How AMPK and PKA Interplay to Regulate Mitochondrial Function and Survival in Models of Ischemia and Diabetes

Zhang, Jingdian; Wang, Yumeng; Liu, Xiaofeng; Dagda, Ruben K.; Zhang, Ying

doi:https://doi.org/10.1155/2017/4353510

Oxidative Medicine and Cellular Longevity

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New Insights into the Role of Oxidative Stress in Onset of Cardiovascular Disease

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Review Article | Open Access

Volume 2017 | Article ID 4353510 | https://doi.org/10.1155/2017/4353510

How AMPK and PKA Interplay to Regulate Mitochondrial Function and Survival in Models of Ischemia and Diabetes

Jingdian Zhang,¹Yumeng Wang,²Xiaofeng Liu,³Ruben K. Dagda,⁴and Ying Zhang¹

Academic Editor: Aneta Radziwon-Balicka

Received28 Jul 2017

Accepted02 Nov 2017

Published17 Dec 2017

Abstract

Adenosine monophosphate-activated protein kinase (AMPK) is a conserved, redox-activated master regulator of cell metabolism. In the presence of oxidative stress, AMPK promotes cytoprotection by enhancing the conservation of energy by suppressing protein translation and by stimulating autophagy. AMPK interplays with protein kinase A (PKA) to regulate oxidative stress, mitochondrial function, and cell survival. AMPK and dual-specificity A-kinase anchoring protein 1 (D-AKAP1), a mitochondrial-directed scaffold of PKA, interact to regulate mitochondrial function and oxidative stress in cardiac and endothelial cells. Ischemia and diabetes, a chronic disease that increases the onset of cardiovascular diseases, suppress the cardioprotective effects of AMPK and PKA. Here, we review the molecular mechanisms by which AMPK and D-AKAP1/PKA interplay to regulate mitochondrial function, oxidative stress, and signaling pathways that prime endothelial cells, cardiac cells, and neurons for cytoprotection against oxidative stress. We discuss recent literature showing how temporal dynamics and localization of activated AMPK and PKA holoenzymes play a crucial role in governing cellular bioenergetics and cell survival in models of ischemia, cardiovascular diseases, and diabetes. Finally, we propose therapeutic strategies that tout localized PKA and AMPK signaling to reverse mitochondrial dysfunction, oxidative stress, and death of neurons and cardiac and endothelial cells during ischemia and diabetes.

1. Introduction

AMPK is a heterotrimeric holoenzyme that consists of a catalytic subunit (α) bound to two regulatory subunits (β and γ). Due to the diverse arrangement of different isoforms of the three subunits of the AMPK holoenzyme, there can exist up to 12 different AMPK holoenzymes in different tissues, which add a layer of complexity AMPK-mediated regulation of critical physiological functions in eukaryotes [1, 2].

AMPK activity is induced by a high ratio of intracellular AMP to ATP levels. AMP directly binds to the regulatory subunit of AMPK to facilitate AMPK phosphorylation via the upstream protein kinase LKB1 [3]. Upon phosphorylation by LKB1, activated AMPK restores intracellular energy levels by inhibiting ATP-consuming biosynthetic pathways and by stimulating catabolic ATP-regenerating processes. Furthermore, AMPK is a redox-sensing kinase that regulates cellular bioenergetics. Indeed, mitochondrial-derived free radicals can activate AMPK through LKB1 without altering the ratio of AMP/ATP [4, 5].

AMPK can be activated via two different mechanisms: (1) phosphorylation of threonine 172 (Thr172) by upstream kinases or via autocatalytic-mediated phosphorylation or (2) by binding of AMP to AMPK. Specifically, LKB1, CaMKKb, or TAK1 can phosphorylate Thr172 within the activation loop of the α-subunit when AMP binds to the γ-subunit [2, 6–9]. All the aforementioned upstream kinases, as well as levels of AMP induced by acute/chronic stress, can activate AMPK to activate downstream biological functions [10]. Figure 1 and Supplementary Table S1 show ways that AMPK can be activated pharmacologically in a ROS-dependent manner.

Figure 1

Non-redox-dependent physiological, pharmacological, natural compounds and other conditions that activate AMPK in ischemic preconditioning. This figure highlights some of the well-established and newly discovered AMPK activators or conditions that have benefits in ischemic preconditioning. Pharmacological activators such as metformin and AICAR, some natural compounds, and physiological situations such as exercise and calorie restriction can activate AMPK by increasing the AMP : ATP ratio (shown in the blue rectangle), causing AMP to bind to the γ-subunit. However, a subset of conditions or pharmacological compounds can stimulate AMPK activation in IPC via other mechanisms, such as activated upstream kinases of the α-subunit (shown in the rounded rectangle named “other measures in IPC”), or binding directly to the β-subunit (A769662).

The phosphorylation and subsequent activation of AMPK elicit the following physiological functions depending on the type and intensity of toxic insult and oxidative stress: (1) regulation of metabolism and glucose uptake, (2) modulation of protein synthesis and cellular growth by inhibiting the mammalian target of rapamycin (mTOR) pathway, and (3) initiating autophagy during starvation or by specific conditions that induce severe stress [10]. In the context of metabolic stress (metabolic crisis), most cells or organs benefit from activation of AMPK signaling with the exception of brain tissue which has shown modest cytoprotection or detrimental outcomes during ischemia [11]. Activation of AMPK signaling regulates cell metabolism. For instance, AMPK stimulates fatty acid oxidation [12], mitochondrial biogenesis [13–15], glucose transporter type 4 (GLUT4) translocation, and glucose uptake [16–18], while inhibiting protein synthesis, gluconeogenesis, and fatty acid and cholesterol synthesis, [19–21] to increase ATP levels in order to reduce oxidative stress caused by metabolic crisis [22].

Mitochondria not only are regulators of oxidative phosphorylation and calcium homeostasis but also regulate a variety of converging cell death signaling pathways that activate programmed cell death. The mechanisms by which AMPK regulates mitochondrial function and cell survival have recently gained interest, but this area of research is still in its infancy. Recent evidence shows that AMPK has the capacity to regulate cellular bioenergetics, cell death, and mitochondrial structure/function and dynamics by interacting with PKA or, in parallel, during chronic or acute oxidative stress. In this review, we present evidence on the molecular mechanisms by which AMPK and PKA coregulate mitochondrial function and structure in cardiac cells and neurons, two cell types targeted in ischemia and in diabetes, a chronic disease that increases the risk for developing cardiovascular diseases (CVDs) and stroke. Indeed, the current global incidence of obesity and type 2 diabetes has increased in part due to a combination of sedentary lifestyle and high-calorie diets. Secondly, we highlight the importance of how the temporal dynamics and intracellular localization of activated AMPK and PKA holoenzymes play a critical role in regulating oxidative stress and cellular bioenergetics in cardiac cells, endothelial cells, and neurons.

2. AMPK Regulates Mitochondrial Dynamics, Function, and Structure

Since the mitochondria act as major “power plants” of eukaryotes, exploring the interaction between AMPK and mitochondria will shed more insight as to how cells maintain overall energy homeostasis and mitochondrial quality control [23, 24]. In addition, AMPK promotes mitochondrial biogenesis (generation of new mitochondria) in various tissues. For instance, by stimulating PGC1-α and NRF1/2 expression, AMPK participates in parallel to the E3 ubiquitin ligase Parkin to govern mitochondrial biogenesis, presumably as a compensatory response to preserve mitochondrial homeostasis [3, 25–27].

Mitochondrial fission/fusion and movement (trafficking) is regulated by protein phosphorylation imparted by a variety of ser/thr kinases including PKA and AMPK [28, 29]. Recently, there have been an increasing number of studies that show that AMPK regulates mitochondrial structure and function [5, 26, 30–32]. For instance, in neurons, AMPK signaling regulates anterograde transport of mitochondria in the axons of depolarized neurons [33]. In nonneuronal cells, AMPK signaling supports mitochondrial fragmentation (fission) of oxidatively damaged mitochondria by activating the fission modulator dynamin-related protein 1 (Drp1). In support of this concept, a landmark study recently showed that AMPK facilitates mitochondrial fission induced by acute treatment with the complex I inhibitor rotenone. Conversely, U2OS cells deficient for both the α and β subunits of AMPK are recalcitrant to mitochondrial fragmentation induced by mitochondrial-damaging compounds rotenone and antimicyn-A [29]. Mechanistically, AMPK activation promotes mitochondrial fission by phosphorylating mitochondrial fission factor (MFF) and by activating ULK [29, 34].

Cells require a minimum level of high-quality mitochondria to produce the necessary energy to thrive. Oxidatively damaged and effete mitochondria are continuously targeted for autophagolysosomal-mediated degradation via a selective physiological process termed mitophagy [35, 36]. Importantly, an increase in the turnover of mitochondria via mitophagy allows for not only the removal of damaged/effete mitochondria but also for the induction and integration of mitochondrial biogenesis pathways to restore mitochondrial levels [23]. Given that mitochondrial fission facilitates the induction of mitophagy [37], stimulating Drp1-dependent mitochondrial fission via AMPK signaling facilitates the removal of mitochondria via mitophagy [29, 34] in order to maintain a level of healthy mitochondria.

