J, Rossini L, Rossini P. 1997. (ECTO) nucleotidase kinetics observed by P-NMR spectroscopy: resolution of signals. Pharmacol Rev 36: 353-361. 3I  Berridge MJ, Bootman MD, Roderick HL. 2003. Calcium signaling: dynamics, homeostasis and remodelling. Nature Rev Mol Cell Biol 4: 517-529.  157  Betz AL. 1983. Sodium transport in capillaries isolated from rat brain. J Neurochem 341: 1150-1157. Bezprozvanny I, Bezprozvannaya S, Ehrlich BE. 1994. Caffeine-induced inhibition of inositol(l,4,5)-trisphosphate-gated calcium channels from cerebellum. Mol Biol Cell 5: 97-103. Bodin P, Milner P, Winter R, Burnstock G. 1992. Chronic hypoxia changes the ratio of endothelin to ATP release from rat aortic endothelial cells exposed to high flow. Proc R Soc LondB Biol Sci 247: 131-135. Boulanger C, Luscher TF. 1990. Release of endothelin from the porcine aorta. Inhibition by endothelium-derived nitric oxide. J Clin Invest SS: 587-590. Brini M, Carafoli E. 2000. Calcium signaling: a historical account, recent developments and future perspectives. Cell Mol Life Sci 57: 354-370. Buchan KW, Martin W. 1991. Bradykinin induces elevations of cytosolic calcium through mobilization of intracellular and extracellular pools in bovine aortic endothelial cells. Br J Pharmacol 102: 35-40. Buck E, Zimanyi I, Abramson JJ, Pessah IN. 1992. Ryanodine stabilizes multiple conformational states of the skeletal muscle calcium release channel. J Biol Chem 267: 2356023567. Busse R, Fleming I. 2003. Regulation of endothelium-derived vasoactive autacoid production by hemodynamic forces. Trends Pharmacol Sci 24: 24-29. Buvinic S, Briones R, Huidobro-Toro JP. 2002. P 2 Y i and P2Y2 receptors are coupled to the NO/cGMP pathway to vasodilate the rat arterial mesenteric bed. Br J Pharmacol 136: 847-856. Camello-Almaraz C, Pariente JA, Salido G, Camello PJ. 2000. Differential involvement of vacuolar H -ATPase in the refilling of thapsigargin- and agonist-mobilized Ca stores. Biochem Biophys Res Commun 271: 311-317. +  2+  Campbell WB, Gebremedhin D, Pratt PF, Harder DR. 1996. Identification of epoxyeicosatrienoic acids as endothelium-derived hyperpolarizing factors. Cire Res 78: 415-423. Carey DJ. 1991. Control of growth and differentiation of vascular cells by extracellular matrix proteins. Ann Rev Physiol 53: 161-177. Chaudhary J, Walia M , Matharu J, Escher E, Grover AK. 2001. Caloxin: a novel plasma membrane Ca2+ pump inhibitor. Am J Physiol 280: C1027-1030. Chester AH, Misfeld M , Yacoub MH. 2000. Receptor-mediated contraction of aortic valve leaflets. J Heart Valve Dis 9: 250-255. Chew CS. 1985. Differential effects of extracellular calcium removal and non-specific effects of Ca antagonists on acid secretory activity in isolated gastric glands. Biochim Biophys Acta 846: 370-378. 2+  ClaphamDE. 1995. Calcium signaling. Cell 80: 259-268. Connolly HM, Crary JL, McGoon MD, Hensrud DD, Edwards BS, Edwards WD, Schaff HV. 1997. Valvular heart disease associated with fenfluramine-phentermine. NEngJMed337: 581588.  158  Copello JA, Barg S, Sonnleitner A Porta M, Diaz-Sylvester P, Fill M, Schindler H, Fleischer S. 2002. Differential activation by Ca , ATP and caffeine of cardiac and skeletal muscle ryanodine receptors after block by Mg . J Membr Biol 187: 51-64. 2+  2+  Copello JA, Qi Y, Jeyakumar LH, Ogunbunmi E, Fleischer S. 2001. Lack of effect of cADPriboase and NAADP on the activity of skeletal muscle and heart ryanodine receptors. Cell Calcium 30: 269-284. Davidge ST. 2001. Prostaglandin H synthase and vascular function. Circ Res 89: 650-660. De Oliveria CA, Mantovani B. 1988. Latrunculin A is a potent inhibitor of phagocytosis by macrophages. Life Sci 43: 1825. Dedkova E, Blatter LA. 2002. Nitric oxide inhibits capacitative Ca entry and enhances endoplasmic reticulum Ca uptake into bovine vascular endothelial cells. J Physiol 539: 77-91. 