doi: 10.1161/CIRCULATIONAHA.105.554360
(Circulation. 2005;112:2686-2695.)
© 2005 American Heart Association, Inc.
Molecular Cardiology |
Reduced Mitochondrial Oxidative Capacity and Increased Mitochondrial Uncoupling Impair Myocardial Energetics in Obesity
From the Division of Endocrinology, Metabolism and Diabetes and Program in Human Molecular Biology and Genetics (S.B., S.S., B.T.O., P.T., E.D.A.), University of Utah School of Medicine, Salt Lake City, Utah, and USDA/ARS Children’s Nutrition Research Center and Department of Pediatrics (M.E.Y.), Baylor College of Medicine, Houston, Tex.
Correspondence to E. Dale Abel, MB,BS, DPhil, Division of Endocrinology, Metabolism and Diabetes, Program in Human Molecular Biology & Genetics, 15 N 2030 E, Bldg 533, Room 3410B, Salt Lake City, UT 84112. E-mail dale.abel{at}hmbg.utah.edu
Received April 6, 2005; revision received July 19, 2005; accepted August 8, 2005.
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Abstract |
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Background— Obesity is a risk factor for cardiovascular disease and is strongly associated with insulin resistance and type 2 diabetes. Recent studies in obese humans and animals demonstrated increased myocardial oxygen consumption (M
O2) and reduced cardiac efficiency (CE); however, the underlying mechanisms remain unclear. The present study was performed to determine whether mitochondrial dysfunction and uncoupling are responsible for reduced cardiac performance and efficiency in ob/ob mice.
Methods and Results— Cardiac function, MO2, mitochondrial respiration, and ATP synthesis were measured in 9-week-old ob/ob and control mouse hearts. Contractile function and MO2 in glucose-perfused ob/ob hearts were similar to controls under basal conditions but were reduced under high workload. Perfusion of ob/ob hearts with glucose and palmitate increased MO2 and reduced CE by 23% under basal conditions, and CE remained impaired at high workload. In glucose-perfused ob/ob hearts, mitochondrial state 3 respirations were reduced but ATP/O ratios were unchanged. In contrast, state 3 respiration rates were similar in ob/ob and control mitochondria from hearts perfused with palmitate and glucose, but ATP synthesis rates and ATP/O ratios were significantly reduced in ob/ob, which suggests increased mitochondrial uncoupling. Pyruvate dehydrogenase activity and protein levels of complexes I, III, and V were reduced in obese mice.
Conclusions— These data indicate that reduced mitochondrial oxidative capacity may contribute to cardiac dysfunction in ob/ob mice. Moreover, fatty acid but not glucose-induced mitochondrial uncoupling reduces CE in obese mice by limiting ATP production and increasing MO2.
Key Words: obesity • metabolism • energetics • fatty acids • mitochondria
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Introduction |
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The prevalence of obesity is increasing in the United States, with approximately one third of the adult population being reported as obese.1 Obesity is an independent risk factor for the development of heart failure. It has been proposed that a mismatch between fatty acid (FA) uptake and FA oxidation may result in intramyocardial accumulation of lipids. This may induce lipotoxic injury and cardiac dysfunction via a number of mechanisms, including ceramide-activated apoptosis.2 Moreover, an association between increased lipid accumulation and diastolic dysfunction (with preserved systolic function) has been reported in hearts isolated from ob/ob mice, which are a model of severe obesity,3 and myocardial lipid accumulation has been associated with left ventricular hypertrophy and impaired septal contractility in humans with obesity.4
Clinical Perspective p 2695
Obesity and insulin resistance in both humans and animals alter cardiac metabolism by increasing cardiac FA oxidation and myocardial oxygen consumption (MO2), thereby reducing cardiac efficiency (CE).5,6 This metabolic shift toward FA utilization has been proposed to contribute to the development of left ventricular dysfunction. Indeed, normalization of cardiac metabolism by overexpressing a human GLUT4 transgene in db/db mice (an animal model of obesity and diabetes) reversed cardiac dysfunction, which suggests that altered myocardial metabolism contributed to contractile dysfunction in this model.7,8 The mechanisms responsible for increased FA oxidation and reduced CE in the hearts of obese humans and animals await complete elucidation. Moreover, normalization of myocardial substrate metabolism by treatment of db/db mice with peroxisome proliferator-activated receptor (PPAR)-
and -
agonists failed to restore cardiac function.9,10 Thus, additional defects are likely to persist in the hearts of genetically obese and diabetic mice that cannot be reversed by short-term normalization of systemic metabolic abnormalities.
A potential mechanism for increased oxygen consumption and increased FA utilization in the hearts of obese animals is mitochondrial uncoupling. Although streptozotocin diabetes has been shown to be associated with increased expression of uncoupling protein-3 (UCP3) mRNA in the heart,11 no studies have directly evaluated whether mitochondrial uncoupling directly contributes to myocardial dysfunction in either diabetes or obesity. Second, increased FA concentrations have been associated with increased expression of UCP3 in skeletal muscle and cardiac muscle,12,13 but whether or not increased FA delivery uncouples mitochondria in the heart in obesity remains to be established definitively.
The present studies were undertaken to test the hypothesis that abnormal substrate metabolism and contractile dysfunction in the hearts of obese mice are associated with or result from impaired mitochondrial energetics. We demonstrate that multiple mitochondrial defects impair ATP generation in the hearts of obese animals, and mitochondrial energetics is further impaired by FA-induced uncoupling.
