Search tips
Search criteria 


Logo of emmExperimental and Molecular MedicineArchiveAbout the journalGuide to authors
Exp Mol Med. 2017 June; 49(6): e341.
Published online 2017 June 2. doi:  10.1038/emm.2017.68
PMCID: PMC5519013

Protein tyrosine phosphatase 1B is a mediator of cyclic ADP ribose-induced Ca2+ signaling in ventricular myocytes


Cyclic ADP-ribose (cADPR) releases Ca2+ from ryanodine receptor (RyR)-sensitive calcium pools in various cell types. In cardiac myocytes, the physiological levels of cADPR transiently increase the amplitude and frequency of Ca2+ (that is, a rapid increase and decrease of calcium within one second) during the cardiac action potential. In this study, we demonstrated that cADPR levels higher than physiological levels induce a slow and gradual increase in the resting intracellular Ca2+ ([Ca2+]i) level over 10 min by inhibiting the sarcoendoplasmic reticulum Ca2+ ATPase (SERCA). Higher cADPR levels mediate the tyrosine-dephosphorylation of α-actin by protein tyrosine phosphatase 1B (PTP1B) present in the endoplasmic reticulum. The tyrosine dephosphorylation of α-actin dissociates phospholamban, the key regulator of SERCA, from α-actin and results in SERCA inhibition. The disruption of the integrity of α-actin by cytochalasin B and the inhibition of α-actin tyrosine dephosphorylation by a PTP1B inhibitor block cADPR-mediated Ca2+ increase. Our results suggest that levels of cADPR that are relatively higher than normal physiological levels modify calcium homeostasis through the dephosphorylation of α-actin by PTB1B and the subsequent inhibition of SERCA in cardiac myocytes.


Ca2+ plays a fundamental role in the cardiac contraction and relaxation cycle by linking the electrical depolarization of cardiomyocytes with contraction (that is, excitation–contraction coupling; EC coupling).1 Cellular depolarization after the action potential is generated from the sinoatrial node activates voltage-operated Ca2+ channels, which causes an influx of Ca2+ across the sarcolemma and into the cytoplasm.1 The resulting Ca2+ influx activates ryanodine receptors (RyRs) on the sarcoplasmic reticulum (SR), which causes more Ca2+ to be released into the cytosol—this phenomenon is known as Ca2+-induced Ca2+ release (CICR).2, 3, 4 A transient increase in the free cytosolic calcium concentration ([Ca2+]i), Ca2+ transient in cardiac myocytes allows the actin and myosin contractile filaments to engage and slide past each other, resulting in cardiac muscle contraction.4 Sarcoendoplasmic reticulum Ca2+ ATPase (SERCA) in sarcoplasmic reticulum (SR) in cardiac myocytes transfers Ca2+ from the cytosol to the lumen of the SR as a result of ATP hydrolysis during muscle relaxation.5 The transfer of Ca2+ by SERCA from the cytosol to the SR is inhibited by unphosphorylated phospholamban (PLB).6 PLB phosphorylation can relieve the inhibition of the SERCA pump and enhance [Ca2+]i.6

Cyclic ADP-ribose (cADPR) is synthesized from NAD+ by bifunctional ectoenzymes including CD38 and CD157, and monofunctional ADP ribosyl cyclase from the Aplysia mollusc.7, 8, 9 In cardiac myocytes, nanomolar cADPR concentrations increase the amplitude and frequency of Ca2+ transient through an increased accumulation of Ca2+ in the SR and the subsequent luminal Ca2+-dependent activation of RyRs.10 In this study, we investigated the mechanism by which micromolar cADPR concentrations affect [Ca2+]i in cardiac myocytes.

Materials and methods


The reagents 3-(3,5-dibromo-4-hydroxy-benzoyl)-2-ethyl-benzofuran-6-sulfonic acid-(4-(thiazol-2-ylsulfamyl)-phenyl)-amide a PTP inhibitor; 8-hydroxy-7-(6-sulfonaphthalen-2-yl)diazenyl-quinoline-5-sulfonic acid, an SHP1/2 PTPase inhibitor; and sodium stibogluconate were from Calbiochem (San Diego, CA, USA). Fura 2 AM and Fura 2 lowaff were obtained from Invitrogen (Carlsbad, CA, USA) and TEFLabs (Austin, TX, USA), respectively.

