Cellular Biology
Multifunctional Mitochondrial Epac1 Controls
Myocardial Cell Death
Loubina Fazal,* Marion Laudette,* Sílvia Paula-Gomes, Sandrine Pons, Caroline Conte,
Florence Tortosa, Pierre Sicard, Yannis Sainte-Marie, Malik Bisserier, Olivier Lairez,
Alexandre Lucas, Jérôme Roy, Bijan Ghaleh, Jérémy Fauconnier, Jeanne Mialet-Perez,
Frank Lezoualc’h
Rationale: Although the second messenger cyclic AMP (cAMP) is physiologically beneficial in the heart, it largely
Downloaded from http://ahajournals.org by on May 24, 2020
contributes to cardiac disease progression when dysregulated. Current evidence suggests that cAMP is produced
within mitochondria. However, mitochondrial cAMP signaling and its involvement in cardiac pathophysiology are
far from being understood.
Objective: To investigate the role of MitEpac1 (mitochondrial exchange protein directly activated by cAMP 1) in
ischemia/reperfusion injury.
Methods and Results: We show that Epac1 (exchange protein directly activated by cAMP 1) genetic ablation
(Epac1−/−) protects against experimental myocardial ischemia/reperfusion injury with reduced infarct size and
cardiomyocyte apoptosis. As observed in vivo, Epac1 inhibition prevents hypoxia/reoxygenation–induced adult
cardiomyocyte apoptosis. Interestingly, a deleted form of Epac1 in its mitochondrial-targeting sequence protects
against hypoxia/reoxygenation–induced cell death. Mechanistically, Epac1 favors Ca2+ exchange between
the endoplasmic reticulum and the mitochondrion, by increasing interaction with a macromolecular complex
composed of the VDAC1 (voltage-dependent anion channel 1), the GRP75 (chaperone glucose-regulated protein
75), and the IP3R1 (inositol-1,4,5-triphosphate receptor 1), leading to mitochondrial Ca2+ overload and opening
of the mitochondrial permeability transition pore. In addition, our findings demonstrate that MitEpac1 inhibits
isocitrate dehydrogenase 2 via the mitochondrial recruitment of CaMKII (Ca2+/calmodulin-dependent protein
kinase II), which decreases nicotinamide adenine dinucleotide phosphate hydrogen synthesis, thereby, reducing
the antioxidant capabilities of the cardiomyocyte.
Conclusions: Our results reveal the existence, within mitochondria, of different cAMP–Epac1 microdomains that
control myocardial cell death. In addition, our findings suggest Epac1 as a promising target for the treatment of
ischemia-induced myocardial damage. (Circ Res. 2017;120:645-657. DOI: 10.1161/CIRCRESAHA.116.309859.)
Key Words: calcium
■
cyclic AMP
■
ischemia reperfusion injury
C
yclic AMP (cAMP) is a ubiquitous second messenger
that controls numerous physiological processes, including metabolism, Ca2+ homeostasis, and gene transcription. While most studies focused on the biological effects
of cytosolic cAMP, its possible role in mitochondrial function and pathophysiology has been neglected until recently.
Today, an increasing body of evidence strongly suggests
that cAMP is also produced in the mitochondrion.1,2 There,
cAMP is generated in the mitochondrial matrix by the type
■
mitochondria
■
reactive oxygen species
10 soluble adenylyl cyclase (sAC), which is activated in response to HCO3– or Ca2+ ions.1,3,4 It has been proposed that
cAMP produced by sAC activates a pool of the cAMP effector
PKA (protein kinase A) present in the mitochondrial matrix,
resulting in the phosphorylation of the cytochrome c oxidase
subunit IV isoform 1, which consequently enhances oxidative phosphorylation and, hence, ATP synthesis.1,3 Besides
ATP production, the mitochondria play a crucial role in other
important cellular processes, such as Ca2+ buffering, reactive
Original received August 26, 2016; revision received January 11, 2017; accepted January 16, 2017. In December 2016, the average time from submission
to first decision for all original research papers submitted to Circulation Research was 13.4 days.
From the Inserm, UMR-1048, Institut des Maladies Métaboliques et Cardiovasculaires, Toulouse, France (L.F., M.L., S.P.-G., C.C., F.T., P.S., Y.S.-M.,
M.B., O.L., A.L., J.M.-P., F.L.); Université de Toulouse, France (L.F., M.L., S.P.-G., C.C., F.T., P.S., Y.S.-M., M.B., O.L., A.L., J.M.-P., F.L.); Inserm,
U955, Equipe 03, F-94000, Créteil, France (S.P., B.G.), and Inserm, UMR-1046 (J.R., J.F.); and UMR CNRS-9214, PHYMEDEX, Université de
Montpellier, France (J.R., J.F.).
*These authors contributed equally to this article.
The online-only Data Supplement is available with this article at http://circres.ahajournals.org/lookup/suppl/doi:10.1161/CIRCRESAHA.
116.309859/-/DC1.
Correspondence to Frank Lezoualc’h, Inserm, UMR-1048, Institut des Maladies Métaboliques et Cardiovasculaires 1 avenue Jean Pouhlès, 31432
Toulouse Cedex 4, France. E-mail Frank.Lezoualch@inserm.fr
© 2017 American Heart Association, Inc.
Circulation Research is available at http://circres.ahajournals.org
DOI: 10.1161/CIRCRESAHA.116.309859
645
646 Circulation Research February 17, 2017
Novelty and Significance
What Is Known?
• The second messenger cAMP is produced in the cytosol and mitochondria of cardiomyocytes.
• Dysregulation of cAMP signaling contributes to cardiac remodeling and
heart failure.
• Epac1 (exchange protein directly activated by cAMP 1) induces cardiomyocyte hypertrophy in response to β-adrenergic receptor stimulation.
What New Information Does This Article Contribute?
• Epac1 gene deletion is cardioprotective against ischemia/reperfusion
injury in vivo.
• Epac1 is activated by soluble adenylyl cyclase during hypoxia/reoxygenation to transduce cardiomyocyte death.
• Under hypoxia, the activation of mitochondrial Epac1 increases mitochondrial Ca2+ overload and reduces reactive oxygen species detoxification, thereby, inducing cardiomyocyte death.
Nonstandard Abbreviations and Acronyms
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8-CPT-AM
BRET
CaMKII
cAMP
GRP75
Epac1
ER
HX+R
IDH2
IP3R1
I/R
MCU
MitEpac1
MPTP
NADPH
NX
PKA
ROS
sAC
VDAC1
WT
8-pCPT-2′-O-Me-cAMP-AM
bioluminescence resonance energy transfer
Ca2+/calmodulin-dependent protein kinase II
cyclic adenosine monophosphate
chaperone glucose-regulated protein 75
exchange protein directly activated by cAMP 1
endoplasmic reticulum
hypoxia/reoxygenation
isocitrate dehydrogenase 2
inositol-1,4,5-triphosphate receptor 1
ischemia/reperfusion
mitochondrial Ca2+ uniporter
mitochondrial Epac1
mitochondrial permeability transition pore
nicotinamide adenine dinucleotide phosphate
normoxia
protein kinase A
reactive oxygen species
soluble adenylyl cyclase
voltage-dependent anion channel 1
wild-type
oxygen species (ROS) production, and apoptosis.2 This is well
illustrated in the context of myocardial ischemia/reperfusion
(I/R), a clinical relevant form of myocardial injury in which
mitochondrial Ca2+ overload and an excessive production of
ROS trigger the opening of the mitochondrial permeability
transition pore (MPTP), resulting in mitochondrial depolarization and cardiomyocyte death.5
In the heart, cAMP regulates many physiological processes, such as contractility, relaxation, and automaticity,
and represents the strongest mechanism for increasing cardiac function in response to β-adrenergic receptor activation.6 However, the sustained release of catecholamines from
adrenergic nerves observed during myocardial ischemia
cAMP is a ubiquitous second messenger, and its possible role in
mitochondrial function and pathophysiology has yet to be investigated. Here we show that genetic inhibition of the cAMP-binding
protein, Epac1, is cardioprotective against myocardial ischemia/
reperfusion injury. Mechanistically, Epac1 is activated by soluble
adenylyl cyclase and promotes cardiomyocyte death during hypoxia/reoxygenation. Furthermore, we found that mitochondrial
Epac1 regulated different aspects of mitochondrial function,
such as Ca2+ uptake, reactive oxygen species production, and
mitochondrial permeability transition pore opening. Thus, the
development of Epac1 pharmacological inhibitors may represent
a promising therapeutic avenue for the treatment of ischemia/
reperfusion injury.
overactivates myocardial β-adrenergic receptor and subsequent cAMP production that is believed to further accelerate
ischemia-induced cell damage.7,8 Therefore, cAMP production that is physiologically beneficial in the heart largely
contributes to cardiac disease progression when dysregulated.6 Because cardiomyocyte death is one of the hallmarks
of myocardial I/R injury,9 many efforts have been made to
understand the signaling events involving cAMP to this process. Most studies that have demonstrated the effect of cAMP
signaling on cell death have primarily focused on PKA.8,10,11
However, cAMP also stimulates a family of proteins directly activated by cAMP, named Epac (exchange proteins directly activated by cAMP12,13). The Epac proteins, Epac1 and
Epac2, are guanine exchange factors for the small G-proteins
Rap1 and Rap2 and function in a PKA-independent manner. Compelling evidence indicate that Epac proteins induce
sarcoplasmic reticulum Ca2+ leakage14,15 and localize at the
nuclear envelope of cardiomyocytes to promote cardiac remodeling.16–18 However, Epac compartmentalization is still
poorly described, and its involvement in cardiomyocyte death
has yet to be investigated.