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Methods |
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Animals
Nine week-old male ob/ob mice on the C57BL/6J background and their lean C57BL/6J controls were obtained from the Jackson Laboratory (Bar Harbor, Maine). Mice were housed in conventional cages and maintained with a 12-hour light/12-hour dark photoperiod in humidity- and temperature-controlled rooms with free access to water and food. Experimental procedures in animals were performed in accordance with protocols approved by the Institutional Animal Care and Use Committee of the University of Utah.
Heart Perfusion
Mice were anesthetized by intraperitoneal injection of 15 mg of chloral hydrate, and the heart was rapidly excised and arrested in ice-cold buffer. The aorta was then cannulated and retrogradely perfused at constant pressure of 60 mm Hg with 37°C Krebs buffer containing (in mmol/L) NaCl 118, KCl 4.7, NaHCO3 25, MgSO4 1.2, KH2PO4 1.2, and CaCl2 2 gassed with 95% O2 and 5% CO2. Hearts were perfused with either 11 mmol/L glucose alone or combined with 1 mmol/L palmitate that was prebound to 3% BSA. Left ventricular pressure was monitored from a water-filled balloon placed through the left atrial appendage and connected to a Millar transducer (Millar Instruments). The balloon was inflated to achieve an end-diastolic pressure of 7 to 10 mm Hg. Heart rates were maintained at 360 bpm by pacing at 6 Hz at the level of the atria.
Myocardial Oxygen Consumption
Oxygen consumption was calculated from the difference in oxygen content of incoming (aortic) and outgoing (pulmonary artery) perfusate with the formula: MO2=% O2 perfusate–% O2 pulmonary arteryxcoronary flowxatmospheric pressure/760xO2 solubilityxO2 density, where O2 solubility=23.9 µL/mL and O2 density=0.03933 µmol/µL, respectively, at 37°C.
Calcium-Induced Inotropic Protocol
Hearts were allowed to stabilize for 30 minutes before acquisition of hemodynamic parameters and MO2 at baseline (2 mmol/L calcium concentration). The calcium content of the perfusate was then increased from 2 to 4 mmol/L, and contractile parameters and MO2 were measured after 20 minutes of stabilization. These studies were performed in hearts that were perfused either with glucose as sole substrate or in hearts perfused with glucose and palmitate.
Saponin-Permeabilized Fibers
Respiratory parameters of the total mitochondrial population were studied in situ in fresh saponin-permeabilized fibers as described previously.14 Briefly, small pieces (2 to 5 mg) of cardiac muscle were taken from the left ventricle and permeabilized with 50 µg/mL saponin at 4°C in buffer A containing (in mmol/L) K2EGTA 7.23, K2CaEGTA 2.77, MgCl2 6.56, imidazole 20, dithiothreitol 0.5, K-methanS 53.3, taurine 20, Na2ATP 5.3, PCr 15, and KH2PO4 3, pH 7.1 adjusted at 25°C. The fibers were then washed twice for 10 minutes in buffer B containing (in mmol/L) K2EGTA 7.23, K2CaEGTA 2.77, MgCl2 1.38, imidazole 20, dithiothreitol 0.5, K-methanS 100, taurine 20, KH2PO4 3, and BSA 2 mg/mL, pH 7.1 at 25°C.
Respiration and ATP Measurements
The respiratory rates of saponin-permeabilized fibers were determined with the same oxygen sensor probe used for the MO2 measurements in 2 mL of buffer B at 25°C with continuous stirring. Studies were performed with 3 independent substrates (in mmol/L): (1) glutamate 5 and malate 2, (2) pyruvate 10 and malate 5, or (3) palmitoyl-carnitine 0.02 and malate 2. The solubility of oxygen in buffer B is 215 nmol of O2 per mL at 25°C. Oxygen consumption rates were expressed as nmol of O2 · min–1 · mg dry fiber weight–1. Respiratory parameters were defined as follows. Basal respiration rates before the addition of ADP (V0) were defined at state 2. Maximally ADP (1 mmol/L)–stimulated respiration rates (VADP) were defined as state 3, and respiration rates in the absence of ADP phosphorylation and measured in the presence of 1 µg/mL oligomycin (Voligomycin) were termed state 4. This nomenclature has been used in prior studies15–17 but differs from other studies in which state 4 respirations were measured either in the absence of added ADP or after a period of time during which ADP was believed to be depleted. ATP concentration was determined by a bioluminescence assay based on the luciferin/luciferase reaction with the ATP assay kit (ThermoLabsystems).