2+  2+  Demers P, Elkouri S, Sirois MG, Carrier R. 2001. Coronary artery endothelial dysfunction after ischemia-reperfusion and acute untreated rejection in a canine heterotopic heart transplanatation model. Transplantation 71: 26-32. Dimmeler S, Fleming I, Fisslthaler B, Hermann C, Busse R, Zeiher A M . 1999. Activation of nitric oxide synthase in endothelial cells by Akt-dependent phosphorylation. Nature 399: 601605. Dooley S, Delvoux B, Lahme B, Mangasser-Stephan K, Gressner A M . 2000. Modulation of transforming growth factor beta response and signaling during transdifferentiation of rat hepatic stellate cells to myofibroblasts. Hepatology 31: 1094-1106. Drexler H. 1997. Endothelial Factors. In: Heart Failure. Poole-Wilson P, Colucci W, Massie B, Chatterjee K, Coats A (eds). Churchill Livingstone, New York, 173-186. Dubyak GR, el-Moatassim C. 1993. Signal transduction via P2-purinergic receptors for extracellula ATP and other nucleotides. Am J Physiol 265: C577-C606. Dunn PM, Blakeley AGH. 1988. Suramin: a reversible p2-purinoceptor antagonist in the mouse vas deferens. Br J Pharmacol 93: 243-245. Durbin AD, Gotlieb AI. 2002. Advances towards understanding heart valve response to injury. Cardiovasc Pathol 11: 69-11. Edwards G, Dora KA, Gardener MJ, Garland CJ, Weston AH. 1998. K is an endotheliumderived hyperpolarizing factor in rat arteries. Nature 396: 269-272. +  Eisner DA, Trafford AW, Diaz ME, Overend CL, O'Neill SC. 1998. The control of Ca release from the cardiac sarcoplasmic reticulum: regulation versus autoregulation. Cardiovasc Res 38: 589-604/ Ely SW, Berne RM. 1992. Protective effects of adenosine in myocardial ischemia. Circulation 85: 893-904. Emerson GG, Segal SS. 2000. Endothelial cell pathway for conduction of hyperpolarization and vasodilation along hamster feed artery. Circ Res 86: 94-100. Farb A, Virmani R, Burke AP. 2000. Pathogenesis and Pathology of valvular heart disease. In: Valvular Heart Disease, 3/e. Alpert JS, Dalen JE, Rahimtoola SH (eds). Lippincott Williams and Wilkins, New York, 1-39. 159  Ferraris VJ, Rodriguez ER. 1991. Ultrastructure of the normal heart. In: Cardiovascular Pathology. Silver M (ed). Churchill Livingstone, New York. 43-101.  Filip DA, Radu A, Simionescu M . 1986. Interstitial cells of the heart valves possess characteristics similar to smooth muscle cells. Circ Res 59: 310-320. Fill M , Copello JA. 2002. Ryanodine receptor calcium release channels. Physiol Rev 82: 893922. Fitzgerald LW, Burn TC, Brown BS, Patterson JP, Corjay MH, Valentine PA, Sun JH, Link JR, Abbaszade I, Hollis JM, Largent BL, Hartig PR, Hollis GF, Meunier PC, Robichaud AJ, Robertson DW. 2000. Possible role of valvular serotonin 5-HT2B receptors in the cardiopathy associated with fenfluramine. Mol Pharmacol 57: 75-81. Flaumenhaft R, Rifkin DB. 1991. Extracellular matrix regulation of growth factor and protease activity. Curr Opin Cell Biol 3: 817-823. Fleetwood G, Coade SB, Goardon JL, Pearson JD. 1989. Kinetics of adenine nucleotide catabolism in coronary circulation of rats. Am J Physiol 256: HI 565-H1572. Flynn ERM, Bradley KN, Muir TC, McCarron JG. 2001. Functional separate intracellular Ca stores in smooth muscle. J Biol Chem 276: 36411-36418.  2+  Frieden M , Graier WF. 2000. Subplasmalemmal ryanodine sensitive Ca release contributes to Ca -dependent K channel activation in a human umbilical vein endothelial cell line. J Physiol 524:715-724. 2+  2+  +  Galvin JE, Hemric ME, Ward K. 2000. Cytotoxic mAb from rheumatic carditis recognizes heart valves and laminin. J Clin Invest 106: 217-224. Gibson A, McFadzean I, Wallace P, Wayman CP. 1998. Capacitative Ca regulation of smooth muscle tone. Trends Pharmacol Sci 19: 266-269.  2+  entry and the  Go Y M , Park H, Maland MC, Darley-Usmar V M , Stoyanov B, Wetzker R, Jo H. 1998. Phosphatidylinositol 3-kinase gamma mediates shear stress-dependent activation of JNK in endothelial cells. Am J Physiol 275: HI 898-H1904. Gotlieb AI, Rosenthal A, Kazemian P. 2001. Fibroblast growth factor 2 regulation of mitral valve interstitial cell repair in vitro. J Thorac Cardiovasc Surg 124: 591-597. Goto Y, Miura M, Iijima T. 1996. Extrusion mechanisms of intracellular Ca in human aortic endothelial cells. Eur J Pharmacol 314: 185-192. 