In this study, we showed that Epac1 genetic ablation
(Epac1−/−) protected against experimental myocardial I/R injury with reduced infarct size and cardiomyocyte apoptosis.
Mechanistic studies allowed us to propose a model, whereby
I/R stimulated cAMP production by sAC, which in turn activated MitEpac1 (mitochondrial Epac1), leading to mitochondrial Ca2+ overload, a decrease in ATP production, a decrease
in ROS detoxification, and eventually apoptosis. These data
also suggest that the inhibition of Epac1 could reduce myocardial damage during cardiac ischemia.
Methods
Animals
All animal procedures were performed in accordance with
Institutional Guidelines on Animal Experimentation and with a
French Ministry of Agriculture license. Moreover, this investigation conformed to the Guide for the Care and Use of Laboratory
Fazal et al Role of Epac1 in Ischemia/Reperfusion Injury 647
Animals published by the Directive 2010/63/EU of the European
Parliament. Mice were housed in a pathogen-free facility, and all
animal experiments were approved by the Animal Care and Use
Committees of the University of Toulouse. Epac1-deficient mice
(Epac1−/−) have been engineered in our laboratory as previously
described.17 Eight-week-old male Epac1−/− mice and littermate controls (wild-type [WT]) in this study were obtained by heterozygous
crossing.
Plasmid Constructs and Transfection
The Epac1–bioluminescence resonance energy transfer (BRET)
sensor CAMYEL was constructed from the pQE30-CAMYEL prokaryotic expression vector (a gift from Dr L.I. Jiang) as previously
described.19 The human Epac1 expression vector was a gift from Dr
J.L. Bos. Primary neonatal rat cardiomyocytes were transfected using Lipofectamine 2000 (Invitrogen) according to the manufacturer’s
instructions.
BRET Assay
Neonatal rat cardiomyocytes transfected with the Epac1-BRET sensor CAMYEL were harvested and lysed in a buffer containing 40
mmol/L HEPES, pH 7.2, 140 mmol/L KCl, 10 mmol/L NaCl, 1.5
mmol/L MgCl2, 0.5% Triton X-100, and a cocktail of protease inhibitors (Roche Applied Science). BRET experiments were performed as
previously described.19 Emission from Renilla luciferase and citrine
were measured simultaneously in a plate reader (TECAN infinite
F200).
Statistical Analysis
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Analyses were performed using Prism 7 (GraphPad Software).
Results are expressed as mean±SEM or fold increase, as appropriate. Genotype–treatment interactions were studied by using
2-way analysis of variance. Multiple comparisons were performed
with 1-way analysis of variance followed by post hoc test with
Bonferroni correction or Tukey posttest. Statistical significance
was set to P<0.05.
Results
Epac1 Deficiency Is Cardioprotective Against
I/R Injury
We first analyzed cardiac Epac1 expression in ischemic failing human heart samples and in mice subjected to myocardial
I/R injury. In both human and mouse hearts, Epac1 protein
levels were markedly increased compared with that in control hearts (Figure 1A and 1B), suggesting that Epac1 upregulation is associated with myocardial ischemic damage. To
test this hypothesis, Epac1−/− mice and their WT littermates
were subjected to myocardial I/R injury. Although the area
at risk was similar in both genotype (Figure 1C), the infarct
size-to-area at risk ratio was significantly reduced in Epac1−/−
(33±4%) when compared with that in WT (53±4%; Figure 1C
and 1D). Consistently, cardiomyocyte apoptosis, assayed by
TUNEL (terminal deoxynucleotidyl transferase dUTP nickend labeling) staining, was markedly reduced in Epac1−/− mice
compared with that in WT mice (Figure 1E), whereas it was
similar in both genotypes at baseline (Online Figure I).
Accordingly, in WT animals, I/R injury was accompanied by an upregulation of the proapoptotic protein Bax, a
downregulation of the antiapoptotic protein Bcl2 (Online
Figure II), an increase in cytochrome c level, and caspase 9
and caspase 3 activation (Figure 1F through 1H). In marked
contrast, this I/R-induced apoptotic response was partially inhibited by the genetic ablation of Epac1 (Figure 1F
through 1H; Online Figure II). Altogether, these results
suggest Epac1 as a transducer of cardiomyocyte apoptosis
after myocardial I/R injury.
Epac1 Is Activated by Soluble Adenylyl Cyclase
During Hypoxia/Reoxygenation to Transduce
Cardiomyocyte Death
To test whether Epac1 may directly influence cell death, we
next subjected isolated cardiomyocytes from adult Epac1−/−
and WT mice to either normoxia (NX) or 4-hour hypoxia
followed by 2-hour reoxygenation (HX+R), which mimics
in vivo I/R. Under HX+R, WT cardiomyocytes exhibited an
increase in membrane permeability assayed by LDH (lactate dehydrogenase) release (Figures 2B), a decrease in cell
viability assayed by trypan blue exclusion and cellular ATP
level (Figures 2A; Online Figure III), and the expression of
I/R-associated apoptotic markers (Online Figure IV). As observed in vivo, Epac1 deletion prevented HX+R-induced cell
damages (Figure 2A and 2B; Online Figure III). These data
confirmed HX+R in isolated cardiomyocytes as an in vitro
surrogate to in vivo myocardial I/R injury.
Next, to test the activation of Epac1 during HX+R, neonatal cardiomyocytes were transfected with an Epac1 BRET
sensor to monitor Epac1 activation.19 HX+R induced a significant increase in the BRET ratio when compared with NX,
which was blocked by a selective Epac1 inhibitor, CE3F419
(Figure 2C), confirming Epac1 activation during HX+R.
Furthermore, CE3F4 prevented HX+R-induced cell damage
phenocopying Epac1 deletion (Figure 2D), and the membrane-permeant Epac1-specific agonist, 8-pCPT-2′-O-MecAMP-AM (8-CPT-AM),20 mimicked the effects of HX+R in
WT cardiomyocytes cultured in NX conditions (Figure 2E).
Of note, 8-CPT-AM did not induce any HX+R-associated cell
damages in Epac1−/− cardiomyocytes, confirming the specificity of the agonist (Figure 2E). These data indicate that Epac1
activation is sufficient to provoke cardiomyocyte cell death in
HX+R conditions.
During HX+R, we observed that WT cardiomyocytes accumulated cAMP, the cognate activator of Epac1 (Figure 2F).
Because sAC was recently shown to produce cAMP in hypoxic condition,21 we investigated its possible involvement
in HX+R-mediated Epac1 activation. The selective sAC inhibitor, KH7, blocked cAMP accumulation and significantly
reduced HX+R-induced Epac1 activation in WT cardiomyocytes (Figure 2C and 2F), as well as HX+R-induced cell damages, similarly to CE3F4 (Figure 2D).19 Taken together, these
results provide strong evidence that Epac1 is activated by
cAMP produced by sAC and directly promotes cardiomyocyte
death under HX+R conditions.
MitEpac1 Promotes Cardiomyocyte Death
The protein sequence of Epac1 contains a predicted mitochondrial-targeting domain (Figure 3A). Cell fractionation followed by Western blot analysis showed that Epac1
is localized both in the cytosol and in the mitochondria
(Figure 3B). To assess the specific localization of Epac1,
we performed subfractionation of mitochondria (free of endoplasmic reticulum [ER]) in WT hearts (Figure 3C). The
purity of the fractions was verified by immunoblotting with
specific protein markers, such as monoamine oxidase-A for
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Figure 1. Epac1 deficiency is cardioprotective against ischemia/reperfusion (I/R) injury. A and B, Quantification of Epac1 protein
in human left ventricular myocardium from nonischemic control (CTL; n=4) or patients with ischemic cardiomyopathy (ICM; n=5), and
in wild-type (WT) or Epac1−/− heart mice subjected or not to I/R (n=6 per group). Representative immunoblots are shown. GAPDH
(glyceraldehyde-3-phosphate dehydrogenase), loading control. C, Quantification of the area at risk (AAR) expressed as percentage of
left ventricle size and infarct size expressed as percentage of AAR. D, A representative cross-section stained with Evans blue and TTC of
WT and Epac1−/− heart mice subjected to I/R. E, Representative images of TUNEL (terminal deoxynucleotidyl transferase dUTP nick-end
labeling) staining of heart sections from WT and Epac1−/− mice subjected to I/R. DAPI, nuclear marker; α-actinin, cardiomyocyte marker.