Preparation of cardiac myocytes

This study was approved by the institutional review committee of Chonbuk National University (Reference Number: CBU 2008-0057). New Zealand white rabbits (1.8–2.4 kg) were anesthetized with an intramuscular injection of 50 mg kg−1 ketamine and 20 mg kg−1 xylazine hydrochloride. The hearts were removed after deep anesthesia was confirmed by the disappearance of the corneal reflex and the withdrawal of the hindlimb resulting from clamping of the paw. Cardiac myocytes were enzymatically isolated from the ventricle as previously described11 and superfused at 34−36 °C with a solution containing (mM) 8.5 NaCl, 14.5 NaHCO3, 4.2 KCl, 1.18 MgSO4·7H2O, 2.5 CaCl2 and 11.1 glucose (oxygenated at 95% O2, 5% CO2).

Fluorimetric determination of [Ca2+]i

Rabbit ventricular myocytes were loaded with fura 2-AM (5 μM) through a 60-min incubation. After they were washed, the cells were seeded in a 200-μl well with a glass coverslip on the bottom and incubated on the stage of an inverted fluorescence microscope (Nikon, Tokyo, Japan) that was continuously perfused at 37 °C. The fluorescence was measured at a determined site through a pinhole with alternating excitation wavelengths of 340 and 380 nm and an emission wavelength of 510 nm using a Ca2+ microspectrofluorometer (PTI). At the end of each recording, the data were calibrated in terms of [Ca2+]i as described by Grynkyewicz et al. based on equation (a)12 and normalized to calculate the % increase of [Ca2+]i (b)6, 13, 14, 15 A Kd value of 229 nM was assumed for the binding of Ca2+ to fura 2-AM. Rmax, Rmin, Sf2 and Sb2 were measured in each experimental cell by the addition of 20 mM CaCl2 (Rmax) and 50 mM EGTA (Rmin).

equation image
equation image

At the beginning of each experiment, the cells were washed in a Ca2+-free solution containing (mM) 135 NaCl, 5.4 KCl, 1 MgCl2, 10 glucose, and 5 HEPES. Patch-pipettes were pulled from borosilicate glass capillary tubules by a micropipette puller (PP-83, Narishige Co. Ltd, Tokyo, Japan) and fire-polished. The patch-pipette tip resistance was between 4–6 MΩ. The intracellular solution for filling each patch pipette contained 110 mM KCl, 5 mM K2ATP, 10 mM HEPES (pH 7.2 with KOH). After attachment to the myocytes, the resistance was monitored beginning when the giga seal formation (Axon AxoScope 10). cADPR (100 μM) or IP3 (100 nM) was applied to the cytosol by rupturing the plasma membrane with a patch-pipette containing each reagent. The reagents 8-Bromo cADPR (Br-cADPR), ryanodine, caffeine, dantrolene, xestospongin, tetracaine, the PTP1B inhibitor, the SHP1/2 PTPase inhibitor or sodium stibogluconate were applied to the bath. Thapsigargin was also applied to the cytosol with a patch pipette.

Immunoprecipitation and immunoblotting

The isolated ventricular myocytes were lysed in lysis buffer containing (in mM) 150 NaCl, 20 HEPES, 1 EDTA, and 0.1 PMSF, as well as 1% Triton X-100 (in μg ml−1), at pH 7.2, and the lysates were centrifuged at 13,000 g for 10 min. The proteins were then immunoprecipitated with rabbit IgG (Sigma), mouse anti-SERCA (Affinity BioReagents), mouse anti-α-actin (Sigma) or mouse anti-PLB antibodies (Affinity BioReagents) (1:100 dilution). The immune complexes were subsequently collected by adding protein A or G beads (1/10 volume, Sigma), fractionated by 10% SDS-PAGE, and transferred to polyvinylidene difluoride membranes. The blots were incubated with anti-phosphotyrosine (Santa Cruz Biotechnology, Inc., Dallas, TX, USA), anti-α-actin, anti-PLB antibodies, anti-phospho-Ser,16 or anti-phospho-Thr17 PLB antibodies (Badrilla, Leeds, UK) and subsequently incubated with goat anti-mouse or anti-rabbit alkaline phosphatase-conjugated secondary antibodies (Santa Cruz Biotechnology). The proteins were visualized using an enhanced chemiluminescence system (Intron, Seongnam, Republic of Korea) and an LAS 3000 imaging system (Fuji, Tokyo, Japan). To detect the total or tyrosine-phosphorylated α-actin in SR vesicles, we removed the IgG heavy chain band using ImmunoCruzTM IP/WB Optima E (Santa Cruz Biotechnology, Inc.) according to the manufacturer’s instructions.