Determination of Mitochondrial Enzyme Activities
Total carnitine palmitoyl-transferase (CPT; CPT 1+CPT 2) activity was measured in mitochondria that were isolated as described previously.18 Mitochondria (&200 µg) were assayed in 1 mL of reaction buffer containing (in mmol/L) HEPES 20, EGTA 1, sucrose 220, KCl 40, 5,5'-dithio-bis (2-nitrobenzoic acid) (DTNB) 0.1, BSA 1.3 mg/mL, and palmitoyl-CoA 40 µmol/L, pH 7.4 at 25°C. The reaction was started by adding 1 mmol/L carnitine and was monitored at 412 nm for 4 minutes with an Ultrospec 3000 spectrophotometer. CPT 2 activity was measured with the same reaction as total CPT but after addition of malonyl-CoA (10 µmol/L), which completely inhibits CPT 1 activity. CPT 1 activity was calculated by subtracting CPT 2 activity from total CPT activity. Citrate synthase (CS) activity was assessed in frozen cardiac tissue (&10 mg). Hearts were homogenized on ice in 20% (wt/vol) homogenization buffer containing (in mmol/L) HEPES 20, EDTA 10, pH 7.4. The homogenates were then frozen for 1 hour to liberate CS from mitochondrial matrix and were then diluted 1:10. The reaction was performed in 1 mL of reaction buffer containing (in mmol/L) HEPES 20, EGTA 1, sucrose 220, KCl 40, DTNB 0.1, and acetyl-CoA 0.1, pH 7.4 at 25°C, and was started by the addition of 0.05 mmol/L oxaloacetate and finally monitored at 412 nm for 3 minutes with an Ultrospec 3000 spectrophotometer. ß-Hydroxyacyl-CoA dehydrogenase activity was measured in the same homogenate as used for CS assay but diluted 1:4. The reaction was performed in 1 mL of reaction buffer containing (in mmol/L) HEPES 20, EGTA 1, KCN 1, and NADH 0.15, pH 7.4 at 25°C. The reaction was started by the addition of 0.1 mmol/L acetoacetyl-CoA and monitored at 340 nm for 4 minutes with an Ultrospec 3000 spectrophotometer. Pyruvate dehydrogenase (PDH) activity was assayed as described before19 with a radioactive-enzymatic method. Frozen heart tissue was homogenized in a buffer containing (in mmol/L) HEPES 25 (pH 7.4), EDTA 3, sodium dichloroacetate 5, N--tosyl-L-lysylchloromethane 1, ADP 1, dithiothreitol 5, CaCl2 2, MgCl2 5, and potassium fluoride (KF) 25, supplemented with 1.5% Triton X-100 and 5 µmol/L leupeptin. For determination of the total fraction of the PDH (PDHt), the HEPES concentration was increased to 75 mmol/L and the KF was omitted from the homogenization buffer to allow for PDH dephosphorylation by endogenous PDH phosphatases. Total and active PDH were determined in a reaction mixture containing (in mmol/L) HEPES 50 (pH 7.4), thiamine pyrophosphate 0.4, coenzyme A 0.4, dithiothreitol 2, NAD+ 5, and MgCl2 5, supplemented with 0.17% Triton X-100, 5 U/mL dihydrolipoamide reductase (E3), 20 µL of homogenate, and 2 µCi [1-14C]-pyruvate. The PDH reaction yielding acetyl-CoA + CO2 was performed at 30°C for 7 minutes before termination of the reaction by addition of 2 mol/L acetic acid in 2% sodium dodecylsulfate (SDS). The 14CO2 released from the PDH reaction was quantified with a scintillation counter (Beckman Coulter Inc). The activity of PDH is expressed as the total and active forms, with the percentage of active PDH calculated with the following formula: (active form/total activity)x100. PDH activity was expressed as nmol · min–1 · mg tissue–1.
Western Blot Analysis
Total proteins were extracted from frozen hearts that were initially pulverized under liquid nitrogen and then homogenized with a Polytron in sample buffer containing (in mmol/L) HEPES 30, pH7.4, sodium pyrophosphate 50, sodium fluoride 100, EDTA 1, and sodium orthovanadate 10 supplemented with 1% Triton X-100 and protease inhibitor cocktail (Roche Diagnostics). Samples were then centrifuged for 15 minutes at 9000 rpm at 4°C. The supernatant was collected and centrifuged for 1 hour at 4°C at 47 000 rpm. For mitochondrial proteins, hearts were removed and homogenized in 1 mL of ice-cold mitochondrial buffer containing (in mmol/L) HEPES 20 (pH7.4), KCl 140, EDTA 10, and MgCl2 5 with a tight-fitting Teflon-glass homogenizer (10 to 15 seconds). The homogenate was centrifuged for 10 minutes at 700g at 4°C. The corresponding supernatant was centrifuged for 10 minutes at 8000g at 4°C. The mitochondrial pellets were then suspended in 50 µL of sample buffer. Protein concentration was measured with Micro BCA reagent (Pierce). Protein extracts were resolved by SDS-PAGE and electrotransferred onto a PVDF membrane (Millipore). Membranes were probed with the appropriate primary antibody. The following antibodies were used: rabbit anti-UCP3 (1/500, Affinity Bioreagents, Golden, Colo), goat anti-UCP2 (1/100, Chemicon International, Temecula, Calif), mouse anti-OxPhos complex II (iron-sulfur protein; 1/1000), mouse anti-OxPhos complex III (core I; 1/1000), mouse anti-OxPhos complex I (-subcomplex 9; 1/1000), and mouse anti-OxPhos complex V (F1 complex, -subunit; 1/1000; Molecular Probes–Invitrogen, Carlsbad, Calif). For loading control, mouse anti- tubulin (1/2000, Sigma, Saint Louis, Mo) was used for total heart proteins, and Coomassie blue R-250 (BioRad) staining was performed for mitochondrial proteins. Protein detection was performed with the appropriate horseradish peroxidase–conjugated secondary antibody and ECL or ECL Plus detection systems (Amersham Biosciences).
Statistical Analysis
Data are presented as mean±SE. Significance (P<0.05) was determined by ANOVA followed by Fisher’s least protected squares test. Statistical calculations were performed with the Statview 5.0.1 software package (SAS Institute).