2+  Grigioni F, Enriquez-Sarano M , Ling LH, Bailey KR, Seward JB, Tajik AJ, Frye RL. 1999. Sudden death in mitral regurgitation due to flair leaflet. J Am Coll Cardiol 34: 2086-2087. Grover AK, Sampson SE. 1997. Peroxide resistance of ER Ca pump in endothelium: implications to coronary artery function. Am J Physiol 273: C1250-C1258. 2+  Grynkiewicz G, Poenie M, Tsien RY. 1985. A new generation of Ca improved fluorescence properties. J Biol Chem 260: 3440-3450.  2+  indicators with greatly  Hafizi S, Taylor PM, Chester AH, Allen SP, Yacoub MH. 2000. Mitogenic and secretory responses of human valve interstitial cells to vasoactive agents. J Heart Valve Dis 9: 454-458.  160  Hattori Y. 1999. Cardiac histamine receptors: their pharmacological consequences and signal transuction pathways. Methods Find Exp Clin Pharmacol 21:123-131. Hengstenberg C, Rose ML, Page C, Taylor PM, Yacoub MH. 1990. Immunocytochemical changes suggestive of damage to endothelial cells during rejection of human cardiac allografts. Transplantation 49: 895-899. Hill SJ. 1990. Distribution, properties and functional characteristics of three classes of histamine receptor. Pharmacol Rev 42: 45-83. Hishikawa K, Oemar BS, Yang Z, Luscher TF. 1997. Pulsatile stretch stimulates superoxide producion and activates nuclear factor-kappa-B in human coronary smooth muscle. Circ Res 81: 797-803. Hoogduijn MJ, McGurk S, Smit NP, Nibbering PH, Ancans J, van der Laarse A, Thody AJ. 2002. Ligand-dependent activation of the melannocortin 5 receptor: cAMP production and ryanodine-receptor-dependent elevations of [Ca ],. Biochem Biophys Res Commun 290: 844850. 2+  Hourani SMO, Hall DA, Nieman CJ. 1992. Effects of the P2-purinoceptor antagonist, suramin, on human platelet aggregation induced by adenosine 5'-diphosphate. Br J Pharmacol 105: 453457. Huang A, Sun D, Smith CJ, Connetta JA, Shesely EG, Koller A, Kaley G. 2000. In eNOS knockout mice skeletal muscle arteriolar dilation to acetylcholine is mediated by EDHF. Am J Physiol 278: H762-H768. Hughes MJ, Coret IA. 1972. On specificity of histamine receptors in the heart. Am J Physiol 223: 1257-1262. Iesaki T, Gupte SA, Kaminski PM, Wolin MS. 1999. Inhibition of guanylate cyclase stimulation by NO and bovine arterial relaxation to peroxynitrite and H2O2. Am J Physiol 277: H978-H985. Imaizumi Y, Ohi Y, Yamamura H, Ohya S, Muraki K, Watanabe M. 1999. Ca regulator of ion channel activity. Jpn J Pharmacol 80: 1-8.  2+  spark as a  Inoue R, Tanabe M , Kono K, Maruyama K, Ikemoto T, Endo M. 2003. Ca -releasing effect of cerivastatin on the sarcoplasmic reticulum of mouse and rat skeletal muscle fibers. J Pharmacol Sci 93: 279-88. 2+  Irani K. 2000. Oxidant signaling in vascular cell growth, death, and survival. Circ Res 87: 179183. Jacob R, Merritt JE, Hallam TJ, Rink TJ. 1988. Repetitive spikes in cytoplasmic calcium evoked by histamine in human endothelial cells. Nature 335: 40-45. Jaggar JH, Porter VA, Lederer WJ, Nelson MT. 2000. Calcium sparks in smooth muscle. Am J Physiol 278: C235-C256. Johnson CL, Johnson CG, Bazan E, Garver D, Gruenstein E, Ahluwalia M. 1990. Histamine receptors in human fibroblasts: inositol phosphates, Ca , and cell growth. Am J Physiol 27: C533-543. 2+  161  Johnson JD, VanGoor F, Jobin RM, Wong CJH, Goldberg Jl, Chang JP. 2000. Agonist-specific Ca signaling systems, composed of multiple intracellular Ca stores, regulate gonadotropin secretion. Mol Cell Endocrinol 170: 15-29. 2+  2+  Kaumann AJ, Molenaar P. 1997. Modulation of human cardiac function through 4 betaadrenoceptor populations. Naunyn-Schmiedeberg Arch Pharmacol 355: 667-681. Kettlun C, Gonzalez A, Rios E, Fill M. 2003. Unitary Ca current through mammalian cardiac and amphibian skeletal muscle ryanodine receptor channels under near-physiological ionic conditions. J Gen Physiol 111: 407-417. 