Fluorimetric measurement of SR Ca2+ uptake

Rabbit SR vesicles (0.5 mg per 1 ml cuvette) were pre-incubated for 1 min at room temperature in the SR Ca2+ uptake solution containing (mM) 50 KCl, 20 MOPS, 0.01 CaCl2, 5 NaN3, 1 KH2PO4, 5 creatine phosphate, and 10 U creatine phosphokinase. Rabbit SR vesicles (0.5 mg per 1 ml cuvette) suspended in a cuvette were mixed with 1 μM Fura-2 lowAff. The Fura 2 fluorescence outside of the vesicles was monitored over time with alternating excitation wavelengths of 340 and 380 nm and an emission wavelength of 510 nm, using a Ca2+ microspectrofluorometer (PTI). The extravesicular Ca2+ concentration was expressed as a fluorescence excitation ratio (R340nm/380nm).

Identification of proteins

The dried samples were analyzed by matrix-assisted laser desorption/ionization-time-of flight (MALDI-TOF) mass spectrometry (Voyager-DE PRO) for peptide mass fingerprinting and by electrospray ionization quadrupole time of flight (ESI-Q-TOF) mass spectrometry for peptide sequencing. Database searches were carried out using MS-Fit, accessed via the World Wide Web at

Measurement of ATPase activity in intact SR vesicles

The ATPase activity in the SR vesicles was determined using an ATPase assay kit (Innova Biosciences, Cambridge, UK) according to the manufacturer’s instructions with minor modifications. Briefly, SR vesicles (0.1 μg) in a total volume of 100 μl were incubated for 10 min in the presence of various concentrations of cADPR (0–40 μM) with or without a 10 min pretreatment with various inhibitors. The mixture was incubated for 1 min at 37 °C in substrate buffer (0.5 M Tris-HCl, 0.1 M MgCl2, 10 mM purified ATP, 5 μM calcein-AM, 5 mM sodium azide, and 1 mM ouabain, pH 7.4) with or without Na-orthovanadate (2–20 μM). After incubation, the reaction was stopped by the addition of 50 μl of Gold Mix from the ATPase assay kit. Two minutes later, 20 μl of stabilizer from the ATPase assay kit was added, and the solution was incubated for 20 min at 37 °C in the dark. The enzyme activity was calculated by measuring the Pi-dye complex released via ATP hydrolysis using an ELISA plate reader at 635 nm (Molecular Devices, Sunnyvale, CA, USA).

Statistical analysis

Values are expressed as the mean±s.e.m. Significant differences were determined by Student’s t-test; P<0.05 was considered significant.


cADPR induces an increase in the resting intracellular Ca2+ concentration ([Ca2+]i) in isolated rabbit ventricular myocytes independently of ryanodine- and IP3-sensitive pools

To investigate the effect of higher cADPR levels on resting [Ca2+]i, we intracellularly applied cADPR at micromolar levels in the cytosol through a patch pipette in rabbit ventricular myocytes and monitored resting [Ca2+]i. Intracellular cADPR application increased resting [Ca2+]i slowly in a concentration-dependent manner, reaching a maximum at 100 μM cADPR (Figure 1a). When the cells were pretreated with 10 μM 8-Br-cADPR (a competitive cADPR antagonist) for 10 min, the intracellular cADPR application had no effect on the resting [Ca2+]i (Figure 1b), indicating that cell dialysis by patch pipette itself did not change the [Ca2+]i. Pretreatment with xestospongin C (2 μM), an IP3 antagonist, did not affect cADPR-induced increase in resting [Ca2+]i (Figure 1b). Pretreatment with ryanodine, a RyR blocker, and tetracaine, a RyR2 inhibitor, blocked caffeine-induced but not cADPR-induced increase in resting [Ca2+]i (Figures 1c and e). These results indicate that cADPR-induced an increase in resting [Ca2+] in cardiac myocytes that did not involve RyRs and IP3 receptors.