2.1. AMPK Regulates Mitochondrial Quality Control

AMPK is a bona fide regulator of mitochondrial dynamics, mitochondrial autophagy, and biogenesis. Indeed, when metabolic stress persists, damaged mitochondria will lead to robust Drp1-dependent mitochondrial fragmentation which can facilitate apoptosis [38, 39]. As mentioned before, activated AMPK triggers mitochondrial fission, at least in part via phosphorylation of MFF, which consequently activates the kinase ULK1 to initiate autophagy. Thus, AMPK may couple mitochondria fission to mitophagy in a continuous feed-forward cycle to maintain the levels of high-quality mitochondria and energy in the cell. A study by Toyama et al., 2016 shed insight on the mechanism by which AMPK activates fission in human U2OS osteosarcoma cells, SV40-immortalized murine embryonic fibroblasts (MEFs), and layer 2/3 cortical pyramidal neurons [29]. On the contrary, other research reports suggest that metformin can inhibit Drp1-mediated mitochondrial fission in endothelial cells of streptozocin- (STZ-) induced diabetic ApoE^−/− mice and in adipose tissue of STZ-induced diabetic WT mice [40, 41]. Overall, these studies suggest that AMPK can have opposing effects on mitochondrial fission/fusion, a phenomenon that likely depends on the bioenergetic status and levels of oxidative stress in the cell.

2.2. MFF Level Regulates AMPK-Mediated Fission

One possibility is that the levels of MFF may govern the ability of AMPK to regulate mitochondrial dynamics. MFF was observed to be in low abundance in human umbilical vein endothelial cells (HUVECs) and human vascular smooth muscle cells (HVSMCs) [41]. In addition, AMPK has been found to directly mediate mitochondrial fission via MFF in response to energy stress [29]. Neurons contain intermediate levels of MFF level while MFF is undetectable in astrocytes and brain endothelial cells or other heart or muscle tissues according to the Human Protein Atlas Program. In peripheral tissues, MFF levels are low including myocytes, hepatocytes, endothelial cell, astrocytes, and in renal glomeruli. AMPK regulates mitochondrial fission through MFF in U2OS cells [29]. Interestingly, AMPK may induce mitochondrial fusion in cells that are chronically stressed or in certain pathological conditions. For instance, endothelial cells from streptozotocin- (STZ-) induced diabetic ApoE^−/− mice treated with metformin show an inhibition of Drp1-mediated mitochondrial fission [41]. In addition, AMPK activation inhibits high glucose-induced Drp1-mediated mitochondrial fission in epididymal adipose tissue both in vitro and in in vivo [40]. Supplementary Table S2 gives a comprehensive list of pharmacological compounds that confer protection in cells by activating AMPK in a non-ROS manner (Supplementary Materials online, Table S2). Adipose tissue, another tissue with low levels of MFF, benefits from the inhibition of mitochondrial fission via AMPK activation in hyperglycemic conditions. Overall, it is likely that the levels of oxidative stress and the extent of mitochondrial damage dictate whether AMPK promotes fusion or fission. Future studies that elucidate the mechanisms by which oxidative stress regulates AMPK-mediated mitochondrial fission/fusion are warranted.

During physiological conditions, neurons require a continuous distribution of mitochondria across long distances including dendrites, axons, and synapses in order to meet end-to-end energy requirements, neurotransmission, dendrite development, and efficient Ca⁺²buffering [42]. Given that AMPK regulates mitochondrial movement in neurons [33], it is conceivable that neurons contain a higher level of MFF to achieve a minimum level of mitochondrial trafficking required in very extensive and vast neuronal networks. Hence, AMPK activation induces diverse effects on mitochondria dynamics which partly depends on levels of endogenous MFF across different tissues.

3. Role of AMPK as a Redox Sensor of Mitochondrial ROS

The mitochondria are the main generators of cellular ATP production via oxidative phosphorylation. However, if protein complexes embedded in the inner mitochondrial membrane or enzymes which catalyze cascade of redox reactions in ETC lose their tight association with the IMM or are damaged, electrons will leak and consequently generate detrimental levels of ROS by interacting with oxygen [43]. For instance, electrons can leak from complex I and react with oxygen to generate superoxide [44, 45]. Indeed, the mitochondria are the primary source of intracellular ROS levels and contribute up to 95% of total ROS levels [46].

Transient and moderate levels of ROS during preconditioning will induce cytoprotective responses by regulating either protein function and/or gene expression [47]. Recent ischemia preconditioning studies show that ROS-mediated activation of AMPK is associated with resistance against ischemia. A myriad of different toxic and physiological stimuli that activate AMPK can exert cytoprotection in models of ischemia. For instance, Supplementary Table S1 shows that hydrogen peroxide, hypoxic conditions, low glucose concentrations, thyroid hormone, and many drugs can activate AMPK in a ROS-dependent manner despite a stable ratio of AMP/ATP [4, 5, 30, 31, 48, 49] (Supplementary Materials online, Table S1).

3.1. Redox-Activation of AMPK Regulates Cell Survival during Ischemia

Sublethal hypoxic and ischemic events (ischemic preconditioning) or some drugs can enhance the tolerance of tissues and organs, to subsequent lethal injury induced by hypoxia, ischemia, and ischemia-reperfusion [50]. The induction of this ischemic tolerance can be achieved by three major approaches: (1) ischemic conditioning, (2) hypoxic conditioning, and (3) chemical conditioning [51]. Interestingly, hypothermic preconditioning exerts a more pronounced cardioprotective effect than ischemic preconditioning [52]. AMPK can be activated by ischemic preconditioning as well [4, 5, 30, 48, 49, 52–54]. In this context, mitochondrial-derived ROS induced by different preconditioning paradigms leads to activation of AMPK and induces resistance to subsequent lethal injury. Mechanistically, ROS scavengers or compound C can both diminish this protection alone suggesting that ROS is a modulator of AMPK-dependent cytoprotection against ischemia [30, 48, 53]. The fact that cells deficient in mitochondrial DNA (ρ0 cells), or cells treated with mito-TEMPO, fail to activate AMPK [4, 5] and abolishes the protective effects induced by ischemic conditioning further corroborates the concept that mitochondrial ROS is required to confer protection against ischemic insults [30].

4. The Diverse Effects of AMPK Activation on Ischemia, Ischemia-Reperfusion, and Preconditioning in the Brain

Some studies have shown that AMPK activation via ischemic preconditioning can prevent injury during ischemia-reperfusion in many organs including the heart, liver, and kidney [49, 55–58]. In contrast, investigators found that acute activation of AMPK prior to lethal ischemia is detrimental to the brain, whereas mild activation of AMPK signaling is beneficial [58–60]. Indeed, the authors of those studies demonstrated detrimental outcomes in vivo and in vitro as evident by the induction of larger infarct volumes, lower neurobehavioral scores, and decreased cell viability compared to control groups.

It is conceivable that the detrimental effects of acute and prolonged activation of AMPK prior to ischemia depend on both the metabolic status and mitochondrial health of neurons prior to ischemia. Given that neurons consume the majority of glucose (~20% of total glucose) and rely on oxidative phosphorylation to thrive, neurons predominantly utilize glucose as their main substrate for producing energy via oxidative metabolism [61]. However, neurons lack or contain very low levels of the 6-phosphofructo-2-kinase (PFK2) which is required to synthesize fructose-2,6-bisphosphate (F2,6P2), a powerful allosteric activator of PFK1 [62, 63]. Neurons can oxidize fatty acids and utilize amino acids. Hence, when ischemia ensues, p-AMPK will not lead to an increase in glycolysis but increased fatty acid oxidation in neurons, leading to enhanced oxidative phosphorylation to restore the ATP levels. Enhanced AMPK signaling in the brain under anaerobic conditions or hypoglycemia leads to metabolic failure during ischemia with detrimental consequences. Hence, increased AMPK signaling does not consistently protect neurons from ischemia insult as in other cells such as myocyte, hepatocyte, renal cell, endotheliocyte, or even adjacent astrocytes [11, 56, 57, 64].

Over the past decades, other investigators have made considerable efforts to illustrate the role of AMPK in cerebral ischemia. In order to avoid the off-target effects by drugs that activate AMPK, genetic models that ablate the expression for either the α1or α2 catalytic subunit of AMPK have been examined to further elucidate the in vivo role of AMPK in cerebral ischemia [65, 66]. Since AMPK activation likely enhances metabolism and survival of astrocytes as in peripheral tissues, increased AMPK activity can provide a favorable bioenergetics environment for neurons via the lactate shuttle [11]. Hence, future studies should explore whether AMPK can be activated specifically in CNS neurons. Indeed, a recent paper shed light on the effects of AMPK activation in neurons in vivo [67]. In brief, one study showed that AMPK is not activated in neurons during lethal ischemia phase but only during the ischemic preconditioning phase induced by cortical spreading depression (CSD) prior to the onset of ischemia. In addition, CSD enhances ischemic tolerance to temporary focal ischemia and a significant increase in the levels of phosphorylated α subunit of AMPK occurs 12 h. following CSD [67, 68]. The increased level of phosphorylated α subunit of AMPK was restricted to neurons—neurons predominantly located within the superficial layers of the cerebral cortex—but was not observed in astroglial cells. This observation was further confirmed by Shen et al. 2017 [67].