2+  Kim K M , Herrera GA, Battarbee HD. 1999. Role of glutaraldehyde in calcification of porcine aortic valve fibroblasts. Am J Pathol 154: 843-852. Kim K M . 1994. Cell death and calcification of canine fibroblasts in vitro. Cells Mater 4: 247261. Knittel T, Mehde M , Grundmann A, Saile B, Schard J, Ramadori G. 2000. Expression of matrix metalloproteinases and their inhibitors during hepatic tissue repair in the rat. Histochem Cell 5/0/113:443-453.  Kohler R, Brakemeier S, Kuhn M, Degenhardt C, Buhr H, Pries A, Hoyer J. 2001. Expression of ryanodine receptor type 3 and TRP channels in endothelial cells: comparison of in situ and cultured human endothelial cells. Cardiovasc Res 51: 160-168. Krsti MK, Stepanovi R, Hi K, Krsti SK. 1996. Endothelium-independent contractile and relaxant responses to histamine in the rabbit aorta and common carotid, mesenteric, renal, and femoral arteries. Gen Pharmacol 11: 529-533. Kuang X , Chan L, Liang W, Laher I, van Breemen C, Wang X. 2003. The role of Kc in endothelial cell hyperpolarization and endothelium-dependent relaxation in the rabbit aorta. In: EDHF 2002. Vanhoutte PM (ed). Taylor and Francis, New York, 274-282. a  Kurki P, Ogata K, Tan EM. 1988. Monoclonal antibodies to proliferating cell nuclear antigen (PCNA)/cyclin as probes for proliferating cells by immunofluorescence microfluorescence microscopy and flow cytometry. J Immunol Methods 109: 49-59. Kuzmin AI, Lakomkin V L , Kapelko VI, Vassort G. 1998. Interstitial ATP level and degradation in control and postmyocardial infarcted rats. Am J Physiol 275: C766-C771. L'Heureux N , Stoclet JC, Auger FA, Lagaud GJ, Germain L, Riantsitohaina R. 2001. A human tissue-engineered vascular media: a new model for pharmacological studies of contractile responses. FASEB J15: 515-524. Laskey RE, Adams DJ, Cannell M , van Breemen C. 1992. Calcium entry-dependent oscillations of cytoplasmic calcium concentration in cultured endothelial cells monolayers. Proc Natl Acad Sci USA 1189: 1690-1694. Lau KL, Kong SK, Ko WH, Kwan HY, Huang Y, Yao X. 2003. cGMP stimulates endoplasmic reticulum Ca(2+)-ATPase in vascular endothelial cells. Life Sci 73: 2019-28. Lavallee M, Takamura M , Parent R, Thorin E. 2001. Crosstalk between endothelin and nitric oxide in the control of vascular tone. Heart Fail Rev 6: 365-376.  162  Lesh RE, Marks AR, Somlyo AV, Fleischer S, Somlyo AP. 1993. Anti-ryanodine receptor antibody binding sites in vascular and endocardial endothelium. Circ Res 72: 481-488. Lester WM, Damji AA, Tanaka M , Gedeon I. 1992. Bovine mitral valve organ culture: role of interstitial cells in repair of valvular injury. J Mol Cell Cardiol 24: 43-53. Lester WM, Gotlieb AI. 1988. In vitro repair of the wounded porcine mitral valve. Circ Res 62: 833-845. Lester WM, Rosenthal A, Granton B, Gotlieb AI. 1988. Porcine mitral valve interstitial cells in culture. Lablnvest59: 710-719. Levy S. 2001. Pharmacologic management of atrial fibrillation: current therapeutic strategies. Am Heart JUV. S15-S21. Li A M . 1993. A study on the changes of myocardial intracellular calcium in patients with heart failure. Zhonghua Xin Xue Guan Bing Za Zhi 21: 207-208 Li L, van Breemen C. 1995. Na -Ca exchange in intact endothelium of rabbit cardiac valve. Circ Res 76: 396-404. +  2+  Lilly LB, Gollan JL. 1995. Ryanodine-induced calcium release from hepatic microsomes and permeabilized hepatocytes. Am J Physiol 268: G l 017-24. Lis Y, Burleigh MC, Parker DJ, Child A H , Hogg J, Davies MJ. 1987. Biochemical characterization of individual normal, floppy and rheumatic human mitral valves. Biochem J 244: 597-603. Lopez JA, Ross RS, Fishbein MC, Siegel RJ. 1987. Nonbacterial thrombotic endocarditis: a review. Am Heart J113: 773-784. Lounsbury K M , Hu Q, Ziegelstein RC. 2000. Calcium signaling and oxidant stress in the vasculature. Free Rad Biol Med 28: 1362-1369. Lukyanenko V, Viatchenko-Karpinski S, Smirnov A, Wiesner TF, Gyorke S. 2001. Dynamic regulation of sarcoplasmic reticulum Ca content and release by luminal Ca(2+)-sensitive leak in rat ventricular myocytes. Biophys J SI: 785-98. 