Figure 1
cADPR induces an increase in resting [Ca2+]i in isolated rabbit ventricular myocytes independent of ryanodine- and IP3-sensitive pools. (a) The effect of intracellular cADPR application on resting [Ca2+]i in isolated rabbit ventricular myocytes. cADPR ...

To prevent the perturbation of Ca2+ signaling by Fura 2-mediated Ca2+ buffering and the effect of Ca2+ influx by calcium channels in the plasma membrane, we investigated whether cADPR induces a Ca2+ release from isolated SR vesicles using Fura-2 lowAff, a low affinity calcium chelator. The addition of ATP rapidly decreased extravesicular [Ca2+] (Figures 2a and b) due to Ca2+ chelation followed by Ca2+ uptake into SR vesicles via an SR Ca2+ pump and then the maintenance of a steady state of [Ca2+]. When 100 μM cADPR or 10 mM caffeine was added after the steady state in the absence or presence of 10 μM tetracaine, an increase in [Ca2+] outside the vesicles was seen (Figures 2a and b). Tetracaine pretreatment blocked caffeine- but not cADPR-induced increase in extravesicular [Ca2+] (Figures 2a and b). These results support the hypothesis that cADPR-induced increase in resting [Ca2+]i in cardiac myocytes did not involve RyRs.

Figure 2
Effect of tetracaine on cADPR- and caffeine-induced Ca2+ release from isolated SR vesicles. (a, b) Rabbit SR vesicles (0.5 mg per 1 ml cuvette) suspended in a cuvette were mixed with 1 μM Fura-2 lowAff. The Fura 2 fluorescence ...

cADPR induces α-actin tyrosine dephosphorylation and its dissociation from PLB

PLB regulates SERCA via a physical interaction.18 Dephosphorylated PLB inhibits SERCA activity, whereas phosphorylation of PLB by cAMP-dependent protein kinase (PKA) relieves the inhibitory effect on SERCA.19 PLB is regulated via phosphorylation/dephosphorylation of Ser16 and Thr17 by PKA, a Ca2+/calmodulin-dependent protein kinase and protein phosphatases.16, 17, 20, 21, 22 It has been reported that cADPR increases SERCA activity in Xenopus oocytes.10, 23 However, we found that cADPR inhibits SR ATPase activity in a concentration-dependent manner, which is completely blocked by 8-Br-cADPR pretreatment (Figure 3a). To determine whether cADPR-induced increase in resting [Ca2+]i involves phosphorylation including PLB phosphorylation, we investigated the effect of phosphatase inhibitors. Okadaic acid (OA), a serine phosphatase inhibitor, had no effect on cADPR-induced increase in resting [Ca2+]i. In contrast, phenylarsine oxide (PAO), a tyrosine phosphatase inhibitor, blocked cADPR-induced increase in resting [Ca2+]i (Figure 3b). However, cADPR and PAO had no effect on phosphorylation of Ser16 residue of PLB (Figure 3c). These data suggest that tyrosine phosphorylation rather than serine/threonine phosphorylation, such as that which characterizes PLB phosphorylation, is required for cADPR-mediated calcium signaling.

Figure 3
cADPR dissociates α-actin from PLB by tyrosine dephosphorylation and mediates an increase in resting [Ca2+]i. (a) Effect of cADPR on ATPase activity in rabbit SR vesicles. ATPase in intact SR vesicles was assayed as described in Materials and ...

We identified a 42-kDa tyrosine-phosphorylated protein associated with PLB using an immunoprecipitation assay. cADPR dissociated the protein with PLB, which was blocked by 8-Br-cADPR pretreatment (Figure 3d). MALDI-TOF and ESI-Q-TOF mass spectrometry revealed that the 42-kDa protein was α-actin. cADPR decreased the association of α-actin with PLB by approximately half, which was blocked by PAO pretreatment (Figure 3e). These results indicate that cADPR activates a protein tyrosine phosphatase that dephosphorylates tyrosine residues on α-actin and dissociates α-actin from PLB.