Arrows indicate positive TUNEL nuclei. Scale bar, 50 μm. Right, Quantification of TUNEL-positive staining (n=500 in 6 independent
experiments). F-H, Quantification of the indicated proteins (n=6 in each condition). Representative immunoblots are shown. Data are
means±SEM and were analyzed with 2-way analysis of variance (ANOVA)/Bonferroni posttest. *P<0.05, **P<0.01, ***P<0.001 vs the
indicated value. Epac1 indicates exchange protein directly activated by cAMP 1.
mitochondrial outer-membrane and intermembrane space,
cytochrome c oxidase subunit 4 for inner membrane, and
isocitrate dehydrogenase (IDH2) for the matrix, respectively. We found that Epac1 was expressed in the mitochondrial
inner membrane and matrix (Figure 3C). Since the mitochondrion plays a critical role in the regulation of apoptosis,
we further investigated whether MitEpac1 plays a role in
HX+R-induced cell death.
To this end, we constructed a mutant form of Epac1 deleted for its putative mitochondrial-targeting sequence (Epac1∆2–
37
; Figure 3A). Transfection experiments followed by cell
fractionation and immunoblot analysis showed that Epac1∆2–37
was mainly excluded from the mitochondrial compartment
of cardiomyocytes (Figure 3D through 3E). Epac1∆2–37 mutant activated Epac1 downstream effector Rap1 in a similar
fashion as the WT protein (Epac1WT), indicating that loss of
mitochondrial targeting did not impair Epac1 function in the
cytosol (Figure 3F). Importantly, cardiomyocytes transfected
with Epac1∆2–37 exhibited less cell death as compared with cardiomyocytes transfected with the Epac1WT when subjected to
HX+R (Figure 3G). Together, these data strongly suggest that
MitEpac1 participates in cardiomyocyte death during hypoxic
stress.
Epac1 Promotes Mitochondrial Ca2+ Overload
Via the Dependent Anion Channel 1/Chaperone
Glucose-Regulated Protein 75/Inositol-1,4,5Triphosphate Receptor 1 Complex and MPTP
Opening During HX+R
It is well accepted that I/R injury is accompanied by an increase in mitochondrial Ca2+ that triggers the opening of
MPTP, the subsequent depolarization of the mitochondrial
membrane potential (ΔΨm), leading to cytochrome c release
and cardiomyocyte death.22 However, the mechanisms that
control mitochondrial Ca2+ entry in that context are far to be
understood. We, therefore, addressed whether Epac1 would
play a role in such a process using a Ca2+ fluorescent probe
Fazal et al Role of Epac1 in Ischemia/Reperfusion Injury 649
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Figure 2. Epac1 is activated by soluble adenylyl cyclase (sAC) to promote cardiomyocyte death during hypoxia/reoxygenation
(HX+R). A and B, Cell viability determined by trypan blue staining and measurement of lactate dehydrogenase (LDH) release in isolated
adult WT or Epac1−/− cardiomyocytes in normoxia (NX) or HX+R condition (n=6). Representative images of trypan blue staining are
shown. Scale bar, 100 μm. C, Analysis of Epac1 activity by bioluminescence resonance energy transfer (BRET) in neonatal rat ventricular
myocytes transfected with the CAMYEL construct and pretreated with either CE3F4 (20 μmol/L, 1 hour) or KH7 (20 μmol/L, 1 hour) before
to be placed in NX or HX+R condition (n=10). D, LDH release in adult wild-type (WT) cardiomyocytes in NX or HX+R condition (n=6–8).
Cells were pretreated with either CE3F4 or KH7 as in (C). E, LDH release in WT or Epac1−/− cardiomyocytes (n=6–8). Cells were pretreated
or not with CE3F4 (20 μmol/L, 30 minutes) and stimulated with 8-CPT-AM (10 μmol/L, 30 minutes). F, Quantification of intracellular cAMP
in adult WT cardiomyocytes in NX or HX+R condition (n=7). Cells were pretreated or not with KH7 (20 μmol/L, 30 minutes). Data are
means±SEM and were evaluated by 1-way analysis of variance (ANOVA)/Bonferroni posttest. *P<0.05, **P<0.01, ***P<0.001, ****P<0.0001
vs control group or the indicated value. Epac1 indicates exchange protein directly activated by cAMP 1.
Rhod-2-AM.23 Although the disadvantage of Rhod-2-AM is
its nonratiometric nature, the specific accumulation of this
probe in mitochondria makes it one of the most widely used
mitochondrial Ca2+ probe.24 The Rhod-2-AM signal overlapped with the mitochondrial marker Mitotracker green in
adult cardiomyocytes (Online Figure V). 8-CPT-AM induced
a robust increase in mitochondrial Ca2+ in WT cardiomyocytes but not in those of Epac1−/− cells (Figure 4A; Online
Figure V). Furthermore, treatment of Epac1−/− cardiomyocytes with 50 μmol/L of Ca2+ induced much less mitochondrial Ca2+ overload when compared with the WT (Figure 4B;
Online Figure VI), suggesting that mitochondrial Ca2+ level
increased in cardiomyocytes after Epac1 stimulation. Yet, we
found that the mitochondrial Ca2+ uniporter (MCU) was involved in Epac1 effect because the MCU inhibitor, RU360,
significantly reduced 8-CPT-AM-induced mitochondrial Ca2+
(Online Figure VIIA).
To determine how Epac1 influenced mitochondrial Ca2+
uptake, we next analyzed its interaction with a macromolecular complex composed of the VDAC1 (voltage-dependent
anion channel 1), the GRP75 (chaperone glucose-regulated
protein 75), and the IP3R1 (inositol-1,4,5-triphosphate receptor 1). This Ca2+-handling protein complex of the ER (IP3R1)
and the mitochondrion (VDAC1) is highly concentrated at
mitochondria-associated ER membranes, where it regulates
Ca2+ exchange between the ER and the mitochondria.25
Immunoprecipitation assay with Epac1 antibody showed
that 8-CPT-AM increased VDAC1/GRP75/IP3R1 complex
formation, indicating that activated Epac1 favors the association of this complex (Online Figure VIII). We did not observe
any interaction of Epac1 with the RyR2 (type 2 ryanodine
receptor), a dominant sarcoplasmic reticulum Ca2+ channels
protein. This suggests that the Epac1 interaction with the
VDAC1/GRP75/IP3R1 complex is specific (Online Figure
VIII). In addition, size exclusion chromatography followed
by Western blot showed that VDAC1, GRP75, IP3R1, and
Epac1 were eluted and detected in the same high molecular
weight fraction (Online Figure IX). Altogether, these data indicate that all 4 proteins belonged to the same macromolecular complex.
Next, we investigated whether such an effect of Epac1
on VDAC1/GRP75/IP3R1 complex formation would also
occur in hypoxic condition. As expected, we observed by
in situ proximity ligation assay that HX+R significantly increased IP3R1/GRP75, IP3R1/VDAC1, and GRP75/VDAC1
interactions in WT cardiomyocytes (Figure 4C through 4E).