5. AMPK Can Be a Double-Edged Sword during Ischemia

Based on the aforementioned studies, we can conclude that acute AMPK activation prior to ischemia is protective in peripheral tissues but leads to a detrimental outcome in the brain [49, 56, 57, 64, 69, 70]. As mentioned before, these stark contradictions may be explained by the inherent energy metabolism conditions of neurons prior to the onset of toxic insults (e.g., AMPK increases oxidative phosphorylation during anaerobic conditions if activated during ischemia). However, the extent of activation of the AMPK-MFF-mitochondrial fission axis during ischemia may also contribute to these disparate effects [29, 40, 41]. Hence, future studies in in vivo models of ischemia are warranted to understand the role of the AMPK-MFF-fission pathway on neuronal survival in the context of ischemia.

However, there is a consensus that brief periods of AMPK activation prior to ischemia can enhance neuronal survival whereas sustained activation of AMPK induces cell death [11, 60, 67]. In addition, diverse stimuli that can lead to transient AMPK activation, such as brief glutamate exposure [71] and mild mitochondrial-uncoupling stimuli [72, 73]; brief periods of oxygen glucose deprivation in vitro [74]; or brief and intermittent blood vessel occlusion cycle in vivo [60], and CSD [67] can enhance tolerance to ischemia in an AMPK-dependent manner. AMPK activation in this manner prevents neurons from degenerating during ischemia or ischemia/reperfusion by initiating autophagy [67, 74], inducing translocation of glucose transporter 3 (GLUT3) [71], and promoting higher mitochondrial membrane potential to maintain Ca⁺² homeostasis [75] or directly decrease AMPK levels in lethal ischemia [60]. Therefore, AMPK is an enticing target for eliciting neuroprotection via ischemia preconditioning in the brain despite its proapoptotic role during lethal ischemia. This concept is further elaborated below in Section 8. However, this phenomenon is just another example of the importance of ischemic preconditioning and reinforces the concept that “what does not kill you will make you stronger”, quoted by Annalisa Carlucciby Nietzsche.

6. D-AKAP1 Interacts with AMPK to Regulate Survival: Implications for Ischemia/Diabetes

D-AKAP1 (AKAP140/149 and other splice variants AKAP121, sAKAP84) is a protein scaffold that targets PKA to the outer mitochondrial membrane (OMM) to phosphorylate the proapoptotic protein BAD and the profission protein Drp1 [76, 77] to induce mitochondrial fusion and stabilize mitochondrial networks, a phenomenon that is associated with enhanced neuroprotection against toxic insults [28, 77, 78].

Recent evidence suggests that D-AKAP1 and AMPK interact to regulate mitochondrial function and structure. Indeed, D-AKAP1 is a substrate of AMPK. By using targeted in vitro AMPK screens and phosphorylation prediction algorithms, one recent study elegantly showed that D-AKAP1 is a substrate of AMPK in skeletal muscle cells [79]. The physiological effects of AMPK-mediated phosphorylation of D-AKAP1 include an increase in oxidative phosphorylation and mitochondrial-mediated β oxidation of lipids in L6 myoblasts. Mechanistically, AMPK phosphorylates D-AKAP1 in S103 to maintain mitochondrial respiration and transmembrane potential [79]. However, it remains to be seen whether AMPK phosphorylates D-AKAP1 in other tissues. Moreover, it remains to be known whether AMPK-mediated phosphorylation of D-AKAP1 affects mitochondrial dynamics and quality control. In addition, it is conceivable that AMPK uncouples PKA from D-AKAP1 to promote mitochondrial fission and mitophagy. Indeed, there is rationale and evidence that other signaling pathways can uncouple PKA from D-AKAP1 to promote fission. For instance, PINK1, a ser/thr mitochondrial kinase mutated in recessive forms of Parkinson’s disease, triggers the displacement of PKA from D-AKAP1 during toxic insults that damage mitochondria and thereby ensures that fission of damaged mitochondria promotes mitophagy [80]. Hence, during oxidative stress, it is conceivable that AMPK-mediated phosphorylation of D-AKAP1 may limit the accessibility of PKA to D-AKAP1, presumably to allow AMPK to phosphorylate MFF as a feed-forward mechanism to promote mitochondrial fission. In summary, we raise the possibility that AMPK and D-AKAP1/PKA participate in a “tug of war” to regulate mitochondrial fission/fusion. For instance, increased AMPK signaling may induce mitochondrial fission by opposing D-AKAP1/PKA. The D-AKAP1-PKA-Drp1signaling axis promotes mitochondrial fusion whereas the AMPK-mitochondrial fission/fusion signaling axis leads to mitochondrial fragmentation and subsequent activation of mitophagy during toxic stress in neurons, both pathways leading to increased cell survival and mitochondrial homeostasis. However, in the absence of D-AKAP1/PKA signaling during oxidative stress, AMPK can act as a beneficial, compensatory signaling pathway to exert cytoprotection as elaborated below.

There is clear evidence that AMPK can converge at the mitochondrion to enhance protective D-AKAP1/PKA signaling. As reiterated, PKA-mediated phosphorylation of Drp1 via D-AKAP1 promotes mitochondrial fusion and prevents the activation of apoptosis in cells [28]. However, in models of diabetes and chronic stress, PKA-mediated phosphorylation of Drp1 is decreased, leading to mitochondrial fission [40, 81]. Treating cells with AMPK activators such as metformin or AICAR restores mitochondrial interconnectivity by enhancing PKA-mediated phosphorylation of Drp1 [49, 53]. However, additional studies are warranted to unveil the mechanism by which AMPK signaling interplays with mitochondrial PKA in models of ischemia and diabetes.

Beyond the mitochondrion, AMPK and PKA have been shown to cross-talk and interact in a feed-forward manner. For instance, treating vascular smooth muscle cells with AICAR not only stimulates AMPK signaling but also enhances PKA signaling [82]. However, the mechanisms by which these two holoenzymes interact, and whether this interaction occurs in cardiac cells, remain to be elucidated in future studies.

D-AKAP1 is a cardioprotective protein scaffold of PKA. D-AKAP1 is rapidly targeted for proteolytic degradation during oxidative stress via the E3 ligase Siah2 during ischemia [83, 84]. Chronic depletion of endogenous D-AKAP1, as evident in D-AKAP1 knockout mice, show aberrant mitochondrial structure as assessed by electron microscopy, increased ROS production, and reduced mitochondrial function following myocardial infarction (MI). These alterations were associated with robust cardiac mitophagy and apoptosis. Interestingly, reductions in D-AKAP1 levels are correlated with increased infarct size following myocardial infarction in D-AKAP1^−/− mice subjected to ligation of the left coronary artery [84]. However, this study did not address whether elevated mitophagy observed in D-AKAP1 knockout mice subjected to MI is phenocopied by AMPK activation. Consistent with this study, another study showed that a rat model of cardiac hypertrophy depletes D-AKAP1 levels in heart tissue, molecular pathology that is associated with mitochondrial dysfunction [85]. Furthermore, cardiac hypertrophy led to a decrease in endogenous levels of D-AKAP1 via downregulation of nuclear-localized cAMP signaling pathways and significantly increased ROS production [85].

Autophagy may be protective during ischemia, whereas it may be detrimental during reperfusion [86–88]. Thus, D-AKAP1 and AMPK stimulate mitochondria biogenesis and coregulate mitochondrial fission/fusion. Therefore, the interplay of these two proteins during oxidative stress may explain how these two ser/thr kinase govern ischemic preconditioning. Hence, we propose that maintaining normal levels of D-AKAP1 is necessary to preserve a pool of high quality and healthy mitochondria while low levels of D-AKAP1 may stimulate mitophagy, presumably via AMPK activation, of damaged mitochondria following ischemic conditioning (Figure 2).

Figure 2

Model on how AMPK and D-AKAP1/PKA cooperate to regulate mitochondrial structure/function under physiological conditions and during oxidative stress induced by diabetes and ischemia. During homeostasis (indicated in shaded blue), D-AKAP1/PKA and AMPK regulate mitochondrial structure and function to maintain a high ATP/ADP ratio. D-AKAP1/PKA phosphorylates Drp1 at the OMM to inhibit its fission activity and, thereby, promote mitochondrial fusion and maintain oxidative phosphorylation. Concomitantly, AMPK phosphorylates D-AKAP1 leading to stable mitochondrial bioenergetics and structure through an unknown molecular mechanism. These posttranslational events lead to enhanced mitochondrial biogenesis and cell survival. On the other hand, acute or a transient increase in the level of oxidative stress (indicated in shaded red) leads to decreased kinase signaling (uncoupling of PKA from D-AKAP1) and decreased mitochondrial oxidative phosphorylation and mitochondrial dysfunction (decreased transmembrane potential), ensuing mitochondrial damage. AMPK phosphorylates MFF to promote mitochondrial fission, a cellular event that is associated with increased mitophagy. However, is not known whether increased AMPK-mediated fission enhances mitophagy or increased cell survival (conceptual gaps indicated by question marks). On the other hand, conditions that promote ischemia or chronic high levels of oxidative stress, as observed in models of diabetes and CVDs, leads to rapid degradation of endogenous D-AKAP1 through Siah2 (hypoxia), decreased AMPK signaling (diabetes models), increased superoxide levels, and decreased compensatory responses to replenish high quality mitochondria and eventual cell death.

7. The Dual Roles of AMPK Signaling in Diabetes

AMPK has dual effects on mitochondrial function and structure, which likely depends on the levels of oxidative stress of cells. Under physiological conditions, AMPK promotes mitochondrial fission, presumably to stimulate mitophagy as a protective mitochondrial quality control mechanism [29]. However, in chronically stressed cells, AMPK confers cytoprotection, presumably by promoting mitochondrial fusion, mitochondrial biogenesis, eliciting antioxidant responses, and restoring mitochondrial function [29, 89, 90]. Another study showed that enhancing AMPK signaling promotes mitochondrial fusion and reduces cell death caused by ischemia/reperfusion in vivo and in vitro [30].