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Results |
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As previously described, body weights were increased in ob/ob mice (50.62±0.92 versus 23.09±0.37 g; P<0.00001). We have also reported previously that these mice are hyperinsulinemic and exhibit impaired glucose tolerance but are not diabetic.6 Wet and dry heart weights were 13% and 20% (P<0.001) higher in ob/ob mice than in wild-type controls, which is consistent with previous reports of cardiac hypertrophy in these mice. We hypothesized that FA specifically contributes to changes in the bioenergetics and oxygen consumption in ob/ob hearts and mitochondria. We therefore initially determined cardiac performance and M
O2, as well as mitochondrial function, in the absence of FA by examining these parameters in hearts perfused with glucose as sole substrate. Subsequent analysis after perfusion of hearts with glucose plus palmitate then allowed us to ascertain the specific additive effects of FA exposure.
Cardiac Function in Glucose-Perfused Hearts
Basal cardiac function was similar in ob/ob and controls perfused with glucose only (Table 1). The relationship between MO2 and rate pressure product (RPP) was then investigated at different workload conditions. Increasing calcium in the perfusate caused a 2.2-, 2.1-, and 1.9-fold increase in left ventricular developed pressure (LVDP), RPP, and MO2, respectively, in controls. In contrast, the inotropic response of ob/ob hearts to increasing calcium was attenuated (LVDP and RPP increased by only 1.5-fold; Table 1). MO2 did not increase in response to increased workload in ob/ob hearts. Thus, glucose-perfused ob/ob hearts exhibit a defect in oxygen consumption under conditions of increased work (Figure 1A).
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Cardiac Function in Glucose- and Palmitate-Perfused Hearts
We next examined contractile parameters in hearts that were perfused with glucose and the FA palmitate. Palmitate 1 mmol/L was chosen to mimic the in vivo concentrations of free FAs in ob/ob mice.6 Under these conditions, ob/ob hearts showed no statistical difference in LVDP, RPP, dP/dtmin, or dP/dtmax versus age-matched controls (Table 2); however, MO2 was 23% higher in ob/ob hearts than in controls, which led to a significant reduction in CE in obese mice (Table 2). Relative to glucose-perfused control hearts, MO2 increased by 18% in palmitate-perfused controls. This contrasts with ob/ob hearts in which MO2 increased by 62% relative to glucose-perfused ob/ob hearts. Inotropic responses in wild-type hearts perfused with glucose and palmitate were similar to changes in glucose-perfused control hearts. Thus, calcium stimulation resulted in a 2.3-fold increase in LVDP and RPP, which was associated with doubling of MO2 (Table 2; Figure 1B). In ob/ob hearts perfused with glucose and palmitate, the inotropic response to increased calcium was greater than that observed in glucose-perfused ob/ob hearts (1.96- versus 1.5-fold increase in RPP), but peak RPP remained lower in palmitate-perfused ob/ob hearts than in wild-type hearts (Table 2). In contrast to glucose-perfused hearts, MO2 in palmitate-perfused ob/ob hearts increased by 55%, and MO2 was equivalent to wild-type hearts at high workload (50.1±4.1 versus 52.1±1.4 µmol · min–1 · g–1). The relationship between RPP and MO2 was similar in wild-type hearts perfused with or without palmitate, but the relationship was shifted to the left in ob/ob hearts perfused with glucose and palmitate so that any given RPP was associated with greater oxygen utilization (Figure 1B). Thus, CE was reduced significantly in ob/ob hearts perfused with glucose and palmitate both at baseline and after inotropic stimulation (Table 2).
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Mitochondrial Function in Glucose-Perfused Hearts
To test the hypothesis that mitochondrial dysfunction contributed to reduced oxygen consumption in glucose-perfused ob/ob hearts after calcium stress, mitochondrial respiration and ATP synthesis rates were measured in saponin-permeabilized cardiac fibers isolated from glucose-perfused hearts at [2 mmol/L] Ca2+. Experiments were performed with 3 different substrates to isolate potential defects in the tricarboxylic acid (TCA) cycle and electron transport flux with glutamate, in carbohydrate-dependent flux with pyruvate, and in the carnitine shuttle and/or ß-oxidation with palmitoyl-carnitine. Permeabilized fibers that were obtained from ob/ob hearts perfused with glucose as sole substrate exhibited reduced mitochondrial respiration. In glutamate-treated fibers, state 3 and state 4 (Voligomycin) mitochondrial respirations were reduced by 39% (Figure 2). ATP synthesis and ATP/O ratios were unchanged. State 3 mitochondrial respirations were also reduced in ob/ob fibers incubated with palmitoyl-carnitine (20% reduction, P<0.05 versus controls), but the ATP synthesis rates and ATP/O ratios were again similar to controls (Figure 3). The most pronounced changes in mitochondrial function were obtained with pyruvate. State 2 respirations (V0) were reduced by 23% in ob/ob mice compared with controls (P<0.05). State 3 (VADP) and state 4 (Voligomycin) respiration rates were also reduced by 29% and 33% in ob/ob mice versus controls (Figure 4). In contrast to glutamate- and palmitoyl-carnitine–exposed fibers, ATP production was depressed by 35% in obese animals (40.1±5.33 versus 61.65±5.02 nmol ATP · min–1 · mg dry weight–1). Because ATP and oxygen consumption rates were reduced proportionally, the ATP/O ratios were not different from controls.