The absence of Epac1 did not modify VDAC1/GRP75/IP3R1
interaction in NX condition. However, in HX+R condition,
the lack of Epac1 reduced VDAC1/GRP75/IP3R1 interaction compared with that in WT cardiomyocytes (Figure 4C
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Figure 3. MitEpac1 promotes cardiomyocyte death. A, Schematic representation of the different domains of Epac1WT. Epac1Δ2–37
mutant bears a deletion in Epac1 mitochondrial-targeting sequence. B, Representative immunoblot of cytosolic (CYTO) and mitochondrial
(MT) Epac1 expression in cardiac samples of WT or Epac1−/− mice. GAPDH (glyceraldehyde-3-phosphate dehydrogenase) and voltagedependent anion channel 1 (VDAC1) expression were used as loading control of cytosolic and mitochondrial fractions, respectively. C,
Localization of Epac1 in the inner membrane and matrix of mouse cardiac mitochondria. Monoamine oxidase-A (MAO-A), cytochrome c
oxidase (subunit 4 [COX4]) and IDH2 (isocitrate dehydrogenase) are markers for mitochondrial outer-membrane (OM) and intermembrane
space (IMS), inner membrane (IM) and matrix, respectively. Calnexin, endoplasmic reticulum (ER) marker. D, Mitochondrial Epac1/VDAC1
to cytosolic Epac1/tubulin expression ratio in neonatal rat ventricular myocytes transfected with the indicated plasmids (n=4). Tubulin and
VDAC1 expression were used as loading control of cytosolic and mitochondrial fractions, respectively. Representative immunoblots are
shown. E, Immunofluorescence staining of HA-Epac1WT and HA-Epac1Δ2–37 transfected in primary cardiomyocytes. Epac1 was visualized
with an anti-HA. DAPI and Mitotracker stains mark the position of nuclei and mitochondria, respectively. Scale bar, 10 µm. F, Amounts
of Rap1-GTP (n=3 in each group) in primary cardiomyocytes transfected with the indicated plasmids. Cells were stimulated or not with
8-CPT-AM (10 μmol/L, 10 minutes). Representative immunoblots are shown. G, Cell viability of primary cardiomyocytes transfected with
the indicated plasmids (n=8). Data are means±SEM and were evaluated by 1-way analysis of variance (ANOVA)/Bonferroni or Tukey
posttest. *P<0.05, ***P<0.001, ****P<0.0001 vs control group or the indicated value. Epac1 indicates exchange protein directly activated
by cAMP 1; HA, human influenza hemagglutinin; and MitEpac, mitochondrial exchange protein directly activated by cAMP 1.
through 4E). Altogether, these results suggest that Epac1 is
involved in mitochondrial Ca2+ overload by increasing the
interaction with the VDAC1/GRP75/IP3R1 complex, hence,
promoting Ca2+ transfer from the ER to the mitochondria. Our
finding that Epac1 activation enhanced the effect of histamine
on mitochondrial Ca2+ uptake further support this conclusion
(Figure 4F; Online Figure X). Indeed, histamine is known to
stimulate IP3R-mediated Ca2+ transfer from ER to mitochondria.26 Figure 4F through 4G and Online Figure X showed that
8-CPT-AM potentiated the effect of histamine on mitochondrial Ca2+ uptake in WT cardiomyocytes. This Ca2+ transfer
was significantly reduced in the presence of CE3F4 (Figure
4F). Consistently, an IP3R-specific inhibitor, xestospongin
C, also reduced Epac1-induced mitochondrial Ca2+ signal in
WT cardiomyocytes (Online Figure VIIB). These data provide
evidence that Epac1 activation facilitates ER to mitochondrial
Ca2+ transfer.
Because mitochondrial Ca2+ overload promotes MPTP
opening and subsequently triggers cell death, we next investigated the role of Epac1 on MPTP opening in mitochondria isolated from the heart of WT or Epac1−/− mice. MPTP
opening was determined in response to supraphysiological mitochondrial Ca2+ increase as previously described.27
Although 8-CPT-AM potentiated Ca2+-induced MPTP
opening in WT mitochondria, isolated mitochondria from
Epac1−/− mice were resistant to Ca2+-induced MPTP opening (Figure 5A). Using the calcein acetoxymethyl ester
loading/CoCl2 quenching technique to visualize the open/
closed status of MPTP, we observed that the lack of Epac1
delayed MPTP opening in HX+R conditions compared with
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Figure 4. Epac1 increases
mitochondrial Ca2+ uptake via the
VDAC1/GRP75/IP3R1 Ca2+ handling
protein complex. A, Mitochondrial Ca2+
accumulation in adult wild-type (WT)
or Epac1−/− cardiomyocytes stimulated
or not with 8-CPT-AM (10 μmol/L).
Representative traces of the averaged
values of mitochondrial Ca2+ accumulation
(measured as ΔF/F0, where F is the Rhod2-AM fluorescence signal at 270 s, and F0
is the signal at time 0; n=6 in each group).
B, Epac1 deletion prevents mitochondrial
Ca2+ uptake. Experiments were performed
in WT or Epac1−/− cardiomyocytes, which
were incubated with 50 μmol/L external
Ca2+. Averaged values of mitochondrial
Ca2+ accumulation measured as ∆F/F0,
where F is the Rhod-2 fluorescence
signal at 270 s, and F0 is the signal at
time 0 of 50 μmol/L Ca2+ addition (n=6
each experiment). C–E, Typical images
of in situ interactions (red fluorescent
dot) between IP3R1 and GRP75 or
VDAC1 and GRP75 with VDAC1 in WT
or Epac1−/− cardiomyocytes in normoxia
(NX) or hypoxia/reoxygenation (HX+R)
conditions. Nuclei were stained in blue
with DAPI. Scale bar, 20 μm. Graphs
show the quantification of the proximity
ligation assay. Data are means±SEM of 4
independent experiments, and statistical
analysis was performed by a 2-way
analysis of varinace (ANOVA) with a
Bonferroni posttest. **P<0.01, ***P<0.001
vs control group or the indicated value.
F and G, Representative traces of
mitochondrial Ca2+ accumulation in WT
(F) or Epac1−/− (G) cardiomyocytes treated
or not with 8-CPT-AM (10 μmol/L) or
CE3F4 (20 μmol/L) and challenged with
histamine (100 μmol/L). Epac1 indicates
exchange protein directly activated by
cAMP 1; GRP75, glucose-regulated
protein 75; IP3R1, inositol-1,4,5triphosphate receptor 1; and VDAC1,
voltage-dependent anion channel 1.
NX in WT cardiomyocytes (Figures 5B). In addition, JC1 staining and Western blot analysis revealed that 8-CPTAM or HX+R led to depolarization of ΔΨm (Figure 5C)
and increased cytochrome c release (Online Figure XI) in
WT cardiomyocytes but not in Epac1−/− cardiomyocytes or
CE3F4-treated WT cells, highlighting the ability of Epac1
to promote MPTP opening. It is worth mentioning that
cells cotreated with 8-CPT-AM and NIM-811 (Figure 5C),
a nonimmunosuppressive-specific inhibitor of cyclophilin
D that also interacts with the VDAC1/GRP75/IP3R1 complex,26 had similar effect as CE3F4. Altogether, these results
strongly suggest MPTP as a major downstream effector in
the Epac1 cardiac cell death signaling cascade.
MitEpac1 Negatively Regulates IDH2 Activity
Through a CaMKII-Dependent Pathway
Besides Ca2+, ROS play an important role in I/R injury, so we
examined the effects of Epac1 genetic ablation in this process.
Dihydroethidium fluorescence staining showed that I/Rinduced ROS generation was decreased in the heart of Epac1−/−
mice after I/R when compared with WT animals (Figure 6A).
As the mitochondrial generation of ROS is considered the
principal mechanism that initiates cellular oxidative stress in
I/R injury,28 we then tested whether Epac1 was involved in mitochondrial ROS accumulation. 8-CPT-AM treatment of WT
cardiomyocytes provoked an increase in ROS content assayed
using the superoxide-sensitive probe MitoSOX Red; superoxide production remained low and similar to NX condition in
cells devoid of Epac1 treated with 8-CPT-AM or in WT cardiomyocytes treated with 8-CPT-AM and CE3F4 (Figure 6B).
To elucidate the molecular mechanisms whereby Epac1
influenced the redox state of cardiomyocytes, we performed
a phosphoproteomic analysis using 2-dimensional electrophoresis/ProQ Diamond staining coupled to reverse-phase
liquid chromatography and tandem mass spectrometry.
Using this approach, we identified several phosphopeptides
652 Circulation Research February 17, 2017
Figure 5. MitEpac1 induces mitochondrial permeability transition pore (MPTP) opening during hypoxia/reoxygenation (HX+R).
A, Determination of mitochondrial swelling induced by 50 μmol/L Ca2+ in wild-type (WT) or Epac1−/− cardiomyocytes treated or not
with 10 μmol/L 8-pCPT-2′-O-Me-cAMP-AM (8-CPT-AM; n=6). Right, Representative immunoblot showing that the mitochondrial
fractions used for mitochondrial swelling are free of endoplasmic reticulum (ER). GAPDH (glyceraldehyde-3-phosphate dehydrogenase),
voltage-dependent anion channel 1 (VDAC1), and calnexin expression are markers for the cytosol, mitochondria, and ER, respectively.