We further investigated the effect of other specific inhibitors of tyrosine phosphatase on cADPR-induced increase in resting [Ca2+]i in isolated rabbit ventricular myocytes and in extravesicular [Ca2+] in SR vesicles (Figures 4a and b). The pharmacological inhibition of PTP1B but not SHP1/2 blocked cADPR-induced increase in resting [Ca2+]i in ventricular myocytes and extravesicular [Ca2+] in SR vesicles. cADPR-mediated decrease of α-actin association with PLB was abolished by PTP1B but not by SHP1/2 inhibition (Figure 4c). These results suggest that α-actin tyrosine dephosphorylation by PTP1B is required for cADPR-induced increase in resting [Ca2+]i in cardiac myocytes.

Figure 4
Effects of a PTP1B inhibitor, an SHP1/2 inhibitor and stibogluconate on cADPR-induced increase in resting [Ca2+]i in isolated rabbit ventricular myocytes (a) and isolated SR vesicles (b). (a) Fura 2- AM loaded myocytes were incubated with 8 μ ...

α-actin integrity is required for cADPR-induced increase in resting [Ca2+]i in isolated rabbit ventricular myocytes

Our results clearly showed that the dissociation of α-actin from PLB plays a critical role in cADPR-induced increase in resting [Ca2+]i. To determine whether the physical interaction between α-actin and PLB was related to cADPR-induced increase in resting [Ca2+]i, we investigated the effect of cytochalasin B, a disruptor of F-actin, on cADPR-induced increase in resting [Ca2+]i. Pretreatment of the cells with cytochalasin B completely blocked cADPR-induced increase in resting [Ca2+]i (Figure 5a), without affecting IP3- or caffeine-induced increase in resting [Ca2+]i (Figures 5b and c). These results suggest that a physical interaction between α-actin and PLB is required for cADPR-induced increase in resting [Ca2+]i.

Figure 5
Effects of cytochalasin B on cADPR-, IP3- or caffeine-induced increases in resting [Ca2+]i in isolated rabbit ventricular myocytes. cADPR (100 μM) (a) and IP3 (100 nM) (b) were dialyzed via a patch pipette. The arrowheads indicate ...

cADPR-induced inhibition of SERCA is dependent on α-actin integrity and PTP1B activity in isolated rabbit ventricular myocytes

We next investigated the effect of thapsigargin, an SERCA inhibitor, on cADPR-induced increase in resting [Ca2+]i. Direct application of thapsigargin in the cytosol via a patch pipette slowly increased resting [Ca2+]i in a manner similar to that of cADPR, although the effect of thapsigargin was much more potent and slightly more rapid than that of cADPR (Figure 6a). However, the combined application of thapsigargin and cADPR in the cytosol did not have an additive effect on increase in resting [Ca2+]i (Figures 6a and b). Additionally, thapsigargin pretreatment blocked cADPR-induced increase in resting [Ca2+]i (Figure 6c). cADPR inhibited SERCA activity in isolated cardiac SR vesicles in a dose-dependent manner that was blocked by 8-Br-cADPR pretreatment (Figure 3a). cADPR-mediated inhibition of SERCA activity was blocked by α-actin disruption and PTP1B inhibition (Figure 6d). These results suggest that cADPR induces an increase in resting [Ca2+]i by SERCA inhibition via PTP1B -mediated α-actin dephosphorylation.

Figure 6
cADPR induces an increase in resting [Ca2+]i by inhibiting α-actin integrity-dependent SERCA and PTP1B activity. (a) The effects of intracellular cADPR, thapsigargin (Tsg), and both on [Ca2+]i. cADPR (100 μM) (left), Tsg (1 μ ...


Previous studies have reported that cADPR is a specific agonist of RyR channels and induces Ca2+ release by sensitizing the RyR to cytosolic Ca2+.24, 25, 26, 27, 28, 29, 30, 31, 32, 33 Lukyanenko et al.10 reported that cADPR activates SERCA and potentiates a Ca2+ release in saponin-permeabilized rat ventricular myocytes. However, we demonstrated that cADPR inhibits SERCA in intact rabbit ventricular myocytes. This discrepancy may be due to experimental conditions such as the manner in which nucleotides such as ATP are included in the reaction. The report showed that cADPR activates SERCA by monitoring SR Ca2+ uptake in the presence of rheutenium red and ATP. Different from that result, we showed that cADPR inhibits SERCA under conditions closer to the actual physiological conditions in the absence of rheutenium red.