Diabetes increases the risk for damaging endothelial cells and heart tissue. In addition, AMPK signaling is protective in several in vivo models of diabetes [91]. For instance, in vivo rodent models of diabetes exhibit decreased AMPK-mediated signaling (Thr-172 phosphorylation), in liver and kidney tissues [26]. Therefore, reduced AMPK signaling is associated with an inability of cells to mount necessary AMPK-mediated responses to compensate for the loss of energy and mitochondrial dysfunction (Figure 2). In cell cultures of diabetes, enhancing AMPK signaling can protect cells against hyperglycemia and hypoglycemia [91]. For instance, cell stress induced by hyperglycemia can elicit Drp1-mediated mitochondrial fission and increased mitochondrial superoxide, cytopathology that is reversed by elevating AMPK signaling [92]. In addition, pancreatic β cells maintained in low levels of glucose exhibited an increase in superoxide levels, decreased mitochondrial oxidative phosphorylation, and robust phosphorylation of AMPK and of AMPK substrates [31]. However, the physiological implications for AMPK activation in pancreatic β cells remain to be elucidated in this context.

Pharmacological activators of AMPK are cardioprotective in models of diabetes.

Indeed, the AMPK activator metformin efficiently reduces the steady-state levels of mitochondrial superoxide and mitochondrial fission in endothelial cells derived from streptozocin-treated rats, a well characterized in vivo model for diabetes [26]. The protective effects of metformin require AMPK activation as transfecting hyperglycemic HUVECs with a constitutively active mutant of AMPK phenocopies the ability of metformin for blocking Drp1-mediated mitochondrial fission and Drp1-mediated increased levels of mitochondrial superoxide [41]. Another study showed that rats treated with streptozocin for four weeks showed a marked reduction in the levels of superoxide, decreased mitochondrial biogenesis, decreased oxidative phosphorylation, and phosphorylation of AMPK in the heart and the kidney [26]. Pharmacologically cotreating streptozocin-treated mice with the AMPK activator AICAR restores AMPK signaling, reverses mitochondrial pathology, restores mitochondrial oxidative phosphorylation, and reverses kidney pathology, further supporting the concept that activating AMPK signaling is protective in models of diabetes [26] (Supplementary Materials online, Table S2). In another study, treating streptozocin/ApoE^−/− mice with metformin was able to reduce mitochondrial fragmentation [41].

Physiological activation of AMPK activation can protect the heart from ischemia by upregulating glucose uptake and energy-generating glycolytic pathways as well as enhancing fatty acid oxidation. Specifically, phosphorylation of phosphofructokinase [63] by AMPK can promote the generation of ATP via glycolysis [63]. However, downstream ischemia-protective pathways activated by AMPK are blunted in type 2 diabetes. In this context, heart tissue exhibits little flexibility to compensate for energy loss in a similar manner to what neurons undergo during ischemia (Figure 2). A high body mass index and obesity are risk factors for developing CVDs and diabetes. Interestingly, endogenous mRNA levels of D-AKAP1 and of type II regulatory subunit of PKA (PKA/RIIβ) have been observed to be decreased in adipocytes and subcutaneous adipose tissue of obese individuals [93, 94]. Although is not known whether D-AKAP1 levels are downregulated in tissues of diabetes individuals, it is worth noting that D-AKAP1 is transcriptionally regulated by PPRγ in a PKA-dependent manner [93]. Therefore, given that PPRγ-mediated signaling is impaired in type II diabetes, these observations suggest that decreased expression of D-AKAP1 and PKA/RIIβ—proteins involved in lipolysis and mitochondrial metabolism—may contribute to the pathology in CVDs and type II diabetes subjects with a high BMI. In addition, patients with type 2 diabetes (T2D) are highly susceptible to developing CVD and restoring normoglycemia alone is insufficient for reducing the risk of CVDs in T2DM [95] suggesting that other therapeutic strategies need to be developed to reduce the onset of cardiovascular complications. In support of this concept, several known antidiabetic drugs in clinical work are used to reduce the incidence of diabetes-related CVDs such as metformin, thiazolidinediones (TZDs), and statins. Indeed, Cilostazol has been shown to restore AMPK activation and exert cardio- and vasculoprotective actions in in vivo or in vitro [96–102].

8. Therapeutic Perspectives

Diabetic individuals are highly prone to experiencing strokes, minitransient ischemic episodes, and other cerebral vascular complications [91]. As mentioned before, there is a consensus that AMPK is protective in models of diabetes. Given that the levels of AMPK signaling are severely compromised in diabetic tissues [26, 103], normalizing AMPK activity—as induced by metformin—continues to be an enticing therapeutic strategy for treating diabetes. On the other hand, it is not clear whether eliciting AMPK signaling is protective in models of ischemia. Some studies have shown that AMPK is protective during the ischemic phase in mice subjected to ischemia/reperfusion paradigms [104]. In vitro, pharmacologically pretreating tissues with AMPK activators can protect in cell culture and in vivo models of ischemia [15, 105, 106] (Supplementary Materials online, Table S2). Conversely, one in vivo study showed that inhibitors of AMPK activity increased protection against brain damage following ischemia [107]. Hence, future studies are warranted to further identify specific “windows” of opportunity by which AMPK confers robust neuroprotection during ischemia.

8.1. D-AKAP1: An AMPK Substrate with Therapeutic Applications

Overall, the aforementioned published data suggests that PKA and AMPK converge in the mitochondrion to enhance cytoprotection against ischemia. However, as mentioned before, how mitochondrial PKA (D-AKAP1/PKA) and AMPK cooperate to regulate survival of neurons or cardiac cells depends on the oxidative status of cells. During chronic stress, which may decrease PKA signaling in mitochondria, AMPK may serve to promote mitophagy. However, during physiological conditions, both kinases may cooperate to maintain mitochondrial function and survival. Consistent with the concept that AMPK and mitochondrial PKA cooperate to maintain cell survival during ischemia, one study demonstrated that PKA-mediated phosphorylation of Drp1 and PKA-mediated mitochondrial fusion during nitrite-preconditioning conditions exert cytoprotection of cardiac myocytes against ischemia in vivo and in vitro [30]. Nitrite-induced PKA-mediated protection of cardiac cells against ischemia requires AMPK activity and mitochondrial ROS [30]. Hence, given that AMPK signaling is blunted in diabetes, these studies suggest that therapeutic interventions that activate mitochondrial PKA can be beneficial to prevent the onset of ischemia in diabetes.

D-AKAP1 is highly sensitive to proteolytic degradation via the E3 ubiquitin ligase Siah2 during ischemia [83, 108]. Given that D-AKAP1 robustly and rapidly undergoes Siah2-mediated degradation during ischemia, it is conceivable that small molecular compounds that can coactivate PKA or stabilize endogenous levels of D-AKAP1 may confer significant protection during ischemia. There is experimental evidence to support this notion. For instance, Siah2 knockout mice exhibit little heart pathology after being subjected to ischemia reperfusion (e.g., myocardial infarct size) [108]. Cells treated with diffusible cyclic AMP analogues can increase the expression of D-AKAP1 in cell culture studies [109]. Therefore, it is conceivable that other PKA activators (e.g., forskolin) could be employed to increase D-AKAP1 in vivo to prevent the degradation of D-AKAP1 during ischemia.

There is significant controversy on the consequences of global activation of PKA on cell survival during ischemia. For instance, overt PKA activation exacerbates pathology in heart tissue during ischemia. Indeed, excessive β-adrenergic receptor activation leads to activation of protein kinase A (PKA), leading to increased opening of the L-type calcium currents and a subsequent increase in cytosolic calcium levels, the latter being potentially harmful to cardiac tissue [110, 111]. On the other hand, treating ischemic heart tissue with H89, an inhibitor of protein kinase A, promotes postischemic cardiac contractile recovery and reduces infarct size [112]. In neurons, the binding of cyclic AMP to the regulatory subunit of PKA is rapidly inhibited during the acute phase of cerebral ischemia, leading to reduced neuronal survival [113–115]. Hence, in this case, enhancing PKA signaling prior to ischemia may prove beneficial.

In addition, activation of global PKA activity can negate the protective effects of AMPK in different models of chronic stress and degeneration. For instance, while different studies have shown that PKA governs AMPK-mediated mitochondrial biogenesis and cytoprotection [25, 116], cytosolic PKA has been shown to oppose various physiological effects of AMP kinase in insulin-signaling cells and blocks the ability of metformin for decreasing glucose levels in primary hepatocytes [117, 118].

Given that D-AKAP1 is a substrate of AMPK, it is conceivable that compounds that elicit AMPK-mediated phosphorylation of D-AKAP1 are a better therapeutic option as opposed to using global PKA activators (e.g., forskolin) for conferring neuroprotection during ischemia. On the other hand, AMPK-activating compounds such as AICAR increases PKA signaling in vitro [82]. Hence, it remains to be seen whether cotreatment of heart cells or neurons with AMPK and PKA-stimulating compounds exert an additive, protective effect during ischemia. Alternatively, compounds that increase the endogenous levels of D-AKAP1 can offer cytoprotection in models of ischemia. Experimentally induced cardiac infarct depletes D-AKAP1 levels, molecular pathology that is associated with mitochondrial dysfunction [85]. In that study, cyclic AMP analogues were used to increase endogenous D-AKAP1 levels to protect cardiac cells from ischemia insult. To this end, it is conceivable that pharmacological compounds that increase D-AKAP1 levels can be used in hypertensive individuals with left ventricular hypertrophy. Therefore, we raise the possibility that D-AKAP1/PKA and AMPK are novel therapeutic targets for treating ischemia. However, future studies are warranted to elucidate whether single or dual pharmacological activation of mitochondrial PKA or AMPK can confer protection during ischemia.