B, Representative images of mitochondrial green fluorescence of calcein and its quantification in WT or Epac1−/− cardiomyocytes in
normoxia (NX) or hypoxia/reoxygenation (HX+R) condition (n=6–8 for each group). DAPI, nuclear marker (blue). Scale bar, 20 μm. C,
Quantification of fluorescence of JC-1. Representative images of JC-1 staining in WT or Epac1−/− cardiomyocytes pretreated with CE3F4
(20 μmol/L, 30 minutes) or NIM-811 (5 μmol/L, 30 minutes) and stimulated with 8-CPT-AM (10 μmol/L, 30 minutes; n=6) are shown. Red
fluorescence indicates hyperpolarized (aggregate) mitochondria; green fluorescence indicates depolarized (monomer) mitochondria.
DAPI, nuclear marker (blue). Scale bar, 20 μm. Data are means±SEM and were analyzed by 1-way analysis of variance (ANOVA)/
Bonferroni posttest. *P<0.05, **P<0.01, ****P<0.0001 vs control group or the indicated value. Epac1 indicates exchange protein directly
activated by cAMP 1.
Downloaded from http://ahajournals.org by on May 24, 2020
that were differentially represented in WT cardiomyocytes
stimulated or not with 8-CPT-AM (Figure 6C), among which
was spot 155, which corresponded to the IDH2 (isoelectric
point 8.88, molecular weight 50,90 kDa). IDH2 is an enzyme located in the mitochondrial matrix that is mainly and
abundantly expressed in the heart. IDH2 plays a key role in
the cellular defense against oxidative damage by supplying
nicotinamide adenine dinucleotide phosphate (NADPH29) to
regenerate 2 major antioxidant molecules that are the mitochondrial glutathione and thioredoxin.30 In line with the
phosphoproteome data, coimmunoprecipitation experiments
showed that Epac1 activation increased IDH2 serine-specific
phosphorylation that leads to the decrease in IDH2 activity
(Figure 6D). As expected, IDH2 activity was significantly
decreased in the mitochondria isolated from the hearts of
WT mice and treated with 8-CPT-AM or placed in HX+R
condition (Figure 6E). In contrast, Epac1 inhibition or genetic ablation prevented the decrease in mitochondrial IDH2
activity and the subsequent decline in NADPH production
(Figure 6E and 6F). Furthermore, there was no decrease in
IDH2 activity in cardiomyocytes transfected with Epac1∆2–37
compared with those transfected with Epac1WT, suggesting
that MitEpac1 was selectively involved in the regulation of
IDH2 phosphorylation, hence, activity (Figure 6G). Finally,
IDH2 knockdown decreased cell viability compared with
siRNA control in HX+R conditions (Online Figure XIIB,
bar 5 compared with bar 7). 8-CPT-AM failed to potentiate
the effect of IDH2 knockdown compared with siRNA control in HX+R conditions, indicating that Epac1-induced cell
death involved IDH2 inhibition (Online Figure XIIB, bar 6
compared with bar 8). Taken together, these data suggest that
MitEpac1 regulates the phosphorylation of IDH2 and, therefore, decreases the ability of the mitochondria to counteract
the increase in ROS production during HX+R.
Because Epac1 is not a phosphotransferase, we next
sought to identify the missing link between Epac1 and IDH2
phosphorylation. CaMKII (Ca2+/calmodulin-dependent protein kinase II) is a key downstream effector of Epac1 and
is localized both in the cytosol and in the mitochondria.31
Surprisingly, Epac1 deletion specifically decreased mitochondrial CaMKII protein level while having no effect on
the total amount of CaMKII protein (Figure 7A and 7B).
Consistent with previous findings showing that ≈10% of
CaMKII is localized to mitochondria,32 we did not observe
any significant increase in cytosolic CaMKII expression in
Epac1−/− cardiomyocytes compared with WT (Figure 7C).
Similar to the results obtained in Epac1−/− cells, transfection
of Epac1∆2–37 in WT cardiomyocytes specifically reduced
mitochondrial CaMKII protein level (Figure 7D and 7E).
Furthermore, coimmunoprecipitation experiments showed
that Epac1, CaMKII, and IDH2 were involved in the same
macromolecular complex (Figure 7F). Consistently, the
CaMKII inhibitor KN93 prevented Epac1-mediated IDH2
phosphorylation (Figure 6D) and decrease in activity in
the mitochondria isolated from the hearts of WT mice and
treated with 8-CPT-AM but had no effect in Epac1−/− mitochondria (Figure 7G). As expected, this effect also translated
on NADPH content (Figure 7H). Interestingly, bioinformatic
Fazal et al Role of Epac1 in Ischemia/Reperfusion Injury 653
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Figure 6. MitEpac1 (mitochondrial exchange protein directly activated by cAMP 1) phosphorylates isocitrate dehydrogenase
2 (IDH2) and negatively regulates its activity. A, Representative images of dihydroethidium (DHE) fluorescence staining of heart
cryosections from WT and Epac1−/− mice subjected or not to ischemia/reperfusion (I/R). Scale bar, 20 μm. Quantification of DHE
fluorescence staining (n=4). B, Representative images of MitoSOX red fluorescence staining and its quantification (n=6) in wild-type
(WT) or Epac1−/− cardiomyocytes pretreated or not with CE3F4 (20 μmol/L, 30 minutes) and stimulated or not with 8-pCPT-2′-O-MecAMP-AM (8-CPT-AM; 10 μmol/L, 30 minutes). DAPI (blue), nuclear marker. Scale bar, 20 μm. C, ProQ Diamond and EZ Coomassie
Blue staining of a representative 2D gel of cardiomyocyte protein extracts. A representative enlargement of the gel showing the
marked region is illustrated. The ratio of volume value is indicated in the table. The change in the intensity of the protein spot (155)
is indicated as increased (up) in the stimulated 8-CPT-AM (10 μmol/L, 10 minutes) vs control (CT). D, Representative immunoblots of
3 independent experiments showing IDH2 phosphorylation at Ser, Tyr, and Thr residues. Cardiomyocytes were preincubated or not
with either CE3F4 (20 μmol/L, 30 minutes) or KN-93 (5 μmol/L, 30 minutes) and were stimulated or not with 8-CPT-AM (10 μmol/L, 30
minutes) before immunoprecipitation (IP) experiments against IDH2. IgG and GAPDH (glyceraldehyde-3-phosphate dehydrogenase)
were used as control for IP. Input is a control of cell lysates. E, IDH2 activity; and F, NADPH/NADP ratio in isolated mitochondria from
WT and Epac1−/− mice hearts. Mitochondria were either pretreated or not with CE3F4 (20 μmol/L, 30 minutes) and stimulated or not
with 8-CPT-AM (10 μmol/L, 30 minutes), or incubated 30 minutes in hypoxia (HX) followed by 15 minutes of reoxygenation (HX+R;
n=7). G, Determination of IDH2 activity in cardiomyocytes transfected with the indicated plasmids. Cells were preincubated or not
(VEHICLE) with CE3F4 (20 μmol/L, 30 minutes) and stimulated with 8-CPT-AM (10 μmol/L, 30 minutes) (n=6). Data are means±SEM
and were evaluated by 2-way analysis of variance (ANOVA)/Bonferroni posttest. *P<0.05, **P<0.01, ***P<0.001, ****P<0.0001 vs control
group or the indicated value. Epac1 indicates exchange protein directly activated by cAMP 1; ID, identity; and NADPH, nicotinamide
adenine dinucleotide phosphate hydrogen.
analysis of IDH2 sequence led us to identify a potential
phosphorylation site for CaMKIIδ isoform (analysis with
Group-based Prediction System v3.0), which is present in
the mitochondrial matrix of cardiomyocytes (Online Figure
XIII). Knock down of CaMKIIδ with specific siRNA (SiCaMKIIδ) prevented 8-CPT-AM-induced IDH2 phosphorylation, suggesting that this CaMKIIδ isoform specifically targets
IDH2 (Online Figure XIV). Altogether, these data strongly
suggest that MitEpac1 is involved in the mitochondrial localization of CaMKII, which phosphorylates IDH2 when Epac1
is activated and, therefore, leaves the cells vulnerable to oxidative damage during HX+R and I/R injury (Figure 8).
Discussion
In this work, we provided new insights into understanding the
role and compartmentalization of cAMP and Epac1. The novel
contributions include the following: (1) Epac1 was upregulated
in human ischemic failing hearts, and its genetic deletion significantly reduced infarct size in the setting of I/R injury, providing the first direct evidence that Epac1 activation contributes
to I/R injury; (2) either genetic ablation or pharmacological inhibition of Epac1 protected against I/R- or HX+R-induced cardiomyocyte apoptosis; (3) mechanistic studies demonstrated
that Epac1 was activated by sAC and promoted MPTP opening and cell death during HX+R; (4) Epac1 regulated different
654 Circulation Research February 17, 2017
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Figure 7. Epac1 regulates the mitochondrial localization of CaMKII (Ca2+/calmodulin-dependent protein kinase II), which inhibits
isocitrate dehydrogenase 2 (IDH2) activity. A, Quantification of mitochondrial CaMKII; B, total CaMKII; and C, cytosolic CaMKII protein
expression in the hearts of wild-type (WT) or Epac1−/− mice. Representative immunoblots of 4 independent experiments are shown.