Ca2+ transient is a transient increase of calcium in the cell that peaks and gradually decreases during the cardiac action potential. Ca2+ transient is exclusively dependent on Ca2+ influx through L-type calcium channels. Excitation-contraction (EC) coupling in cardiac myocytes is mediated by a mechanism known as calcium-induced calcium release (CICR) where Ca2+ entry via L-type calcium channels induces calcium release from ryanodine-sensitive Ca2+ stores.34, 35 In cardiomyocytes, a cytosolic injection of 8-amino-cADPR reduces Ca2+ transient and contractions, indicating that cADPR increases EC coupling.29 In addition, photoreleased cADPR induces an increase in the magnitude and frequency of whole cell Ca2+ transient. In this study, we focused on the effect of cADPR on resting [Ca2+]i but not Ca2+ transient. We investigated the effect of cADPR on resting [Ca2+]i at higher concentrations than physiological level. We observed that relatively high concentrations of cADPR inhibit rather than activate SERCA activity, resulting in an increase in resting [Ca2+]i in cardiac myocytes. The endogenous level of cADPR in the heart is 1.04–150 pmol mg−1, which corresponds to 30 nM–4.5 μM depending on experimental conditions.36, 37 Hypoxia increases cADPR concentration by twofold in the second-order branches of the pulmonary artery and by 10-fold in the third order branches.38 These results suggest that cADPR level could increase up to approximately 50 μM during specific pathological states in the heart. It has been known that myocardial ischemia, a hypoxic condition induced by blood flow restriction, increases Ca2+ concentration in cardiomyocytes, and it is associated with abnormal cardiac function.13 Cardiac ADPR cyclase, a protein distinct from CD38 or the archetypical ADPR cyclase from A. californica, has not been cloned to date.39 To verify the direct relationships between higher level of cADPR and ischemic injury, the identification of cardiac ADPR cyclase is necessary. The present study suggests that high levels of cADPR under pathophysiological conditions might decrease SR load and inhibit CICR, resulting in the inhibition of excitation-contraction (EC) coupling in cardiac myocytes.

Our results show that α-actin is involved in cADPR- but not IP3- or caffeine-induced increase of [Ca2+]i. The disruption of α-actin blocked cADPR- but not IP3- or caffeine-induced increases in resting [Ca2+]i, suggesting that α-actin integrity is required for cADPR action. Interestingly, α-actin was associated with PLB, and their association was decreased by cADPR treatment. The cADPR-mediated dissociation was inhibited by PTP1B inhibition. Our results suggest that cADPR activates PTP1B, which causes tyrosine dephosphorylation of α-actin.

Interestingly, although cADPR and IP3 act on the same calcium stores, only cADPR-mediated calcium response was sensitive to the disruption of α-actin integrity. IP3 mediates calcium release by direct action on IP3 receptor in SR vesicles, whereas cADPR mediates it indirectly via PTP1B, possibly resulting in the sensitivity difference to α-actin disruption.


This work was supported by the Basic Science Research Program through the National Research Foundation of Korea (NRF) funded by the Ministry of Science, ICT and future Planning (2014R1A2A1A10054634 and 2012M3A9B4028749)


The authors declare no conflict of interest.