Conflicts of Interest

The authors have no conflicts of interest to declare.

Acknowledgments

This work was supported by a National Institutes of Health Grant GM103554 (to Ruben K. Dagda) and by a crosswise project Grant 3R2168713428 from the Department of Science and Technology of Jilin Province (to Ying Zhang).

Supplementary Materials

Table S1: Different conditions that induce AMPK activation through ROS. Table S2: Other conditions that activate AMPK in a non-ROS-mediated mechanism. (Supplementary materials)

References

D. G. Hardie, “AMP-activated/SNF1 protein kinases: conserved guardians of cellular energy,” Nature Reviews Molecular Cell Biology, vol. 8, no. 10, pp. 774–785, 2007.
View at: Publisher Site | Google Scholar
D. Carling, M. J. Sanders, and A. Woods, “The regulation of AMP-activated protein kinase by upstream kinases,” International journal of obesity, vol. 32, Supplement 4, pp. S55–S59, 2008.
View at: Publisher Site | Google Scholar
L. Hang, J. Thundyil, and K. L. Lim, “Mitochondrial dysfunction and Parkinson disease: a Parkin-AMPK alliance in neuroprotection,” Annals of the New York Academy of Sciences, vol. 1350, no. 1, pp. 37–47, 2015.
View at: Publisher Site | Google Scholar
B. M. Emerling, F. Weinberg, C. Snyder et al., “Hypoxic activation of AMPK is dependent on mitochondrial ROS but independent of an increase in AMP/ATP ratio,” Free Radical Biology & Medicine, vol. 46, no. 10, pp. 1386–1391, 2009.
View at: Publisher Site | Google Scholar
Y. Han, Q. Wang, P. Song, Y. Zhu, and M. H. Zou, “Redox regulation of the AMP-activated protein kinase,” PLoS One, vol. 5, no. 11, article e15420, 2010.
View at: Publisher Site | Google Scholar
A. Woods, S. R. Johnstone, K. Dickerson et al., “LKB1 is the upstream kinase in the AMP-activated protein kinase cascade,” Current Biology, vol. 13, no. 22, pp. 2004–2008, 2003.
View at: Publisher Site | Google Scholar
M. Momcilovic, S. P. Hong, and M. Carlson, “Mammalian TAK1 activates Snf1 protein kinase in yeast and phosphorylates AMP-activated protein kinase in vitro,” The Journal of Biological Chemistry, vol. 281, no. 35, pp. 25336–25343, 2006.
View at: Publisher Site | Google Scholar
K. A. Anderson, T. J. Ribar, F. Lin et al., “Hypothalamic CaMKK2 contributes to the regulation of energy balance,” Cell Metabolism, vol. 7, no. 5, pp. 377–388, 2008.
View at: Publisher Site | Google Scholar
S. A. Hawley, M. Davison, A. Woods et al., “Characterization of the AMP-activated protein kinase kinase from rat liver and identification of threonine 172 as the major site at which it phosphorylates AMP-activated protein kinase,” The Journal of Biological Chemistry, vol. 271, no. 44, pp. 27879–27887, 1996.
View at: Publisher Site | Google Scholar
S. Krishan, D. R. Richardson, and S. Sahni, “Adenosine monophosphate-activated kinase and its key role in catabolism: structure, regulation, biological activity, and pharmacological activation,” Molecular Pharmacology, vol. 87, no. 3, pp. 363–377, 2015.
View at: Publisher Site | Google Scholar
B. Manwani and L. D. McCullough, “Function of the master energy regulator adenosine monophosphate-activated protein kinase in stroke,” Journal of Neuroscience Research, vol. 91, no. 8, pp. 1018–1029, 2013.
View at: Publisher Site | Google Scholar
R. Kirchmair, J. Dong, H. Xu et al., “Nesfatin-1 stimulates fatty-acid oxidation by activating AMP-activated protein kinase in STZ-induced type 2 diabetic mice,” PLoS One, vol. 8, no. 12, article e83397, 2013.
View at: Publisher Site | Google Scholar
L. Yu, B. Gong, W. Duan et al., “Melatonin ameliorates myocardial ischemia/reperfusion injury in type 1 diabetic rats by preserving mitochondrial function: role of AMPK-PGC-1alpha-SIRT3 signaling,” Scientific Reports, vol. 7, article 41337, 2017.
View at: Publisher Site | Google Scholar
C. L. Zhang, H. Feng, L. Li et al., “Globular CTRP3 promotes mitochondrial biogenesis in cardiomyocytes through AMPK/PGC-1alpha pathway,” Biochimica et Biophysica Acta (BBA) - General Subjects, vol. 1861, no. 1, Part A, pp. 3085–3094, 2017.
View at: Publisher Site | Google Scholar
D. Wan, Y. Zhou, K. Wang, Y. Hou, R. Hou, and X. Ye, “Resveratrol provides neuroprotection by inhibiting phosphodiesterases and regulating the cAMP/AMPK/SIRT1 pathway after stroke in rats,” Brain Research Bulletin, vol. 121, pp. 255–262, 2016.
View at: Publisher Site | Google Scholar
J. Li, X. Hu, P. Selvakumar et al., “Role of the nitric oxide pathway in AMPK-mediated glucose uptake and GLUT4 translocation in heart muscle,” American Journal of Physiology. Endocrinology and Metabolism, vol. 287, no. 5, pp. E834–E841, 2004.
View at: Google Scholar
L. Ji, X. Zhang, W. Liu et al., “AMPK-regulated and Akt-dependent enhancement of glucose uptake is essential in ischemic preconditioning-alleviated reperfusion injury,” PLoS One, vol. 8, no. 7, article e69910, 2013.
View at: Publisher Site | Google Scholar
H. Yuan, Y. Hu, Y. Zhu et al., “Metformin ameliorates high uric acid-induced insulin resistance in skeletal muscle cells,” Molecular and Cellular Endocrinology, vol. 443, pp. 138–145, 2017.
View at: Publisher Site | Google Scholar
G. R. Steinberg and B. E. Kemp, “AMPK in health and disease,” Physiological Reviews, vol. 89, no. 3, pp. 1025–1078, 2009.
View at: Publisher Site | Google Scholar
H. Motoshima, B. J. Goldstein, M. Igata, and E. Araki, “AMPK and cell proliferation—AMPK as a therapeutic target for atherosclerosis and cancer,” The Journal of Physiology, vol. 574, no. 1, pp. 63–71, 2006.
View at: Publisher Site | Google Scholar
R. Russell 3rd, “Stress signaling in the heart by AMP-activated protein kinase,” Current Hypertension Reports, vol. 8, no. 6, pp. 446–450, 2006.
View at: Publisher Site | Google Scholar
T. Yamauchi, J. Kamon, Y. Minokoshi et al., “Adiponectin stimulates glucose utilization and fatty-acid oxidation by activating AMP-activated protein kinase,” Nature Medicine, vol. 8, no. 11, pp. 1288–1295, 2002.
View at: Publisher Site | Google Scholar
J. Zhu, K. Z. Wang, and C. T. Chu, “After the banquet: mitochondrial biogenesis, mitophagy, and cell survival,” Autophagy, vol. 9, no. 11, pp. 1663–1676, 2013.
View at: Publisher Site | Google Scholar
M. M. Mihaylova and R. J. Shaw, “The AMPK signalling pathway coordinates cell growth, autophagy and metabolism,” Nature Cell Biology, vol. 13, no. 9, pp. 1016–1023, 2011.
View at: Publisher Site | Google Scholar
K. Marcinko and G. R. Steinberg, “The role of AMPK in controlling metabolism and mitochondrial biogenesis during exercise,” Experimental Physiology, vol. 99, no. 12, pp. 1581–1585, 2014.
View at: Publisher Site | Google Scholar
L. L. Dugan, Y. H. You, S. S. Ali et al., “AMPK dysregulation promotes diabetes-related reduction of superoxide and mitochondrial function,” The Journal of Clinical Investigation, vol. 123, no. 11, pp. 4888–4899, 2013.
View at: Publisher Site | Google Scholar
B. B. Kahn, T. Alquier, D. Carling, and D. G. Hardie, “AMP-activated protein kinase: ancient energy gauge provides clues to modern understanding of metabolism,” Cell Metabolism, vol. 1, no. 1, pp. 15–25, 2005.
View at: Publisher Site | Google Scholar
R. A. Merrill, R. K. Dagda, A. S. Dickey et al., “Mechanism of neuroprotective mitochondrial remodeling by PKA/AKAP1,” PLoS Biology, vol. 9, no. 4, article e1000612, 2011.
View at: Publisher Site | Google Scholar
E. Q. Toyama, S. Herzig, J. Courchet et al., “Metabolism. AMP-activated protein kinase mediates mitochondrial fission in response to energy stress,” Science, vol. 351, no. 6270, pp. 275–281, 2016.
View at: Publisher Site | Google Scholar
C. Kamga Pride, L. Mo, K. Quesnelle et al., “Nitrite activates protein kinase A in normoxia to mediate mitochondrial fusion and tolerance to ischaemia/reperfusion,” Cardiovascular Research, vol. 101, no. 1, pp. 57–68, 2014.
View at: Publisher Site | Google Scholar