GAPDH (glyceraldehyde-3-phosphate dehydrogenase) and voltage-dependent anion channel 1 (VDAC1) expression were used as loading
control of cytosolic and mitochondrial fractions, respectively. D, Quantification of mitochondrial CaMKII; and E, cytosolic CaMKII in
cardiomyocytes transfected with the indicated plasmids (n=6). Representative immunoblots are shown. F, Representative immunoblots
showing the interaction of IDH2 with CaMKII and Epac1 in cardiomyocytes stimulated or not with 8-pCPT-2′-O-Me-cAMP-AM (8-CPTAM; 10 μmol/L, 30 minutes) before immunoprecipitation (IP) experiments against IDH2. IgG and GAPDH were used as control for IP. Input
is a control of cell lysates. G, IDH2 activity; and H, NADPH/NADP ratio in isolated-mitochondria from the hearts of WT or Epac1−/− mice.
Mitochondria were preincubated or not with KN93 (5 μmol/L, 30 minutes) and stimulated or not (VEHICLE) with 8-CPT-AM (10 μmol/L, 30
minutes; n=7). Data are means±SEM and were evaluated by 2-way analysis of variance (ANOVA)/Bonferroni posttest. *P<0.05, **P<0.01,
***P<0.001, ****P<0.0001 vs control group or the indicated value. Epac1 indicates exchange protein directly activated by cAMP 1; and
NADPH, nicotinamide adenine dinucleotide phosphate hydrogen.
aspects of mitochondrial function, such as Ca2+ uptake, ROS
production, and MPTP opening. Our results further add credence that Epac1 is highly compartmentalized and functions as
an important stress response switch in the heart.
Our in vivo and in vitro data showed that the genetic ablation or the inhibition of Epac1 prevented cardiomyocyte apoptosis during I/R injury or HX+R stress, respectively. Recent
studies have shown that the various biological actions of Epac1
depend on its subcellular localization. Indeed, the perinuclear
localization of Epac1 in cardiomyocyte is consistent with its
role in the regulation of gene transcription during cardiac hypertrophic remodeling.16–18 Furthermore, independently of its
effect on sarcoplasmic reticulum function, Epac1 was reported
to act on the myofilament compartment where it regulates the
phosphorylation of sarcomeric proteins to increase myofilament Ca2+ sensitivity.33 Finally, Epac1 was previously found
in the mitochondrion of Epac1-transfected COS-7 cells in a
cell cycle–dependent manner,34 although it was not linked to
any biological function. Here we found that Epac1 is indeed
localized in the mitochondrion of cardiomyocytes, where it
exerts its regulatory role on cardiomyocyte cell death via its
activation by cAMP produced by sAC. These findings allow to
provide a mechanistic confirmation to the previously described
data, showing that sAC-dependent cAMP signaling modulated
the mitochondrial pathway of apoptosis in adult cardiomyocytes.21 These data also reinforce the importance of Epac1 localization because mainly MitEpac1 is involved in inducing
apoptosis in HX+R-cultured cells. During the course of our
study, Wang et al35 demonstrated that a modest increase in
mitochondrial cAMP levels, through direct activation of sAC
with HCO3–, prevented Ca2+-induced MPTP opening through
Epac1, which they assumed that Epac1 might protect from
cardiomyocyte death. Based on our observations, this pathway
is not operational in the setting of HX+R because MitEpac1
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Figure 8. Schema illustrating a working hypothesis of Epac1 signaling in ischemia/reperfusion (I/R) injury. In the setting of I/R,
soluble adenylyl cyclase type 10 (sAC) is activated to promote cAMP accumulation, thereby, activating mitochondrial Epac1 (MitEpac1).
MitEpac1 increases Ca2+ transfer from the endoplasmic reticulum (ER) to mitochondria via the VDAC1/GRP75/IP3R1 complex. In addition,
MitEpac1-CaMKII (Ca2+/calmodulin-dependent protein kinase II) forms a multiprotein complex with isocitrate dehydrogenase 2 (IDH2), a
critical enzyme of the tricarboxylic acid (TCA) cycle involved in reactive oxygen species (ROS) detoxification. CaMKII inhibits IDH2 activity
by Serine phosphorylation, thereby, decreasing nicotinamide adenine dinucleotide phosphate hydrogen (NADPH) synthesis in the matrix.
MitEpac1-induced mitochondrial Ca2+ overload and ROS accumulation promotes mitochondrial permeability transition pore (MPTP)
opening and myocardial cell death. α-KG indicates α-ketoglutarate; Epac1, exchange protein directly activated by cAMP 1; GRP75,
chaperone glucose-regulated protein 75; GSH, reduced glutathion; GSR, glutathione reductase; GSSG, Oxidized glutathion; IP3R1,
inositol-1,4,5-triphosphate receptor 1; MCU, mitochondrial Ca2+ uniporter; NADP+, nicotinamide adenine dinucleotide phosphate; and
VDAC1, voltage-dependent anion channel 1.
shows opposite effect, such as stimulation of mitochondrial
Ca2+ entry, MPTP opening, and cell death. One explanation for
this discrepancy could be the higher levels of cAMP production observed in the model of HX+R together with the activation of other actors, such as ROS and CaMKII signaling.
Altogether, these data strongly suggest a major role of the
mitochondrial sAC-Epac1 axis in the physiology and pathophysiology of the cardiomyocyte. These findings add up to
the accumulating evidence linking Epac protein signaling to
cardiomyocyte functions. Indeed, Epac proteins exert their
biological function in combination with scaffolding proteins,
such as β-arrestin, cAMP phosphodiesterases that regulates
the duration and intensity of cAMP signaling, and PKA.36,37
Because various mitochondrial compartments contain these
proteins that are able to sense or respond to cAMP and may
have antagonistic outputs,2 further studies are needed to identify the multimolecular complexes that affect cAMP-Epac1 signaling and Epac1 mitochondrial function in cardiomyocytes.
In this study, we also identified at least 2 different mechanisms that contribute to the deleterious activation of Epac1
during HX+R in vitro and possibly by extension to myocardial I/R injury in vivo. First, we identified Epac1 as a regulator of Ca2+ entry in the mitochondria. Indeed, the lack of
Epac1 prevented Ca2+ accumulation during HX+R. The
MCU was involved in this effect of Epac1 because RU360
reduced 8-CPT-AM-induced mitochondrial Ca2+ (Online
Figure VIIA). Because CaMKII increases MCU current31
and is a downstream effector of MitEpac1, we speculate that
Epac1 regulates Ca2+ entry into the mitochondria via CaMKIIdependent MCU activation. In addition, based on a previous
finding that Epac1 also induced cytosolic Ca2+ overload via
the production of IP3 and IP3R activation,38 we hypothesize
that Epac1 could induce IP3R channel opening from the ER
and subsequent Ca2+ transfer from the ER to the mitochondria.
Consistently, Epac1 controlled the assembly of the ER/mitochondrial VDAC1/GRP75/IP3R1 protein complex that has
been previously shown to influence Ca2+ exchange between
the ER and the mitochondria.25 Finally, Epac1-mediated mitochondrial Ca2+ overload subsequently provoked MPTP
opening, cytochrome c release, and eventually cell death.
Interestingly, cyclophilin D was also shown to interact with
the VDAC1/GRP75/IP3R1 complex at the mitochondria-associated ER membrane interface,26 and its inhibition prevented
mitochondrial Ca2+ overload by depressing ER/mitochondria
interactions and protected cells against lethal reperfusion injury.26 Therefore, our data show that the proper association of the
VDAC1/GRP75/IP3R1 complex is paramount to mitochondrial Ca2+ overload during HX+R, and that MitEpac1 plays
a crucial role in that process. Whether this Epac1-dependent
sarcoplasmic reticulum–mitochondria Ca2+ coupling may also
contribute to modulate the global Ca2+ homeostasis and excitation–contraction coupling in cardiomyocytes under physiological conditions has yet to be investigated.
Second, our study revealed a key role for Epac1 in the
accumulation of mitochondrial ROS production on HX+R.