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P<0.05 vs glucose-and-palmitate–perfused wild type. ATP synthesis rates were significantly lower in glucose-and-palmitate ob/ob fibers than in similarly perfused wild-type fibers by unpaired t test (P<0.05). mgdw indicates milligrams of dry weight.
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Mitochondrial Function in Glucose- and Palmitate-Perfused Hearts
Mitochondrial analyses were repeated in fibers obtained from hearts that were perfused with glucose and palmitate at [2 mmol/L] Ca2+ to test the hypothesis that FA-induced mitochondrial uncoupling would further impair mitochondrial function in the hearts of ob/ob mice. Compared with glucose-perfused wild-type hearts, state 3 mitochondrial respiration rates and ATP production declined in permeabilized fibers obtained from palmitate-and-glucose–perfused wild-type hearts exposed to glutamate and pyruvate as substrates (Figures 2 and 4
, respectively). These changes were most pronounced with pyruvate, for which state 3 was 19.77±1.78 in glucose-perfused wild-type hearts versus 15.08±0.89 nmol O2 · min–1 · mg dry weight–1 (P<0.05) in glucose-and-palmitate–perfused wild-type hearts (Figure 4). ATP production and state 3 respiration rates were proportionally reduced, and thus, the ATP/O ratios were not different in glucose- versus glucose-and-palmitate–perfused wild-type hearts. In contrast, state 3 respirations tended to increase in ob/ob mitochondria obtained from palmitate-and-glucose–perfused hearts relative to ob/ob mitochondria obtained from hearts that were perfused with glucose alone. Thus, the reduction in respiration rates in ob/ob mitochondria that was apparent in glucose-perfused hearts was no longer seen (Figures 2, 3, and 4). State 4 (Voligomycin) respirations that reflect uncoupled respiration were increased significantly in mitochondria obtained from ob/ob hearts when incubated with palmitoyl-carnitine (P<0.05), and although a similar trend was observed in controls, that difference did not achieve statistical significance (P=0.08). ATP levels were significantly lower in ob/ob mitochondria exposed to pyruvate and palmitoyl carnitine, and the calculated ATP/O ratios (ATP synthesis rates/state 3 respiration) were profoundly reduced in the ob/ob mitochondria obtained from hearts perfused with both glucose and palmitate relative to similarly perfused wild-type hearts.
Mitochondrial Enzyme Activities and Protein Expression
To elucidate the mechanisms responsible for diminished mitochondrial respiration in glucose-perfused ob/ob hearts, the activity of key enzymes involved in glucose oxidation and FA transport and oxidation, as well as the expression of various mitochondrial proteins, was examined. All assays, with the exception of UCP3 immunoblots, were performed in fresh hearts after rapid removal from deeply anesthetized mice. UCP3 immunoblots were performed on mitochondria that were isolated from hearts that were perfused with 1 mmol/L palmitate and 11 mmol/L glucose. As summarized in Table 3, total CPT, CPT 1, and CPT 2 activities were not different between ob/ob and control mice. However, both CS and ß-hydroxyacyl-CoA dehydrogenase activities were slightly increased by 10% (P=0.058) and 14% (P=0.08), respectively, in obese mice. The active fraction of PDH was 21% lower in ob/ob animals than in control animals (1.23±0.08 versus 1.52±0.07 nmol · min–1 · mg tissue–1; P<0.05), but total PDH activity was similar between the 2 groups. Complex I levels were reduced by 57%, and complex III and the -subunit of the ATP synthase were reduced by 30% and 33%, respectively, in ob/ob mice (Figure 5A). To evaluate whether increased expression of uncoupling proteins contributed to the enhancement of FA-induced uncoupling observed in ob/ob mitochondria, we examined the protein content of UCP2 and UCP3. UCP2 protein was undetectable in the hearts of both controls and ob/ob mice (data not shown). UCP3 levels were unchanged in ob/ob hearts compared with their age-matched controls (Figure 5B).
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Discussion |
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This study demonstrated that obesity is associated with specific alterations in mitochondrial oxidative capacity and the coupling of oxygen consumption and ATP production. We found that mitochondria from glucose-perfused ob/ob hearts revealed marked impairments in respiratory capacity that were most pronounced in the presence of pyruvate and also correlated with decreased PDH activity. As a consequence, glucose-perfused ob/ob hearts were severely limited in their ability to increase M
O2 in response to increased workload when glucose was the sole substrate. This contrasts with the responses of ob/ob hearts in the presence of palmitate, in which MO2 rose significantly at high workload. We therefore believe that the limitation in inotropic oxygen consumption in glucose-perfused hearts reflects impaired substrate flux via PDH and reduced oxidative capacity of mitochondria that is also due in part to depletion of key mitochondrial electron transport chain components. In contrast, in hearts perfused with glucose and palmitate, ob/ob hearts exhibited increased MO2 under basal conditions in the absence of a concomitant increase in cardiac performance, which leads to reduced cardiac efficiency. Moreover, in response to an inotropic challenge, MO2 increased further, but CE remained low. Furthermore, FA impaired the coupling of oxygen consumption and ATP generation in ob/ob mitochondria. Thus, the glucose-only perfusions highlighted the presence of global defects in mitochondrial respiratory capacity in ob/ob hearts, and the studies performed after glucose and palmitate perfusion revealed an additional defect, namely, FA-induced mitochondrial uncoupling. FAs therefore preferentially induce mitochondrial uncoupling in obese mouse hearts that is characterized by reduced ATP production that is not accompanied by a proportional reduction in oxygen consumption.