2+  Manabe H, Yutani C. 1998. Atlas of valvular heart disease. Churchill Livingstone, New York, 32,98. Mangion JR, Tighe DA. 1995. Aortic valvular disease in adults. A potentially lethal clinical problem. Postgrad Med 98: 127-135. Marcelin-Jimenez G, Escalante B. 2001. Functional and cellular interactions between nitric oxide and prostacyclin. Comp Biochem Physiol C Toxicol Pharmacol 129: 349-359. Marrelli SP. 2001. Mechanisms of endothelial P 2 Y i - and P2Y2-mediated vasodilation involve differential [Ca ], responses. Am J Physiol 281: H1759-H1766. 2+  Mateo, J, Miras-Portugal MT, Castro E. 1996. Co-existence of P y- and PPADS-sensitive P upurinoceptorsin endothelial cells from adrenal medulla. Br J Pharmacol 119: 1223-1232. 2  2  Matoba T, Shimokawa H, Kubota H, Morikawa K, Fujiki T, Kunihiro I, Mukai Y, Hirakawa Y, Takeshita A. 2002. Hydrogen peroxide is an endothelium-derived hyperpolarizing factor in human mesenteric arteries. Biochem Biophys Res Commun 209: 909-913.  163  McDonald PC, Wilson JE, McNeill S, Gao M, Spinelli JJ, Rosenberg F, Wiebe H, McManus BM. 2002. The challenge of defining normality of human mitral and aortic valves: geometrical and compositional analysis. Cardiovasc Pathol 11: 193-209. Meghji P, Pearson JD, Slakey LL. 1992. Regulation of extracellular adenosine production by ectonucleotidases of adult rat ventricular myocytes. Am J Physiol 263: H40-H47. Mehta D, Izzat MB, Bryan AJ, Angelini GD. 1997. Towards the prevention of vein graft failure. Intl J Cardiol 62: S55-S63. Meissner G. 1986. Ryanodine activation and inhibition of the Ca sarcoplasmic reticulum. J Biol Chem 261: 6300-6306.  2+  release channel of  Messier RH, Bass BL, Aly HM, Jones JL, Domkowski MS, Wallace RB, Hopkins RA. 1994. Dual structure and functional phenotypes of the porcine aortic valve interstitial population: characteristics of the leaflet myofibroblast. J Surg Res 57: 1-21. Mitsuhashi M, Mitsuhashi T, Payan DG. 1989. Multiple signaling pathways of histamine H2 receptors: identification of an H2 receptor dependent Ca mobilization pathway in human HL-60 promyelocytic leukemia cells. J Biol Chem 264: 18356-18362. 2+  Moccia F, Baruffi S, Spaggiari S, Coltrini D, Berra-Romani R, Signorelli S, Castelli L, Taglietti V, Tanzi F. 2001. P2Y1 and P2Y2 receptor-operated Ca signals in primary cultures of cardiac microvascular endothelial cells Microvasc Res 61: 240-252. 2+  Moccia F, Berra-Romani R, Baruffi S, Spaggiari S, Signorelli S, Castelli L, Magistretti J, Taglietti V, Tanzi F. 2002. Ca uptake by the endoplasmic reticulum Ca -ATPase in rat microvascular endothelial cells. Biochem J 364: 235-244. 2+  2+  Mohan RR, Hutcheon AEK, Choi R, Hong J, Lee J, Mohan RR, Ambrosio R Jr, Zieske JD, Wilson SE. 2003. Apoptosis, necrosis, proliferation, and myofibroblast generation in the stroma following LASIK and PRK. Exp Eye Res 76: 71-87. Moore KL. 1988. The cardiovascular system. In: The Developing Human. Clinically Oriented Embryology, 4/e. Saunders, Philadelphia, 286-333. Mountian 1, Manolopoulos VG, De Smedt H, Parys JB, Missiaen L, Wuytack F. 1999. Expression patterns of sarco/endoplasmic reticulum Ca -ATPase and inositol 1,4,5trisphosphate receptor isoforms in vascular endothelial cells. Cell Calcium 25: 371-380. Mulholland DL, Gotlieb AI. 1996. Cell biology of valvular interstitial cells. Can J Cardiol 12: 231-236. Mulholland DL, Gotlieb AI. 1997. Cardiac valve interstitial cells: regulator of valve structure and function. Cardiovasc Pathol 6: 167-174. Neylon CB, Irvine RF. 1990. Synchronized repetitive spikes in cytoplasmic calcium in confluent monolayers of human umbilical vein endothelial cells. FEBS Lett 275: 173-176. Niisato N , Ogata Y , Furuyama S, Sugiya H. 1996. Histamine H i receptor-induced Ca mobilization and prostaglandin E2 release in human gingival fibroblasts. Biochem Pharmacol 52: 1015-1023. 