A. Sarre, J. Gabrielli, G. Vial, X. M. Leverve, and F. Assimacopoulos-Jeannet, “Reactive oxygen species are produced at low glucose and contribute to the activation of AMPK in insulin-secreting cells,” Free Radical Biology & Medicine, vol. 52, no. 1, pp. 142–150, 2012.
View at: Publisher Site | Google Scholar
S. M. Shin, I. J. Cho, and S. G. Kim, “Resveratrol protects mitochondria against oxidative stress through AMP-activated protein kinase-mediated glycogen synthase kinase-3β inhibition downstream of poly(ADP-ribose)polymerase-LKB1 pathway,” Molecular Pharmacology, vol. 76, no. 4, pp. 884–895, 2009.
View at: Publisher Site | Google Scholar
K. Tao, N. Matsuki, and R. Koyama, “AMP-activated protein kinase mediates activity-dependent axon branching by recruiting mitochondria to axon,” Developmental Neurobiology, vol. 74, no. 6, pp. 557–573, 2014.
View at: Publisher Site | Google Scholar
D. F. Egan, D. B. Shackelford, M. M. Mihaylova et al., “Phosphorylation of ULK1 (hATG1) by AMP-activated protein kinase connects energy sensing to mitophagy,” Science, vol. 331, no. 6016, pp. 456–461, 2011.
View at: Publisher Site | Google Scholar
T. Kanki and D. J. Klionsky, “Mitophagy in yeast occurs through a selective mechanism,” The Journal of Biological Chemistry, vol. 283, no. 47, pp. 32386–32393, 2008.
View at: Publisher Site | Google Scholar
C. T. Chu, J. Ji, R. K. Dagda et al., “Cardiolipin externalization to the outer mitochondrial membrane acts as an elimination signal for mitophagy in neuronal cells,” Nature Cell Biology, vol. 15, no. 10, pp. 1197–1205, 2013.
View at: Publisher Site | Google Scholar
G. Twig and O. S. Shirihai, “The interplay between mitochondrial dynamics and mitophagy,” Antioxidants & Redox Signaling, vol. 14, no. 10, pp. 1939–1951, 2011.
View at: Publisher Site | Google Scholar
P. Mishra and D. C. Chan, “Mitochondrial dynamics and inheritance during cell division, development and disease,” Nature Reviews Molecular Cell Biology, vol. 15, no. 10, pp. 634–646, 2014.
View at: Publisher Site | Google Scholar
R. J. Youle and A. M. van der Bliek, “Mitochondrial fission, fusion, and stress,” Science, vol. 337, no. 6098, pp. 1062–1065, 2012.
View at: Publisher Site | Google Scholar
A. Li, S. Zhang, J. Li, K. Liu, F. Huang, and B. Liu, “Metformin and resveratrol inhibit Drp1-mediated mitochondrial fission and prevent ER stress-associated NLRP3 inflammasome activation in the adipose tissue of diabetic mice,” Molecular and Cellular Endocrinology, vol. 434, pp. 36–47, 2016.
View at: Publisher Site | Google Scholar
Q. Wang, M. Zhang, G. Torres et al., “Metformin suppresses diabetes-accelerated atherosclerosis via the inhibition of Drp1-mediated mitochondrial fission,” Diabetes, vol. 66, no. 1, pp. 193–205, 2017.
View at: Publisher Site | Google Scholar
J. Balog, S. L. Mehta, and R. Vemuganti, “Mitochondrial fission and fusion in secondary brain damage after CNS insults,” Journal of Cerebral Blood Flow and Metabolism: Official Journal of the International Society of Cerebral Blood Flow and Metabolism, vol. 36, no. 12, pp. 2022–2033, 2016.
View at: Publisher Site | Google Scholar
P. Mitchell, “Coupling of phosphorylation to electron and hydrogen transfer by a chemi-osmotic type of mechanism,” Nature, vol. 191, no. 4784, pp. 144–148, 1961.
View at: Publisher Site | Google Scholar
Y. R. Chen and J. L. Zweier, “Cardiac mitochondria and reactive oxygen species generation,” Circulation Research, vol. 114, no. 3, pp. 524–537, 2014.
View at: Publisher Site | Google Scholar
M. P. Murphy, “Understanding and preventing mitochondrial oxidative damage,” Biochemical Society Transactions, vol. 44, no. 5, pp. 1219–1226, 2016.
View at: Publisher Site | Google Scholar
H. Vakifahmetoglu-Norberg, A. T. Ouchida, and E. Norberg, “The role of mitochondria in metabolism and cell death,” Biochemical and Biophysical Research Communications, vol. 482, no. 3, pp. 426–431, 2017.
View at: Publisher Site | Google Scholar
R. J. Schauer, A. L. Gerbes, D. Vonier, M. op den Winkel, P. Fraunberger, and M. Bilzer, “Induction of cellular resistance against Kupffer cell-derived oxidant stress: a novel concept of hepatoprotection by ischemic preconditioning,” Hepatology, vol. 37, no. 2, pp. 286–295, 2003.
View at: Publisher Site | Google Scholar
R. R. Lamberts, G. Onderwater, N. Hamdani et al., “Reactive oxygen species-induced stimulation of 5'AMP-activated protein kinase mediates sevoflurane-induced cardioprotection,” Circulation, vol. 120, Supplement 1, no. 11, pp. S10–S15, 2009.
View at: Publisher Site | Google Scholar
L. A. Videla, V. Fernandez, P. Cornejo, and R. Vargas, “Metabolic basis for thyroid hormone liver preconditioning: upregulation of AMP-activated protein kinase signaling,” The Scientific World Journal, vol. 2012, Article ID 475675, 10 pages, 2012.
View at: Publisher Site | Google Scholar
S. Li, A. Hafeez, F. Noorulla et al., “Preconditioning in neuroprotection: from hypoxia to ischemia,” Progress in Neurobiology, vol. 157, pp. 79–91, 2017.
View at: Publisher Site | Google Scholar
Z. Jin, J. Wu, and L. J. Yan, “Chemical conditioning as an approach to ischemic stroke tolerance: mitochondria as the target,” International Journal of Molecular Sciences, vol. 17, no. 3, p. 351, 2016.
View at: Publisher Site | Google Scholar
C. H. Huang, C. Y. Chiang, R. H. Pen et al., “Hypothermia treatment preserves mitochondrial integrity and viability of cardiomyocytes after ischaemic reperfusion injury,” Injury, vol. 46, no. 2, pp. 233–239, 2015.
View at: Publisher Site | Google Scholar
L. A. Videla, V. Fernandez, P. Cornejo et al., “T₃-induced liver AMP-activated protein kinase signaling: redox dependency and upregulation of downstream targets,” World Journal of Gastroenterology, vol. 20, no. 46, pp. 17416–17425, 2014.
View at: Publisher Site | Google Scholar
S. Rohailla, N. Clarizia, M. Sourour et al., “Acute, delayed and chronic remote ischemic conditioning is associated with downregulation of mTOR and enhanced autophagy signaling,” PLoS One, vol. 9, no. 10, article e111291, 2014.
View at: Publisher Site | Google Scholar
C. Peralta, R. Bartrons, A. Serafin et al., “Adenosine monophosphate-activated protein kinase mediates the protective effects of ischemic preconditioning on hepatic ischemia-reperfusion injury in the rat,” Hepatology, vol. 34, no. 6, pp. 1164–1173, 2001.
View at: Publisher Site | Google Scholar
J. Lempiainen, P. Finckenberg, J. Levijoki, and E. Mervaala, “AMPK activator AICAR ameliorates ischaemia reperfusion injury in the rat kidney,” British Journal of Pharmacology, vol. 166, no. 6, pp. 1905–1915, 2012.
View at: Publisher Site | Google Scholar
A. Morrison and J. Li, “PPAR-γ and AMPK—advantageous targets for myocardial ischemia/reperfusion therapy,” Biochemical Pharmacology, vol. 82, no. 3, pp. 195–200, 2011.
View at: Publisher Site | Google Scholar
J. Li, S. E. Benashski, V. R. Venna, and L. D. McCullough, “Effects of metformin in experimental stroke,” Stroke, vol. 41, no. 11, pp. 2645–2652, 2010.
View at: Publisher Site | Google Scholar
X. Zhang, R. Gao, J. Li et al., “A pharmacological activator of AMP-activated protein kinase protects hypoxic neurons in a concentration-dependent manner,” Neurochemical Research, vol. 35, no. 8, pp. 1281–1289, 2010.
View at: Publisher Site | Google Scholar
V. R. Venna, J. Li, S. E. Benashski, S. Tarabishy, and L. D. McCullough, “Preconditioning induces sustained neuroprotection by downregulation of adenosine 5′-monophosphate-activated protein kinase,” Neuroscience, vol. 201, pp. 280–287, 2012.
View at: Publisher Site | Google Scholar
C. P. Chih and E. L. Roberts Jr., “Energy substrates for neurons during neural activity: a critical review of the astrocyte-neuron lactate shuttle hypothesis,” Journal of Cerebral Blood Flow and Metabolism, vol. 23, no. 11, pp. 1263–1281, 2003.
View at: Publisher Site | Google Scholar
A. Almeida, S. Moncada, and J. P. Bolanos, “Nitric oxide switches on glycolysis through the AMP protein kinase and 6-phosphofructo-2-kinase pathway,” Nature Cell Biology, vol. 6, no. 1, pp. 45–51, 2004.