We have previously shown that in isolated working hearts perfused with palmitate and glucose, ob/ob mouse hearts demonstrated elevated rates of FA oxidation and MO2 relative to controls and that increasing the FA concentrations caused a progressive rise in MO2 in ob/ob but not in control hearts.6 These observations led us to hypothesize that FA preferentially uncoupled mitochondria from ob/ob mouse hearts. We therefore elected to initially study hearts that were perfused with glucose as the sole substrate to determine the phenotype of ob/ob hearts and their mitochondria in the absence of the potential contribution of exogenous FA-induced uncoupling. Intriguingly, we observed no difference in MO2 in glucose-perfused ob/ob and wild-type hearts; however, their mitochondria were characterized by reduced rates of mitochondrial respiration and ATP generation, particularly in the presence of pyruvate as a substrate. We therefore reasoned that this reduction in mitochondrial function might reflect a limitation at the level of PDH. This was indeed confirmed by direct analysis of the active fraction of PDH, the activity levels of which were reduced in ob/ob hearts. To further demonstrate that limited PDH flux might impair myocardial performance, we determined MO2 in glucose-perfused hearts that were subjected to an inotropic challenge. Interestingly, the inotropic response to calcium was attenuated in ob/ob mouse hearts, and MO2 failed to increase. The lack of an increase in MO2 despite a modest increase in contractility is unusual but not without precedent. McConville et al20 demonstrated that ß-1-adrenergic stimulation of isolated rat hearts increased RPP in the absence of a concomitant increase in MO2. Our observations imply that the energy that fuels the increased E-C coupling that is induced by high calcium in ob/ob hearts might be coming from anaerobic glycolysis or from more rapid depletion of phosphocreatine pools. The present study design did not allow us to distinguish between these 2 possibilities. It is also possible that the reduction in MO2 in glucose-perfused hearts simply reflects a reduction in work. We think that this is relatively unlikely, because the reduction in work was not proportional to the reduction in MO2, and in FA-perfused hearts, the relatively impaired inotropic response occurred despite an increase in MO2. Recent studies also suggest that the sensitivity of the E-C coupling machinery to calcium may be altered in hearts of ob/ob and db/db mice.3,21,22 Thus, the contribution of altered calcium sensitivity to the impaired inotropic response to calcium observed in the present study needs to be considered. It is unlikely, though, that differences in calcium sensitivity can completely account for the differences in the degree of the inotropic responses and changes in MO2 that were observed in glucose- versus glucose-and-palmitate–perfused ob/ob hearts.
The present data suggest that there is a significant limitation in the ability of ob/ob mouse hearts to utilize glucose under high workload conditions and are supported by our earlier observations that glucose utilization is severely impaired in isolated working ob/ob hearts.6 Mitochondria from glucose-perfused ob/ob hearts that were exposed to glutamate and palmitoyl carnitine also demonstrated a significant reduction in state 3 respirations. Palmitoyl carnitine enters the mitochondria via CPT2 and then undergoes ß-oxidation, which contributes reducing equivalents directly to the electron transport chain in addition to generating acetyl CoA. We observed no defects in the activity of CPT1 or CPT2 or in a representative enzyme of ß-oxidation. Thus, the limitation in state 3 respiration likely represents reduced TCA flux or impaired electron transport chain activity. Glutamate enters the TCA cycle via conversion to -ketoglutarate and then contributes its reducing equivalents to the electron transport chain. Thus, response to this substrate interrogates the TCA cycle and the electron transport chain. We observed no reduction in the activity of 1 of the rate-limiting enzymes of the TCA cycle, namely, CS. We cannot rule out the possibility that -ketoglutarate dehydrogenase activity could be reduced; however, we did observe significant reductions in the content of various components of the electron transport chain. Taken together, these observations suggest that in addition to reduced PDH flux, mitochondrial energetics in obese mice is also limited by changes in electron transport chain flux or capacity.
Having demonstrated that mitochondria from ob/ob mice are defective, we then wanted to determine whether FA further impaired mitochondrial function by selectively uncoupling respiration from ATP generation in ob/ob hearts, by analyzing myocardial oxygen consumption and mitochondrial function in hearts that were perfused with glucose and palmitate. Consistent with our earlier observations in working hearts, the addition of FAs caused a preferential increase in MO2 in ob/ob hearts that was not accompanied by any change in cardiac function. Furthermore, under high workload conditions, ob/ob hearts always exhibited higher MO2 than wild-type hearts, despite a blunted inotropic response. Why did MO2 increase? We believe that the increase in MO2 in part reflects mitochondrial uncoupling. The evidence for this includes the following. State 3 mitochondrial respirations were increased in glucose-perfused control hearts relative to glucose-perfused ob/ob hearts for all substrates. Perfusion of hearts with palmitate led to a reduction in state 3 respirations with pyruvate as substrate in control hearts. One mechanism for this may be an intact Randle cycle in control hearts.23 Given the reduction of PDH activity in ob/ob hearts, we expected to see a pronounced effect of FA on reducing pyruvate respiration. In contrast, state 3 respirations tended to increase in ob/ob mouse hearts after palmitate perfusion. Despite this, ATP generation did not increase, and the ratio of ATP production to oxygen consumption declined. In the presence of palmitoyl-carnitine as a substrate, state 4 respirations were statistically increased in ob/ob hearts and tended to increase in control hearts that were perfused with palmitate. The increase in state 4 respirations is consistent with mitochondrial uncoupling in both groups, but the bioenergetic consequences of this were more severe in ob/ob mitochondria, as evidenced by the reduction in ATP generation and the reduction in ATP/O ratios relative to mitochondria from glucose-and-palmitate–perfused controls. Thus, in light of the reduced mitochondrial efficiency in FA-perfused ob/ob hearts, it would be expected that oxygen consumption would need to increase to maintain ATP generation.