2+  Nilius B, Droogmans G. 2001. Ion channels and their functional role in vascular endothelium. Physiol Rev 81: 1416-1459. 164  Nishida K, Harrison DG, Navas JP, Fisher AA, Dockery SP, Uematsu M, Nerem RM, Alexander RW, Murphy TJ. 1992. Molecular cloning and characterization of the constitutive bovine aortic endothelial cell nitric oxide synthase. J Clin Invest 90: 2092-2096. Novak I, Falus A. 1997. Molecular biology and role of histamine in physiological and pathological reactions - a review. Acta Biol Hungarica 48: 385-394. Paltauf-Doburzynska J, Frieden M , Graier WF. 1999. Mechanisms of Ca store depletion in single endothelial cells in a Ca -free environment. Cell Calcium 25: 345-353. 2+  2+  Paltauf-Doburzynska J, Posch K, Paltauf G, Graier WF. 1998. Stealth ryanodine-sensitive Ca release contributes to activity of capacitative Ca entry and nitric oxide synthase in bovine endothelial cells. J Physiol 513: 369-379. 2+  2+  Paraskos JA. 2000. Combined valvular disease. In: Valvular Heart Disease, 3/e. Alpert JS, Dalen JE, Rahimtoola SH (eds). Lippincott Williams and Wilkins, New York, 291-337. Philipson KD. 1999. Sodium-calcium exchange. In: Calcium as a Cellular Regulator. Carafoli E, Klee CB (eds). Oxford University Press, New York, 279-294. Post SR, Jacobson JP, Insel PA. 1996. P2 purinergic receptor agonists enhance cAMP production in Madin-Darby canine kidney epithelial cells via an autocrine/paracrine mechanism. JBiol Chem 271: 2029-2032. Quaedvlieg PFHJ, Lamers CBHW, Taal BG. 2002. Carcinoid heart disease: an update. Scand J Gastroenterol 37 Suppl 236: 66-71. Ralevic V, Burnstock G. 1998. Receptors for purines and pyrimidines. Pharmacol Rev 50: 413492. Ramadori G, Saile B. 2002. Mesenchymal cells in the liver - one cell type or two? Liver 22: 283-294. Redfield M M , Nicholson WJ, Edwards WD, Tajik AJ. 1992. Valve disease associated with ergot alkaloid use. Echocardiographic and pathologic correlations. Ann Intern Med 117: 50-52. Roberts WC. 1973. Valvular, subvalvular and supravalvular aortic stenosis: morphologic features. Cardiovasc Clin 5: 97-126. Rosales OR Isales CM, Barrett PQ, Brophy C, Sumpio BE. 1997. Exposure of endothelial cells to cyclic strain induces elevations of cytosolic Ca concentration through mobilization of intracellular and extracellular pools. Biochem J326: 385-392. Rose AG. 1996. Etiology of valvular heart disease. Curr Opin Cardiol 11: 98-113. Saiag B, Bodin P, Shacoori V, Catheline M, Rault B, Burnstock G. 1995. Uptake and flowinduced release of uridine nucleotides from isolated vascular endothelial cells. Endothelium 2: 279-285. Scanlon M , Williams DA, Fay FS. 1987. A Ca -insensitive form of fura-2 associated with polymorphonuclear leukocytes. J Biol Chem 262: 6308-6312. 2+  Sedova M , Blatter LA. 1999. Dynamic regulation of [Ca ]j by plasma membrane Ca -ATPase and Na /Ca exchange during capacitative Ca entry in bovine vascular endothelial cells. Cell Calcium 25: 333-343. 2+  +  2+  2+  2+  165  Segura, A M , Luna RE, Horiba K, Stetler-Stevenson WG, McAllister Jr HA, Willerson JT, Ferrans VJ. 1998. Immunohistochemistry of matrix metalloproteinases and their inhibitors in thoracic aortic aneurysms and aortic valves of patients with Marfan's syndrome. Circulation 98: II331-II338. Setola V, Hufeisen SJ, Grande-Allen KJ, Vesely I, Glennon RA, Blough B, Rothman RB, Roth BL. 2003. 