View at: Publisher Site | Google Scholar
A. S. Marsin, L. Bertrand, M. H. Rider et al., “Phosphorylation and activation of heart PFK-2 by AMPK has a role in the stimulation of glycolysis during ischaemia,” Current Biology, vol. 10, no. 20, pp. 1247–1255, 2000.
View at: Publisher Site | Google Scholar
J. Li and L. D. McCullough, “Effects of AMP-activated protein kinase in cerebral ischemia,” Journal of Cerebral Blood Flow and Metabolism, vol. 30, no. 3, pp. 480–492, 2010.
View at: Publisher Site | Google Scholar
P. Wang, T. Y. Xu, Y. F. Guan et al., “Nicotinamide phosphoribosyltransferase protects against ischemic stroke through SIRT1-dependent adenosine monophosphate-activated kinase pathway,” Annals of Neurology, vol. 69, no. 2, pp. 360–374, 2011.
View at: Publisher Site | Google Scholar
J. Li, Z. Zeng, B. Viollet, G. V. Ronnett, and L. D. McCullough, “Neuroprotective effects of adenosine monophosphate-activated protein kinase inhibition and gene deletion in stroke,” Stroke, vol. 38, no. 11, pp. 2992–2999, 2007.
View at: Publisher Site | Google Scholar
P. Shen, S. Hou, M. Zhu, M. Zhao, Y. Ouyang, and J. Feng, “Cortical spreading depression preconditioning mediates neuroprotection against ischemic stroke by inducing AMP-activated protein kinase-dependent autophagy in a rat cerebral ischemic/reperfusion injury model,” Journal of Neurochemistry, vol. 140, no. 5, pp. 799–813, 2017.
View at: Publisher Site | Google Scholar
E. Viggiano, D. Viggiano, A. Viggiano, B. De Luca, and M. Monda, “Cortical spreading depression increases the phosphorylation of AMP-activated protein kinase in the cerebral cortex,” Neurochemical Research, vol. 39, no. 12, pp. 2431–2439, 2014.
View at: Publisher Site | Google Scholar
D. Qi and L. H. Young, “AMPK: energy sensor and survival mechanism in the ischemic heart,” Trends in Endocrinology and Metabolism, vol. 26, no. 8, pp. 422–429, 2015.
View at: Publisher Site | Google Scholar
C. Liu, B. Liang, Q. Wang, J. Wu, and M. H. Zou, “Activation of AMP-activated protein kinase alpha1 alleviates endothelial cell apoptosis by increasing the expression of anti-apoptotic proteins Bcl-2 and survivin,” The Journal of Biological Chemistry, vol. 285, no. 20, pp. 15346–15355, 2010.
View at: Publisher Site | Google Scholar
P. Weisova, C. G. Concannon, M. Devocelle, J. H. Prehn, and M. W. Ward, “Regulation of glucose transporter 3 surface expression by the AMP-activated protein kinase mediates tolerance to glutamate excitation in neurons,” The Journal of Neuroscience, vol. 29, no. 9, pp. 2997–3008, 2009.
View at: Publisher Site | Google Scholar
P. Weisova, U. Anilkumar, C. Ryan, C. G. Concannon, J. H. Prehn, and M. W. Ward, “‘Mild mitochondrial uncoupling’ induced protection against neuronal excitotoxicity requires AMPK activity,” Biochimica et Biophysica Acta (BBA) - Bioenergetics, vol. 1817, no. 5, pp. 744–753, 2012.
View at: Publisher Site | Google Scholar
A. Atlante, S. Gagliardi, G. M. Minervini, E. Marra, S. Passarella, and P. Calissano, “Rapid uncoupling of oxidative phosphorylation accompanies glutamate toxicity in rat cerebellar granule cells,” Neuroreport, vol. 7, no. 15, pp. 2519–2524, 1996.
View at: Publisher Site | Google Scholar
X. Y. Zhang, T. T. Zhang, D. D. Song et al., “Endoplasmic reticulum chaperone GRP78 is involved in autophagy activation induced by ischemic preconditioning in neural cells,” Molecular Brain, vol. 8, no. 1, p. 20, 2015.
View at: Publisher Site | Google Scholar
M. W. Ward, H. J. Huber, P. Weisova, H. Dussmann, D. G. Nicholls, and J. H. Prehn, “Mitochondrial and plasma membrane potential of cultured cerebellar neurons during glutamate-induced necrosis, apoptosis, and tolerance,” The Journal of Neuroscience, vol. 27, no. 31, pp. 8238–8249, 2007.
View at: Publisher Site | Google Scholar
R. A. Merrill and S. Strack, “Mitochondria: a kinase anchoring protein 1, a signaling platform for mitochondrial form and function,” The International Journal of Biochemistry & Cell Biology, vol. 48, pp. 92–96, 2014.
View at: Publisher Site | Google Scholar
R. K. Dagda and T. Das Banerjee, “Role of protein kinase A in regulating mitochondrial function and neuronal development: implications to neurodegenerative diseases,” Reviews in the Neurosciences, vol. 26, no. 3, pp. 359–370, 2015.
View at: Publisher Site | Google Scholar
R. K. Dagda, A. M. Gusdon, I. Pien et al., “Mitochondrially localized PKA reverses mitochondrial pathology and dysfunction in a cellular model of Parkinson’s disease,” Cell Death and Differentiation, vol. 18, no. 12, pp. 1914–1923, 2011.
View at: Publisher Site | Google Scholar
N. J. Hoffman, B. L. Parker, R. Chaudhuri et al., “Global phosphoproteomic analysis of human skeletal muscle reveals a network of exercise-regulated kinases and AMPK substrates,” Cell Metabolism, vol. 22, no. 5, pp. 922–935, 2015.
View at: Publisher Site | Google Scholar
K. R. Pryde, H. L. Smith, K. Y. Chau, and A. H. Schapira, “PINK1 disables the anti-fission machinery to segregate damaged mitochondria for mitophagy,” The Journal of Cell Biology, vol. 213, no. 2, pp. 163–171, 2016.
View at: Publisher Site | Google Scholar
J. Li, Y. Wang, Y. Wang et al., “Pharmacological activation of AMPK prevents Drp1-mediated mitochondrial fission and alleviates endoplasmic reticulum stress-associated endothelial dysfunction,” Journal of Molecular and Cellular Cardiology, vol. 86, pp. 62–74, 2015.
View at: Publisher Site | Google Scholar
J. D. Stone, A. Narine, and D. A. Tulis, “Inhibition of vascular smooth muscle growth via signaling crosstalk between AMP-activated protein kinase and cAMP-dependent protein kinase,” Frontiers in Physiology, vol. 3, p. 409, 2012.
View at: Publisher Site | Google Scholar
A. Carlucci, A. Adornetto, A. Scorziello et al., “Proteolysis of AKAP121 regulates mitochondrial activity during cellular hypoxia and brain ischaemia,” The EMBO Journal, vol. 27, no. 7, pp. 1073–1084, 2008.
View at: Publisher Site | Google Scholar
G. G. Schiattarella, F. Cattaneo, G. Pironti et al., “Akap1 deficiency promotes mitochondrial aberrations and exacerbates cardiac injury following permanent coronary ligation via enhanced mitophagy and apoptosis,” PLoS One, vol. 11, no. 5, article e0154076, 2016.
View at: Publisher Site | Google Scholar
C. Perrino, A. Feliciello, G. G. Schiattarella et al., “AKAP121 downregulation impairs protective cAMP signals, promotes mitochondrial dysfunction, and increases oxidative stress,” Cardiovascular Research, vol. 88, no. 1, pp. 101–110, 2010.
View at: Publisher Site | Google Scholar
Q. Li, N. Li, H. H. Cui et al., “Tongxinluo exerts protective effects via anti-apoptotic and pro-autophagic mechanisms by activating AMPK pathway in infarcted rat hearts,” Experimental Physiology, vol. 102, no. 4, pp. 422–435, 2017.
View at: Publisher Site | Google Scholar
C. Zeng, H. Li, Z. Fan et al., “Crocin-elicited autophagy rescues myocardial ischemia/reperfusion injury via paradoxical mechanisms,” The American Journal of Chinese Medicine, vol. 44, no. 03, pp. 515–530, 2016.
View at: Publisher Site | Google Scholar
Y. Matsui, H. Takagi, X. Qu et al., “Distinct roles of autophagy in the heart during ischemia and reperfusion: roles of AMP-activated protein kinase and Beclin 1 in mediating autophagy,” Circulation Research, vol. 100, no. 6, pp. 914–922, 2007.
View at: Publisher Site | Google Scholar
F. Distelmaier, F. Valsecchi, D. C. Liemburg-Apers et al., “Mitochondrial dysfunction in primary human fibroblasts triggers an adaptive cell survival program that requires AMPK-alpha,” Biochimica et Biophysica Acta (BBA) - Molecular Basis of Disease, vol. 1852, no. 3, pp. 529–540, 2015.
View at: Publisher Site | Google Scholar
L. R. Edmunds, L. Sharma, H. Wang et al., “c-Myc and AMPK control cellular energy levels by cooperatively regulating mitochondrial structure and function,” PLoS One, vol. 10, no. 7, article e0134049, 2015.
View at: Publisher Site | Google Scholar