To evaluate potential mechanisms for the preferential increase in mitochondrial uncoupling in the presence of FAs, we evaluated the possibility that uncoupling protein abundance was increased in the hearts of ob/ob mice. The UCP3 gene is regulated by PPAR-, and its expression levels can be regulated in the adult heart by synthetic PPAR- ligands and conditions that would increase ambient concentrations of free FAs.13,24 Streptozotocin-induced diabetes is associated with increased expression of UCP3 mRNA in rat hearts, but changes in protein levels were not examined.11 In contrast, UCP2 appears to be regulated by FA in neonatal cardiomyocytes but does not appear to be regulated in adults hearts.25 Indeed, we detected minimal myocardial protein expression of UCP2 in the present study, which is consistent with previously published studies in the mouse.26 Because few studies have actually examined changes in uncoupling protein content in the hearts of diabetic or obese rodents, we elected to measure UCP3 protein content by Western blot analyses and confirmed the specificity of our assay by confirming the absence of UCP3 in heart homogenates obtained from UCP3 KO mice.27 To our surprise, we did not observe an increase in UCP3 protein content. Thus, the FA-induced mitochondrial uncoupling that we observed in ob/ob hearts appears to be independent of changes in UCP3 expression. Recent evidence suggests that both FA and superoxide can activate mitochondrial uncoupling.28,29 We have previously demonstrated that rates of FA utilization are increased between 1.5- and 3-fold in isolated working ob/ob hearts depending on perfusion conditions.6 Thus, increased mitochondrial FA flux could lead to or be associated with activation of UCP3. Increased FA oxidation, by increasing the delivery of reducing equivalents to the electron transport chain, ultimately increases the generation of superoxide, which could also increase mitochondrial uncoupling in obese hearts.
The present investigation was performed in animals that were significantly obese and insulin resistant. We have previously shown that at the age studied, these animals have relatively minor defects in glucose tolerance.6 The present studies do not definitively establish whether the mitochondrial adaptations that we observed are specific to obesity or reflect independent effects of leptin deficiency. However, recent observations obtained in humans with obesity and insulin resistance are similar to those that we have observed in ob/ob mouse hearts. Our studies may therefore provide mechanistic insight into these human observations. In a study of women with morbid obesity, Peterson and colleagues30 described increased rates of FA oxidation and uptake, increased MO2, and decreased myocardial efficiency. Scheuermann-Freestone and colleagues31 reported decreased myocardial phosphocreatine/creatine ratios in individuals with type 2 diabetes. Moreover, myocardial energetics was inversely related to serum concentrations of free FAs. Taken together with our previously published observations of increased FA oxidation and increased MO2 in isolated working hearts from ob/ob mice and our current observations, we propose that myocardial energetics is reduced in obesity and insulin-resistant states on the basis of FA-induced mitochondrial uncoupling.
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This work was supported by grants RO1HL73167 and UO1HL70525 from the National Institutes of Health and the Ben and Iris Margolis Foundation to Dr Abel, who is an Established Investigator of the American Heart Association. Dr Boudina is supported by a postdoctoral fellowship from the Juvenile Diabetes Foundation, and B.T. O’Neill is supported by a physician scientist-training award from the American Diabetes Association. We thank Dr Bradford Lowell for kindly providing us with UCP3 knockout mice.
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|---|
1. Mokdad AH, Bowman BA, Ford ES, Vinicor F, Marks JS, Koplan JP. The continuing epidemics of obesity and diabetes in the United States. JAMA. 2001; 286: 1195–1200.
2. Unger RH. Lipotoxic diseases. Annu Rev Med. 2002; 53: 319–336.[CrossRef][Medline] [Order article via Infotrieve]
3. Christoffersen C, Bollano E, Lindegaard ML, Bartels ED, Goetze JP, Andersen CB, Nielsen LB. Cardiac lipid accumulation associated with diastolic dysfunction in obese mice. Endocrinology. 2003; 144: 3483–3490.
4. Szczepaniak LS, Dobbins RL, Metzger GJ, Sartoni-D’Ambrosia G, Arbique D, Vongpatanasin W, Unger R, Victor RG. Myocardial triglycerides and systolic function in humans: in vivo evaluation by localized proton spectroscopy and cardiac imaging. Magn Reson Med. 2003; 49: 417–423.[CrossRef][Medline] [Order article via Infotrieve]
5. Peterson LR, Waggoner AD, Schechtman KB, Meyer T, Gropler RJ, Barzilai B, Davila-Roman VG. Alterations in left ventricular structure and function in young healthy obese women: assessment by echocardiography and tissue Doppler imaging. J Am Coll Cardiol. 2004; 43: 1399–1404.
6. Mazumder PK, O’Neill BT, Roberts MW, Buchanan J, Yun UJ, Cooksey RC, Boudina S, Abel ED. Impaired cardiac efficiency and increased fatty acid oxidation in insulin-resistant ob/ob mouse hearts. Diabetes. 2004; 53: 2366–2374.