3,4-methylenedioxymethamphetamine (MDMA, "Ecstasy") induces fenfluraminelike proliferative actions on human cardiac valvular interstitial cells in vitro. Mol Pharmacol 63: 1223-1229. Shryock JC, Belardinelli L. 1997. Adenosine and adenosins receptors in the cardiovascular system: biochemistry, physiology, and pharmacology. Am J Cardiol 79: 2-10. Siney L, Lewis MJ. 1993. Nitric oxide release from porcine mitral valves. Cardiovasc Res 27: 1657-1661. Skarsgard PL, Wang X, McDonald P, Lui AH, Lam EK, McManus BM, van Breemen C, Laher I. 2000. Profound inhibition of myogenic tone in rat cardiac allografts is due to eNOS- and iNOSbased nitric oxide and an intrinsic defect in vascular smooth muscle contraction. Circulation 101: 1303-1310. Soler-Soler J, Galve E. 2000. Worldwide perspective of valve disease. Heart 83: 721-725. Stein PD, Wang CH, Riddle JM, Sabbah HN, Magilligan Jr DJ, Hawkins ET. 1989. Scanning electron microscopy of operatively excised severely regurgitant floppy mitral valves. Am J Cardiol 64: 392-394. Stepien O, Zhang Y, Zhu D, Marche P. 2002. Dual mechanism of action of amlodipine in human vascular smooth muscle cells. JHypertens 20: 95-102. Stisapesan R, Williams AJ. 1996. Modification of the conductance and gating properties of ryanodine receptors. JMembr Biol 153: 93-103. Su, X , Wachtel RE, Gebhart GF. 2000. Mechanosensitive potassium channels in rat colon sensory neurons. JNeurophysiol 84: 836-843. Supino PG, Borer JS, Yin A. 2002. The epidemiology of valvular heart disease: an emerging public health problem. Adv Cardiol 39: 1-6. Tamura K, Fukuda Y, Ishizaki M , Masuda Y, YamanakaN, Ferrans VJ. 1995. Abnormalities in elastic fibers and other connective-tissue components of floppy mitral valve. Am Heart J 129: 1149-1158. Taylor PM, Allen SP, Yacoub MH. 2000. Phenotypic and functional characterization of interstitial cells from human heart valves, pericardium and skin. J Heart Valve Dis 9: 150-158. Taylor PM, Batten P, Brand NJ, Thomas PS, Yacoub MH. 2003. The cardiac vale interstitial cell. Intl J Biochem Cell Biol 35: 113-118. Teubl M , Groschner K, Kohlwein SD, Mayer B, Schmidt K. 1999. Na /Ca exchange facilitates Ca -dependent activation of endothelial nitric oxide synthase. J Biol Chem 274: 19529-29535. +  2+  2+  Tran QK, Ohashi K, Watanabe H. 2000. Calcium signaling in endothelial cells. Cardiovasc Res 48: 13-22. 166  Trepakova ES, Gericke M , Hirakawa Y , Weisbrod RM, Cohen RA, Bolotina V M . 2001. Properties of a native cation channel activated by Ca store depletion in vascular smooth muscle cells. JBiol Chem 276: 7782-7790. 2+  Turner DJ, Segura BJ, Cowles RA, Zhang W, Mulholland MW. 2001. Functional overlap of IP3- and cADP-ribose-sensitive calcium stores in guinea pig myenteric neurons. Am J Physiol 281: G208-G215. Twort CH, van Breemen C. 1988. Cyclic guanosine monophosphate-enhanced sequestration of Ca by sarcoplasmic reticulum in vascular smooth muscle. Circ Res 62:961-964. 2+  Ullrich V, Bachschmid M. 2000. Superoxide as a messenger of endothelial function. Biochem Biophys Res Commun 278: 1-8. van Breemen C, Chen Q, Laher 1. 1995. Superficial buffer barrier function of smooth muscle sarcoplasmic reticulum. Trends Pharmacol Sci 16:98-105. Varadi A, Rutter GA. 2002. Dynamic imaging of endoplasmic reticulum Ca concentration in insulin-secreting M1N6 cells using recombinant targeted cameleons: roles of sarco(endo)plasmic reticulum Ca -ATPase (SERCA)-2 and ryanodine receptors. Diabetes 51: S190-S201. 2+  2+  Vassort G. 2001. Adenosine 5'-triphosphate: a P2-purinergic agonist in the myocardium. Physiol Rev 81: 767-806. Verma SC, McNeill JH. 1977. Cardiac histamine receptors: differences between left and right atria and right ventricle. J Pharmacol Exp Ther 200: 352-362. Viana F, De Smedt H, Droogmans G, Nilius B. 1998. Calcium signaling through nucleotide receptor P2Y2 in cultured human vascular endothelium. Cell Calcium 24: 117-127. Villaschi S, Nicosia R. 1993. Angiogenic role of endogenous basic fibroblast growth factor released by rat aorta after injury. Am J Pathol 143: 181-190. Virmani R, Atkinson JB, Forman MB. 1988. The pathology of mitral valve prolapse. Herz 13: 215-226. Wagner AH, Schroeter MR, Hecker M. 2001. 