M. Brownlee, “Biochemistry and molecular cell biology of diabetic complications,” Nature, vol. 414, no. 6865, pp. 813–820, 2001.
View at: Publisher Site | Google Scholar
S. W. Kang, G. Haydar, C. Taniane et al., “AMPK activation prevents and reverses drug-induced mitochondrial and hepatocyte injury by promoting mitochondrial fusion and function,” PLoS One, vol. 11, no. 10, article e0165638, 2016.
View at: Publisher Site | Google Scholar
S. Rodriguez-Cuenca, S. Carobbio, V. R. Velagapudi et al., “Peroxisome proliferator-activated receptor γ-dependent regulation of lipolytic nodes and metabolic flexibility,” Molecular and Cellular Biology, vol. 32, no. 8, pp. 1555–1565, 2012.
View at: Publisher Site | Google Scholar
M. P. Marrades, P. Gonzalez-Muniesa, J. A. Martinez, and M. J. Moreno-Aliaga, “A dysregulation in CES1, APOE and other lipid metabolism-related genes is associated to cardiovascular risk factors linked to obesity,” Obesity Facts, vol. 3, no. 5, pp. 312–318, 2010.
View at: Publisher Site | Google Scholar
H. C. Gerstein, M. E. Miller, R. P. Byington et al., “Effects of intensive glucose lowering in type 2 diabetes,” The New England Journal of Medicine, vol. 358, no. 24, pp. 2545–2559, 2008.
View at: Publisher Site | Google Scholar
M. A. Ewart and S. Kennedy, “Diabetic cardiovascular disease—AMP-activated protein kinase (AMPK) as a therapeutic target,” Cardiovascular & Hematological Agents in Medicinal Chemistry, vol. 10, no. 3, pp. 190–211, 2012.
View at: Publisher Site | Google Scholar
S. A. Hawley, A. E. Gadalla, O. G. Skytte, and D. G. Hardie, “The antidiabetic drug metformin activates the AMP-activated protein kinase cascade via an adenine nucleotide-independent mechanism,” Diabetes, vol. 51, no. 8, pp. 2420–2425, 2002.
View at: Publisher Site | Google Scholar
G. Ceolotto, A. Gallo, I. Papparella et al., “Rosiglitazone reduces glucose-induced oxidative stress mediated by NAD(P)H oxidase via AMPK-dependent mechanism,” Arteriosclerosis, Thrombosis, and Vascular Biology, vol. 27, no. 12, pp. 2627–2633, 2007.
View at: Publisher Site | Google Scholar
J. G. Boyle, P. J. Logan, M. A. Ewart et al., “Rosiglitazone stimulates nitric oxide synthesis in human aortic endothelial cells via AMP-activated protein kinase,” The Journal of Biological Chemistry, vol. 283, no. 17, pp. 11210–11217, 2008.
View at: Publisher Site | Google Scholar
W. Sun, T. S. Lee, M. Zhu et al., “Statins activate AMP-activated protein kinase in vitro and in vivo,” Circulation, vol. 114, no. 24, pp. 2655–2662, 2006.
View at: Publisher Site | Google Scholar
J. E. Kim, J. Y. Sung, C. H. Woo et al., “Cilostazol inhibits vascular smooth muscle cell proliferation and reactive oxygen species production through activation of AMP-activated protein kinase induced by heme oxygenase-1,” The Korean Journal of Physiology & Pharmacology, vol. 15, no. 4, pp. 203–210, 2011.
View at: Publisher Site | Google Scholar
K. Suzuki, K. Uchida, N. Nakanishi, and Y. Hattori, “Cilostazol activates AMP-activated protein kinase and restores endothelial function in diabetes,” American Journal of Hypertension, vol. 21, no. 4, pp. 451–457, 2008.
View at: Publisher Site | Google Scholar
A. Elezaby, A. L. Sverdlov, V. H. Tu et al., “Mitochondrial remodeling in mice with cardiomyocyte-specific lipid overload,” Journal of Molecular and Cellular Cardiology, vol. 79, pp. 275–283, 2015.
View at: Publisher Site | Google Scholar
H. Takagi, Y. Matsui, S. Hirotani, H. Sakoda, T. Asano, and J. Sadoshima, “AMPK mediates autophagy during myocardial ischemia in vivo,” Autophagy, vol. 3, no. 4, pp. 405–407, 2007.
View at: Publisher Site | Google Scholar
M. Hu, P. Ye, H. Liao, M. Chen, and F. Yang, “Metformin protects H9C2 cardiomyocytes from high-glucose and hypoxia/reoxygenation injury via inhibition of reactive oxygen species generation and inflammatory responses: role of AMPK and JNK,” Journal of Diabetes Research, vol. 2016, Article ID 2961954, 9 pages, 2016.
View at: Publisher Site | Google Scholar
J. T. Hwang, D. Y. Kwon, O. J. Park, and M. S. Kim, “Resveratrol protects ROS-induced cell death by activating AMPK in H9c2 cardiac muscle cells,” Genes & Nutrition, vol. 2, no. 4, pp. 323–326, 2008.
View at: Publisher Site | Google Scholar
L. Fu, L. Huang, C. Cao, Q. Yin, and J. Liu, “Inhibition of AMP-activated protein kinase alleviates focal cerebral ischemia injury in mice: interference with mTOR and autophagy,” Brain Research, vol. 1650, pp. 103–111, 2016.
View at: Publisher Site | Google Scholar
H. Kim, M. C. Scimia, D. Wilkinson et al., “Fine-tuning of Drp1/Fis1 availability by AKAP121/Siah2 regulates mitochondrial adaptation to hypoxia,” Molecular Cell, vol. 44, no. 4, pp. 532–544, 2011.
View at: Publisher Site | Google Scholar
A. Feliciello, C. S. Rubin, E. V. Avvedimento, and M. E. Gottesman, “Expression of a kinase anchor protein 121 is regulated by hormones in thyroid and testicular germ cells,” The Journal of Biological Chemistry, vol. 273, no. 36, pp. 23361–23366, 1998.
View at: Publisher Site | Google Scholar
W. F. Lubbe, T. Podzuweit, and L. H. Opie, “Potential arrhythmogenic role of cyclic adenosine monophosphate (AMP) and cytosolic calcium overload: implications for prophylactic effects of beta-blockers in myocardial infarction and proarrhythmic effects of phosphodiesterase inhibitors,” Journal of the American College of Cardiology, vol. 19, no. 7, pp. 1622–1633, 1992.
View at: Publisher Site | Google Scholar
Y. Wang and J. I. Goldhaber, “Return of calcium: manipulating intracellular calcium to prevent cardiac pathologies,” Proceedings of the National Academy of Sciences of the United States of America, vol. 101, no. 16, pp. 5697-5698, 2004.
View at: Publisher Site | Google Scholar
S. Makaula, A. Lochner, S. Genade, M. N. Sack, M. M. Awan, and L. H. Opie, “H-89, a non-specific inhibitor of protein kinase A, promotes post-ischemic cardiac contractile recovery and reduces infarct size,” Journal of Cardiovascular Pharmacology, vol. 45, no. 4, pp. 341–347, 2005.
View at: Publisher Site | Google Scholar
K. Tanaka, Y. Fukuuchi, H. Nozaki, E. Nagata, T. Kondo, and T. Dembo, “Acute ischemic vulnerability of PKA in the dendritic subfields of the hippocampus CA1,” Neuroreport, vol. 8, no. 11, pp. 2423–2428, 1997.
View at: Publisher Site | Google Scholar
K. Tanaka, “Alteration of second messengers during acute cerebral ischemia - adenylate cyclase, cyclic AMP-dependent protein kinase, and cyclic AMP response element binding protein,” Progress in Neurobiology, vol. 65, no. 2, pp. 173–207, 2001.
View at: Publisher Site | Google Scholar
K. Tanaka, D. Ito, S. Suzuki, T. Dembo, A. Kosakai, and Y. Fukuuchi, “A novel voltage-sensitive Na⁺ and Ca²⁺ channel blocker, NS-7, prevents suppression of cyclic AMP-dependent protein kinase and reduces infarct area in the acute phase of cerebral ischemia in rat,” Brain Research, vol. 924, no. 1, pp. 98–108, 2002.
View at: Publisher Site | Google Scholar
J. Ke, Y. Liu, J. Yang et al., “Synergistic effects of metformin with liraglutide against endothelial dysfunction through GLP-1 receptor and PKA signalling pathway,” Scientific Reports, vol. 7, article 41085, 2017.
View at: Publisher Site | Google Scholar
L. He, E. Chang, J. Peng et al., “Activation of the cAMP-PKA pathway antagonizes metformin suppression of hepatic glucose production,” The Journal of Biological Chemistry, vol. 291, no. 20, pp. 10562–10570, 2016.
View at: Publisher Site | Google Scholar
D. K. Aw, R. A. Sinha, S. Y. Xie, and P. M. Yen, “Differential AMPK phosphorylation by glucagon and metformin regulates insulin signaling in human hepatic cells,” Biochemical and Biophysical Research Communications, vol. 447, no. 4, pp. 569–573, 2014.
View at: Publisher Site | Google Scholar

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Copyright © 2017 Jingdian Zhang et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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