  • Bers DM. Cardiac excitation-contraction coupling. Nature 2002; 415: 198–205. [PubMed]
  • Fill M, Copello JA. Ryanodine receptor calcium release channels. Physiol Rev 2002; 82: 893–922. [PubMed]
  • Meissner G. Molecular regulation of cardiac ryanodine receptor ion channel. Cell Calcium 2004; 35: 621–628. [PubMed]
  • Roderick HL, Berridge MJ, Bootman MD. Calcium-induced calcium release. Curr Biol 2003; 13: R425. [PubMed]
  • Eisner DA, Sipido KR. Sodium calcium exchange in the heart: necessity or luxury? Circ Res 2004; 95: 549–551. [PubMed]
  • James P, Inui M, Tada M, Chiesi M, Carafoli E. Nature and site of phospholamban regulation of the Ca2+ pump of sarcoplasmic reticulum. Nature 1989; 342: 90–92. [PubMed]
  • Guse AH. Biochemistry, biology, and pharmacology of cyclic adenosine diphosphoribose. Curr Med Chem 2004; 11: 847–855. [PubMed]
  • Liu Q, Kriksunov IA, Graeff R, Munshi C, Lee HC, Hao Q. Crystal structure of human CD38 extracellular domain. Structure 2005; 13: 1331–1339. [PubMed]
  • Prasad GS, McRee DE, Stura EA, Levitt DG, Lee HC, Stout CD. Crystal structure of aplysia ADP ribosyl cyclase, a homologue of the bifunctional ectozyme CD38. Nat Struct Biol 1996; 3: 957–964. [PubMed]
  • Lukyanenko V, Gyorke I, Wiesner TF, Gyorke S. Potentiation of Ca2+ release by cADP-ribose in the heart is mediated by enhanced SR Ca2+ uptake into the sarcoplasmic reticulum. Circ Res 2001; 89: 614–622. [PubMed]
  • Mitra R, Morad M. A uniform enzymatic method for dissociation of myocytes from hearts and stomachs of vertebrates. Am J Physiol 1985; 249: H1056–H1060. [PubMed]
  • Grynkiewicz G, Poenie M, Tsien RY. A new generation of Ca2+ indicators with greatly improved fluorescence properties. J Biol Chem 1985; 260: 3440–3450. [PubMed]
  • Kalogeris T, Baines CP, Krenz M, Korthuis RJ. Cell biology of ischemia/reperfusion injury. Int Rev Cell Mol Biol 2012; 298: 229–317. [PMC free article] [PubMed]
  • Patel JM, Li YD, Zhang J, Gelband CH, Raizada MK, Block ER. Increased expression of calreticulin is linked to ANG IV-mediated activation of lung endothelial NOS. Am J Physiol 1999; 277: L794–L801. [PubMed]
  • Viola HM, Arthur PG, Hool LC. Transient exposure to hydrogen peroxide causes an increase in mitochondria-derived superoxide as a result of sustained alteration in L-type Ca2+ channel function in the absence of apoptosis in ventricular myocytes. Circ Res 2007; 100: 1036–1044. [PubMed]
  • Kranias EG. Regulation of Ca2+ transport by cyclic 3′,5′-AMP-dependent and calcium-calmodulin-dependent phosphorylation of cardiac sarcoplasmic reticulum. Biochim Biophys Acta 1985; 844: 193–199. [PubMed]
  • Kranias EG, Di Salvo J. A phospholamban protein phosphatase activity associated with cardiac sarcoplasmic reticulum. J Biol Chem 1986; 261: 10029–10032. [PubMed]
  • Simmerman HK, Jones LR. Phospholamban: protein structure, mechanism of action, and role in cardiac function. Physiol Rev 1998; 78: 921–947. [PubMed]
  • Kim HW, Steenaart NA, Ferguson DG, Kranias EG. Functional reconstitution of the cardiac sarcoplasmic reticulum Ca2(+)-ATPase with phospholamban in phospholipid vesicles. J Biol Chem 1990; 265: 1702–1709. [PubMed]
  • Davis BA, Schwartz A, Samaha FJ, Kranias EG. Regulation of cardiac sarcoplasmic reticulum calcium transport by calcium-calmodulin-dependent phosphorylation. J Biol Chem 1983; 258: 13587–13591. [PubMed]
  • Kranias EG, Steenaart NA, Di Salvo J. Purification and characterization of phospholamban phosphatase from cardiac muscle. J Biol Chem 1988; 263: 15681–15687. [PubMed]