Recently, Mukai et al39 reported that high glucose–induced
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mitochondrial ROS production in pancreatic β-cells was decreased by stimulation with the glucagon-like peptide-1 receptor ligand exendin-4 in an Epac-dependent manner. Here
we further showed that MitEpac1 inhibited IDH2 via its
phosphorylation on serine residues. This mitochondrial enzyme is primarily expressed in oxidative tissues, including
the heart and skeletal muscle, where it plays an essential role
in maintaining mitochondrial redox homeostasis.29 In cardiac
mitochondria, IDH2 is the major source of the mitochondrial
NADPH required for glutathione production and thioredoxin
recycling.40 Therefore, Epac1-mediated inhibition of IDH2 impaired NADPH production, hence, decreased the antioxidant
capabilities of the cardiomyocytes during HX+R. We extended our work to identify the signaling pathway that accounted
for Epac1-inhibited IDH2. Interestingly, we found that Epac1
promoted the mitochondrial matrix import of CaMKII, where
it interacted with and phosphorylated IDH2. Importantly,
these data could explain how CaMKII, which does not harbor
any N-terminal mitochondrial targeting sequence, transfers to
the mitochondria,31 although the precise mechanism remains
to be identified. Also, previous work has indicated that mitochondrial CaMKII directly controlled MCU activity by phosphorylation, thereby, regulating the rate of Ca2+ influx across
the inner mitochondrial membrane to influence MPTP and
subsequent cell death during myocardial I/R.31 However, the
cardiomyocytes of knockout mice for the MCU channel were
not protected against cardiomyocyte death after I/R injury,41
suggesting other CaMKII to be involved. Therefore, our identification of IDH2 as a CaMKII critical target in HX+R contributes to better understand the multifacet role of CaMKII in
this context. In contrast to what is observed in the heart, Epac1
activation prevented mitochondrial ROS accumulation by decreasing superoxide anion formation during renal I/R injury,
thus, limiting the degree of oxidative stress.42 Although these
findings seem contradictory, Epac signaling is spatially and
temporally regulated by diverse anchoring mechanisms that
control specific functions of this cAMP-sensitive guanine exchange factor by recruitment to distinct subcellular localizations.37 We, therefore, speculate that cell type–specific signals
contribute to differential effect of Epac on mitochondrial ROS
production.
To conclude, our finding provides a novel mechanism
in which different cAMP–Epac1 microdomains control the
mitochondrial cell death pathway (Figure 8). We propose a
model whereby, in the setting of I/R, Epac1 localized at the
mitochondria-associated ER membrane is activated by sAC
to induce mitochondrial Ca2+ overload via the ER/mitochondrial interaction and subsequent MPTP opening. In addition,
we unveil an unsuspected role report for Epac1 in recruiting
CaMKII at the mitochondria. MitEpac1–CaMKII pathway
also inhibited IDH2 activity via serine-dependent phosphorylation to reduce ROS detoxification, thereby, promoting cardiomyocyte death during I/R. Finally, our study highlights on
the therapeutic potential of Epac1 inhibition and the development of Epac1 pharmacological inhibitors as new drugs to
treat I/R injury. Because both Epac1 and IDH2 proteins have
been implicated in cancer, such as melanoma, they might
have more general clinical implications in other systems and
diseases.
Acknowledgments
We thank Jane-Lise Samuel for providing human myocardial samples
and Nicolas Vodovar for critical reading of the article. We acknowledge Corinne Evra and Cédric Baudelin and their staff for animal
housing (Plateforme Anexplo/Genotoul, UMS US006/INSERM/
UPS). We also acknowledge the support from Cellular Imaging
Facility platform I2MC (Madjid Zanoun).
Sources of Funding
F. Lezoualc’h was supported by grants from Institut National de la
Santé et de la Recherche Médicale, Fondation pour la Recherche
Médicale (Programme Equipes FRM 2016, DEQ20160334892),
Fondation de France (00066331), and Université de Toulouse. L.
Fazal and M. Laudette are supported by a fellowship from Fondation
Lefoulon-Delalande and a PhD training grant from Université de
Toulouse, respectively.
Disclosures
None.
References
1. Di Benedetto G, Scalzotto E, Mongillo M, Pozzan T. Mitochondrial
Ca²⁺ uptake induces cyclic AMP generation in the matrix and modulates organelle ATP levels. Cell Metab. 2013;17:965–975. doi: 10.1016/j.
cmet.2013.05.003.
2. Lefkimmiatis K, Zaccolo M. cAMP signaling in subcellular compartments. Pharmacol Ther. 2014;143:295–304. doi: 10.1016/j.
pharmthera.2014.03.008.
3. Acin-Perez R, Salazar E, Kamenetsky M, Buck J, Levin LR, Manfredi G.
Cyclic AMP produced inside mitochondria regulates oxidative phosphorylation. Cell Metab. 2009;9:265–276. doi: 10.1016/j.cmet.2009.01.012.
4. Lefkimmiatis K, Leronni D, Hofer AM. The inner and outer compartments
of mitochondria are sites of distinct cAMP/PKA signaling dynamics. J
Cell Biol. 2013;202:453–462. doi: 10.1083/jcb.201303159.
5. Ong SB, Samangouei P, Kalkhoran SB, Hausenloy DJ. The mitochondrial permeability transition pore and its role in myocardial ischemia
reperfusion injury. J Mol Cell Cardiol. 2015;78:23–34. doi: 10.1016/j.
yjmcc.2014.11.005.
6. El-Armouche A, Eschenhagen T. Beta-adrenergic stimulation and myocardial function in the failing heart. Heart Fail Rev. 2009;14:225–241. doi:
10.1007/s10741-008-9132-8.
7. Lameris TW, de Zeeuw S, Alberts G, Boomsma F, Duncker DJ, Verdouw
PD, Veld AJ, van Den Meiracker AH. Time course and mechanism of
myocardial catecholamine release during transient ischemia in vivo.
Circulation. 2000;101:2645–2650.
8. Yu QJ, Si R, Zhou N, Zhang HF, Guo WY, Wang HC, Gao F. Insulin inhibits beta-adrenergic action in ischemic/reperfused heart: a novel mechanism of insulin in cardioprotection. Apoptosis. 2008;13:305–317. doi:
10.1007/s10495-007-0169-2.
9. Scarabelli TM, Stephanou A, Pasini E, Comini L, Raddino R, Knight RA,
Latchman DS. Different signaling pathways induce apoptosis in endothelial cells and cardiac myocytes during ischemia/reperfusion injury. Circ
Res. 2002;90:745–748.
10. Sanada S, Asanuma H, Tsukamoto O, et al. Protein kinase A as another
mediator of ischemic preconditioning independent of protein kinase C.
Circulation. 2004;110:51–57. doi: 10.1161/01.CIR.0000133390.12306.
C7.
11. Insel PA, Zhang L, Murray F, Yokouchi H, Zambon AC. Cyclic AMP is
both a pro-apoptotic and anti-apoptotic second messenger. Acta Physiol
(Oxf). 2012;204:277–287. doi: 10.1111/j.1748-1716.2011.02273.x.
12. de Rooij J, Zwartkruis FJ, Verheijen MH, Cool RH, Nijman SM,
Wittinghofer A, Bos JL. Epac is a Rap1 guanine-nucleotide-exchange
factor directly activated by cyclic AMP. Nature. 1998;396:474–477. doi:
10.1038/24884.
13. Kawasaki H, Springett GM, Mochizuki N, Toki S, Nakaya M, Matsuda
M, Housman DE, Graybiel AM. A family of cAMP-binding proteins that
directly activate Rap1. Science. 1998;282:2275–2279.
14. Pereira L, Métrich M, Fernández-Velasco M, Lucas A, Leroy J, Perrier
R, Morel E, Fischmeister R, Richard S, Bénitah JP, Lezoualc’h F, Gómez
AM. The cAMP binding protein Epac modulates Ca2+ sparks by a Ca2+/
calmodulin kinase signalling pathway in rat cardiac myocytes. J Physiol.
2007;583:685–694. doi: 10.1113/jphysiol.2007.133066.
Fazal et al Role of Epac1 in Ischemia/Reperfusion Injury 657
Downloaded from http://ahajournals.org by on May 24, 2020
15. Pereira L, Cheng H, Lao DH, Na L, van Oort RJ, Brown JH, Wehrens XH,
Chen J, Bers DM. Epac2 mediates cardiac β1-adrenergic-dependent sarcoplasmic reticulum Ca2+ leak and arrhythmia. Circulation. 2013;127:913–
922. doi: 10.1161/CIRCULATIONAHA.12.148619.
16. Métrich M, Lucas A, Gastineau M, Samuel JL, Heymes C, Morel E,
Lezoualc’h F. Epac mediates beta-adrenergic receptor-induced cardiomyocyte hypertrophy. Circ Res. 2008;102:959–965. doi: 10.1161/
CIRCRESAHA.107.164947.