17-beta-estradiol inhibition of NADPH oxidase expression in human endothelial cells. FASEB J'15: 2121-2130. Walter-Yohrling J, Pratt BM, Ledbetter S, Teicher BA. 2003. Myofibroblasts enable invasion of endothelial cells into three-dimensional tumor cell clusters: a novel in vitro tumor model. Cancer Chemother Pharmacol 52: 263-269. Wang X, Chu W, Lau F, van Breemen C. 1995b. Bradykinin potentiates acetylcholine-induced responses in native endothelial cells from rabbit aorta. Biochem Biophys Res Commun 213: 1061-1067. Wang X, Kim SU, van Breemen C, McLarnon JG. 2000. Activation of purinergic P2X receptors inhibits P2Y-mediated Ca influx in human microglia. Cell Calcium 27: 205-212. 2+  Wang X, Lau F, Li L, Yoshikawa A, van Breemen C. 1995. Acetylcholin-sensitive intracellular Ca store in fresh endothelial cells and evidence for ryanodine receptors. Circ Res 11: 37-42. 2+  Wang X, Reznick S, Li P, Liang W, van Breemen C. 2002. Ca removal mechanisms in freshly isolated rabbit aortic endothelial cells. Cell Calcium 31: 265-277'. 2+  167  Wang X , van Breemen C. 1997. Multiple mechanisms of activating C a entry in freshly isolated rabbit aortic endothelial cells. J Vase Res 34: 196-207. /+  Watanabe T, Tagushi Y, Sasaki K, Kitamura Y. 1981. Increase in histidine decarboxylase activity in mouse skin after application of the tumor promoter tetradecanoylphorbol acetate. Biochem Biophys Res Commun 100: 427-432. Weiner CP, Lizasoain I, Baylis Knowles RG, Charles IG, Moncada S. 1994. Induction of calcium-dependent nitric oxide synthases by sex hormones. Proc Natl Acad Sci USA 91: 52125216. Williams M, Jarvis MF. 2000. Purinergic and pyrimidinergic receptors as potential drug targets. Biochem Pharmacol 59: 1173-1185. Wilson PW. 1997. An epidemiologic perspective of systemic hypertension, ischemic heart disease, and heart failure. Am J Cardiol 80: 3J-8J. Wilson SE, Netto M, Ambrosio R. 2003. Corneal cells: chatty in development, homeostasis, wound healing, and disease. Am J Ophthalmol 136: 530-536. Wilson SE, Schultz GS, Chegini N , Weng J, He YG. 1994. Epidermal growth factor, transforming growth factor alpha, transforming growth factor beta, acidic fibroblast growth factor, basic fibroblast growth factor, and interleukin-1 proteins in the cornea. Exp Eye Res 59: 63-72. Xu J, Jian B, Chu R, Lu Z, Li Q, Dunlop J, Rosenzweig-Lipson S, McGonigle P, Levy RJ, Liang B. 2002. Serotonin mechanisms in heart valve disease II. The 5-HT2 receptor and its signaling pathway in aortic valve interstitial cells. Am J Pathol 161: 2209-2218. Yang Z, Zhang A, Altura BT, Altura BM. 1999. Hydrogen peroxide-induced endotheliumdependent relaxation of rat aorta involvement of Ca and other cellular metabolites. Gen Pharmacol 33: 325-336. 2+  Yumoto Y, Horie M , Kubota T, Ninomiya T, Kobori A, Takenaka K, Takano M, Niwano S, Izumi T. 2004. Bepridil block of recombinant human cardiac IKS current shows a timedependent unblock. J Cardiovasc Pharmacol 43: 178-182. Zacks S, Rosenthal A, Granton B, Havenith M, Opas M, Gotlieb AI. 1991. Characterization of cobblestone mitral valve interstitial cells. Arch Pathol Lab Med 115: 774-779. Ziegelstein RC, Spurgeon HA, Pili R, Passaniti A, Cheng L, Corda S, Lakatta EG, Capogrossi MC. 1994. A functional ryanodine-sensitive intracellular Ca store is present in vascular endothelial cells. Circ Res 74: 151-156. 2+  168  


Citation Scheme:


Citations by CSL (citeproc-js)

Usage Statistics



Customize your widget with the following options, then copy and paste the code below into the HTML of your page to embed this item in your website.
                            <div id="ubcOpenCollectionsWidgetDisplay">
                            <script id="ubcOpenCollectionsWidget"
                            async >
IIIF logo Our image viewer uses the IIIF 2.0 standard. To load this item in other compatible viewers, use this url:


Related Items