  • Le Peuch CJ, Haiech J, Demaille JG. Concerted regulation of cardiac sarcoplasmic reticulum calcium transport by cyclic adenosine monophosphate dependent and calcium—calmodulin-dependent phosphorylations. Biochemistry 1979; 18: 5150–5157. [PubMed]
  • Yamasaki-Mann M, Demuro A, Parker I. cADPR stimulates SERCA activity in Xenopus oocytes. Cell Calcium 2009; 45: 293–299. [PMC free article] [PubMed]
  • Cui Y, Galione A, Terrar DA. Effects of photoreleased cADP-ribose on calcium transients and calcium sparks in myocytes isolated from guinea-pig and rat ventricle. Biochem J 1999; 342: Pt 2 269–273. [PubMed]
  • Dargie PJ, Agre MC, Lee HC. Comparison of Ca2+ mobilizing activities of cyclic ADP-ribose and inositol trisphosphate. Cell Regul 1990; 1: 279–290. [PMC free article] [PubMed]
  • Galione A, Lee HC, Busa WB. Ca(2+-induced Ca2+ release in sea urchin egg homogenates: modulation by cyclic ADP-ribose. Science 1991; 253: 1143–1146. [PubMed]
  • Lee HC. Potentiation of calcium- and caffeine-induced calcium release by cyclic ADP-ribose. J Biol Chem 1993; 268: 293–299. [PubMed]
  • Lee HC, Aarhus R, Graeff R, Gurnack ME, Walseth TF. Cyclic ADP ribose activation of the ryanodine receptor is mediated by calmodulin. Nature 1994; 370: 307–309. [PubMed]
  • Rakovic S, Galione A, Ashamu GA, Potter BV, Terrar DA. A specific cyclic ADP-ribose antagonist inhibits cardiac excitation-contraction coupling. Curr Biol 1996; 6: 989–996. [PubMed]
  • Tanaka Y, Tashjian AH Jr. Calmodulin is a selective mediator of Ca2+-induced Ca2+ release via the ryanodine receptor-like Ca2+ channel triggered by cyclic ADP-ribose. Proc Natl Acad Sci USA 1995; 92: 3244–3248. [PubMed]
  • Thomas JM, Masgrau R, Churchill GC, Galione A. Pharmacological characterization of the putative cADP-ribose receptor. Biochem J 2001; 359: 451–457. [PubMed]
  • Walseth TF, Lee HC. Synthesis and characterization of antagonists of cyclic-ADP-ribose-induced Ca2+ release. Biochim Biophys Acta 1993; 1178: 235–242. [PubMed]
  • Wang YX, Zheng YM, Mei QB, Wang QS, Collier ML, Fleischer S et al. FKBP12.6 and cADPR regulation of Ca2+ release in smooth muscle cells. Am J Physiol Cell Physiol 2004; 286: C538–C546. [PubMed]
  • Gyorke I, Gyorke S. Regulation of the cardiac ryanodine receptor channel by luminal Ca2+ involves luminal Ca2+ sensing sites. Biophys J 1998; 75: 2801–2810. [PubMed]
  • Han S, Schiefer A, Isenberg G. Ca2+ load of guinea-pig ventricular myocytes determines efficacy of brief Ca2+ currents as trigger for Ca2+ release. J Physiol 1994; 480: Pt 3 411–421. [PubMed]
  • Walseth TF, Aarhus R, Zeleznikar RJ Jr, Lee HC. Determination of endogenous levels of cyclic ADP-ribose in rat tissues. Biochim Biophys Acta 1991; 1094: 113–120. [PubMed]
  • Young GS, Choleris E, Lund FE, Kirkland JB. Decreased cADPR and increased NAD+ in the Cd38-/- mouse. Biochem Biophys Res Commun 2006; 346: 188–192. [PubMed]
  • Wilson HL, Dipp M, Thomas JM, Lad C, Galione A, Evans AM. Adp-ribosyl cyclase and cyclic ADP-ribose hydrolase act as a redox sensor. a primary role for cyclic ADP-ribose in hypoxic pulmonary vasoconstriction. J Biol Chem 2001; 276: 11180–11188. [PubMed]
  • Gul R, Kim SY, Park KH, Kim BJ, Kim SJ, Im MJ et al. A novel signaling pathway of ADP-ribosyl cyclase activation by angiotensin II in adult rat cardiomyocytes. Am J Physiol 2008; 295: H77–H88. [PubMed]

Articles from Experimental & Molecular Medicine are provided here courtesy of Korean Society for Biochemistry and Molecular Biology