17. Laurent AC, Bisserier M, Lucas A, Tortosa F, Roumieux M, De Régibus A,
Swiader A, Sainte-Marie Y, Heymes C, Vindis C, Lezoualc’h F. Exchange
protein directly activated by cAMP 1 promotes autophagy during cardiomyocyte hypertrophy. Cardiovasc Res. 2015;105:55–64. doi: 10.1093/cvr/
cvu242.
18. Pereira L, Rehmann H, Lao DH, Erickson JR, Bossuyt J, Chen J, Bers
DM. Novel Epac fluorescent ligand reveals distinct Epac1 vs. Epac2
distribution and function in cardiomyocytes. Proc Natl Acad Sci U S A.
2015;112:3991–3996. doi: 10.1073/pnas.1416163112.
19. Courilleau D, Bisserier M, Jullian JC, Lucas A, Bouyssou P, Fischmeister
R, Blondeau JP, Lezoualc’h F. Identification of a tetrahydroquinoline analog as a pharmacological inhibitor of the cAMP-binding protein Epac. J
Biol Chem. 2012;287:44192–44202. doi: 10.1074/jbc.M112.422956.
20. Vliem MJ, Ponsioen B, Schwede F, Pannekoek WJ, Riedl J, Kooistra
MR, Jalink K, Genieser HG, Bos JL, Rehmann H. 8-pCPT-2’-O-MecAMP-AM: an improved Epac-selective cAMP analogue. Chembiochem.
2008;9:2052–2054. doi: 10.1002/cbic.200800216.
21. Appukuttan A, Kasseckert SA, Micoogullari M, Flacke JP, Kumar S,
Woste A, Abdallah Y, Pott L, Reusch HP, Ladilov Y. Type 10 adenylyl cyclase mediates mitochondrial Bax translocation and apoptosis of adult rat
cardiomyocytes under simulated ischaemia/reperfusion. Cardiovasc Res.
2012;93:340–349. doi: 10.1093/cvr/cvr306.
22. Bernardi P, Di Lisa F. The mitochondrial permeability transition pore: molecular nature and role as a target in cardioprotection. J Mol Cell Cardiol.
2015;78:100–106. doi: 10.1016/j.yjmcc.2014.09.023.
23. Trollinger DR, Cascio WE, Lemasters JJ. Selective loading of Rhod 2 into
mitochondria shows mitochondrial Ca2+ transients during the contractile
cycle in adult rabbit cardiac myocytes. Biochem Biophys Res Commun.
1997;236:738–742. doi: 10.1006/bbrc.1997.7042.
24. Pozzan T, Rudolf R. Measurements of mitochondrial calcium in
vivo. Biochim Biophys Acta. 2009;1787:1317–1323. doi: 10.1016/j.
bbabio.2008.11.012.
25. Szabadkai G, Bianchi K, Várnai P, De Stefani D, Wieckowski MR,
Cavagna D, Nagy AI, Balla T, Rizzuto R. Chaperone-mediated coupling
of endoplasmic reticulum and mitochondrial Ca2+ channels. J Cell Biol.
2006;175:901–911. doi: 10.1083/jcb.200608073.
26. Paillard M, Tubbs E, Thiebaut PA, Gomez L, Fauconnier J, Da
Silva CC, Teixeira G, Mewton N, Belaidi E, Durand A, Abrial M,
Lacampagne A, Rieusset J, Ovize M. Depressing mitochondria-reticulum interactions protects cardiomyocytes from lethal hypoxia-reoxygenation injury. Circulation. 2013;128:1555–1565. doi: 10.1161/
CIRCULATIONAHA.113.001225.
27. Bopassa JC, Michel P, Gateau-Roesch O, Ovize M, Ferrera R. Lowpressure reperfusion alters mitochondrial permeability transition. Am
J Physiol Heart Circ Physiol. 2005;288:H2750–H2755. doi: 10.1152/
ajpheart.01081.2004.
28. Chen YR, Zweier JL. Cardiac mitochondria and reactive oxygen species generation. Circ Res. 2014;114:524–537. doi: 10.1161/
CIRCRESAHA.114.300559.
29. Jo SH, Son MK, Koh HJ, Lee SM, Song IH, Kim YO, Lee YS, Jeong
KS, Kim WB, Park JW, Song BJ, Huh TL, Huhe TL. Control of mitochondrial redox balance and cellular defense against oxidative damage by
mitochondrial NADP+-dependent isocitrate dehydrogenase. J Biol Chem.
2001;276:16168–16176. doi: 10.1074/jbc.M010120200.
30. Lu J, Holmgren A. The thioredoxin antioxidant system. Free Radic Biol
Med. 2014;66:75–87. doi: 10.1016/j.freeradbiomed.2013.07.036.
31. Joiner ML, Koval OM, Li J, et al. CaMKII determines mitochondrial
stress responses in heart. Nature. 2012;491:269–273. doi: 10.1038/
nature11444.
32. Timmins JM, Ozcan L, Seimon TA, Li G, Malagelada C, Backs J, Backs T,
Bassel-Duby R, Olson EN, Anderson ME, Tabas I. Calcium/calmodulindependent protein kinase II links ER stress with Fas and mitochondrial
apoptosis pathways. J Clin Invest. 2009;119:2925–2941. doi: 10.1172/
JCI38857.
33. Cazorla O, Lucas A, Poirier F, Lacampagne A, Lezoualc’h F. The
cAMP binding protein Epac regulates cardiac myofilament function.
Proc Natl Acad Sci U S A. 2009;106:14144–14149. doi: 10.1073/
pnas.0812536106.
34. Qiao J, Mei FC, Popov VL, Vergara LA, Cheng X. Cell cycle-dependent
subcellular localization of exchange factor directly activated by cAMP. J
Biol Chem. 2002;277:26581–26586. doi: 10.1074/jbc.M203571200.
35. Wang Z, Liu D, Varin A, Nicolas V, Courilleau D, Mateo P, Caubere C,
Rouet P, Gomez AM, Vandecasteele G, Fischmeister R, Brenner C. A cardiac mitochondrial cAMP signaling pathway regulates calcium accumulation, permeability transition and cell death. Cell Death Dis. 2016;7:e2198.
doi: 10.1038/cddis.2016.106.
36. Berthouze-Duquesnes M, Lucas A, Saulière A, Sin YY, Laurent AC,
Galés C, Baillie G, Lezoualc’h F. Specific interactions between Epac1, βarrestin2 and PDE4D5 regulate β-adrenergic receptor subtype differential
effects on cardiac hypertrophic signaling. Cell Signal. 2013;25:970–980.
doi: 10.1016/j.cellsig.2012.12.007.
37. Lezoualc’h F, Fazal L, Laudette M, Conte C. Cyclic AMP sensor EPAC
proteins and their role in cardiovascular function and disease. Circ Res.
2016;118:881–897. doi: 10.1161/CIRCRESAHA.115.306529.
38. Ruiz-Hurtado G, Morel E, Domínguez-Rodríguez A, Llach A,
Lezoualc’h F, Benitah JP, Gomez AM. Epac in cardiac calcium signaling. J Mol Cell Cardiol. 2013;58:162–171. doi: 10.1016/j.yjmcc.
2012.11.021.
39. Mukai E, Fujimoto S, Sato H, Oneyama C, Kominato R, Sato Y, Sasaki M,
Nishi Y, Okada M, Inagaki N. Exendin-4 suppresses SRC activation and
reactive oxygen species production in diabetic Goto-Kakizaki rat islets
in an Epac-dependent manner. Diabetes. 2011;60:218–226. doi: 10.2337/
db10-0021.
40. Nickel AG, von Hardenberg A, Hohl M, et al. Reversal of Mitochondrial
Transhydrogenase Causes Oxidative Stress in Heart Failure. Cell Metab.
2015;22:472–484. doi: 10.1016/j.cmet.2015.07.008.
41. Pan X, Liu J, Nguyen T, Liu C, Sun J, Teng Y, Fergusson MM, Rovira
II, Allen M, Springer DA, Aponte AM, Gucek M, Balaban RS, Murphy
E, Finkel T. The physiological role of mitochondrial calcium revealed
by mice lacking the mitochondrial calcium uniporter. Nat Cell Biol.
2013;15:1464–1472. doi: 10.1038/ncb2868.
42. Stokman G, Qin Y, Booij TH, Ramaiahgari S, Lacombe M, Dolman ME,
van Dorenmalen KM, Teske GJ, Florquin S, Schwede F, van de Water
B, Kok RJ, Price LS. Epac-Rap signaling reduces oxidative stress in the
tubular epithelium. J Am Soc Nephrol. 2014;25:1474–1485. doi: 10.1681/
ASN.2013070679.