7. Belke DD, Larsen TS, Gibbs EM, Severson DL. Altered metabolism causes cardiac dysfunction in perfused hearts from diabetic (db/db) mice. Am J Physiol Endocrinol Metab. 2000; 279: E1104–E1113.
8. Semeniuk LM, Kryski AJ, Severson DL. Echocardiographic assessment of cardiac function in diabetic db/db and transgenic db/db-hGLUT4 mice. Am J Physiol Heart Circ Physiol. 2002; 283: H976–H982.
9. Aasum E, Belke DD, Severson DL, Riemersma RA, Cooper M, Andreassen M, Larsen TS. Cardiac function and metabolism in type 2 diabetic mice after treatment with BM 17.0744, a novel PPAR-alpha activator. Am J Physiol Heart Circ Physiol. 2002; 283: H949–H957.
10. Carley AN, Semeniuk LM, Shimoni Y, Aasum E, Larsen TS, Berger JP, Severson DL. Treatment of type 2 diabetic db/db mice with a novel PPARgamma agonist improves cardiac metabolism but not contractile function. Am J Physiol Endocrinol Metab. 2004; 286: E449–E455.
11. Hidaka S, Kakuma T, Yoshimatsu H, Sakino H, Fukuchi S, Sakata T. Streptozotocin treatment upregulates uncoupling protein 3 expression in the rat heart. Diabetes. 1999; 48: 430–435.[Abstract]
12. Schrauwen P. Skeletal muscle uncoupling protein 3 (UCP3): mitochondrial uncoupling protein in search of a function. Curr Opin Clin Nutr Metab Care. 2002; 5: 265–270.[CrossRef][Medline] [Order article via Infotrieve]
13. Stavinoha MA, RaySpellicy JW, Essop MF, Graveleau C, Abel ED, Hart-Sailors ML, Mersmann HJ, Bray MS, Young ME. Evidence for mitochondrial thioesterase 1 as a peroxisome proliferator-activated receptor-alpha-regulated gene in cardiac and skeletal muscle. Am J Physiol Endocrinol Metab. 2004; 287: E888–E895.
14. Veksler VI, Kuznetsov AV, Sharov VG, Kapelko VI, Saks VA. Mitochondrial respiratory parameters in cardiac tissue: a novel method of assessment by using saponin-skinned fibers. Biochim Biophys Acta. 1987; 892: 191–196.[Medline] [Order article via Infotrieve]
15. Cadenas S, Echtay KS, Harper JA, Jekabsons MB, Buckingham JA, Grau E, Abuin A, Chapman H, Clapham JC, Brand MD. The basal proton conductance of skeletal muscle mitochondria from transgenic mice overexpressing or lacking uncoupling protein-3. J Biol Chem. 2002; 277: 2773–2778.
16. Barger JL, Brand MD, Barnes BM, Boyer BB. Tissue-specific depression of mitochondrial proton leak and substrate oxidation in hibernating arctic ground squirrels. Am J Physiol Regul Integr Comp Physiol. 2003; 284: R1306–R1313.
17. Dumas JF, Roussel D, Simard G, Douay O, Foussard F, Malthiery Y, Ritz P. Food restriction affects energy metabolism in rat liver mitochondria. Biochim Biophys Acta. 2004; 1670: 126–131.[Medline] [Order article via Infotrieve]
18. Rodnick KJ, Sidell BD. Cold acclimation increases carnitine palmitoyltransferase I activity in oxidative muscle of striped bass. Am J Physiol. 1994; 266: R405–R412.[Medline] [Order article via Infotrieve]
19. Sterk JP, Stanley WC, Hoppel CL, Kerner J. A radiochemical pyruvate dehydrogenase assay: activity in heart. Anal Biochem. 2003; 313: 179–182.[CrossRef][Medline] [Order article via Infotrieve]
20. McConville P, Fishbein KW, Lakatta EG, Spencer RG. Differences in the bioenergetic response of the isolated perfused rat heart to selective beta1- and beta2-adrenergic receptor stimulation. Circulation. 2003; 107: 2146–2152.
21. Belke DD, Swanson EA, Dillmann WH. Decreased sarcoplasmic reticulum activity and contractility in diabetic db/db mouse heart. Diabetes. 2004; 53: 3201–3208.
22. Minhas KM, Khan SA, Raju SV, Phan AC, Gonzalez DR, Skaf MW, Lee K, Tejani AD, Saliaris AP, Barouch LA, O’Donnell CP, Emala CW, Berkowitz DE, Hare JM. Leptin repletion restores depressed ß-adrenergic contractility in ob/ob mice independently of cardiac hypertrophy. J Physiol. 2005; 565: 463–474.
23. Randle PJ, Garland PB, Hales CN, Newsholme EA. The glucose fatty-acid cycle: its role in insulin sensitivity and the metabolic disturbances of diabetes mellitus. Lancet. 1963; 1: 785–789.[Medline] [Order article via Infotrieve]
24. Young ME, Patil S, Ying J, Depre C, Ahuja HS, Shipley GL, Stepkowski SM, Davies PJ, Taegtmeyer H. Uncoupling protein 3 transcription is regulated by peroxisome proliferator-activated receptor (alpha) in the adult rodent heart. FASEB J. 2001; 15: 833–845.
25. Van Der Lee KA, Willemsen PH, Van Der Vusse GJ, Van Bilsen M. Effects of fatty acids on uncoupling protein-2 expression in the rat heart. FASEB J. 2000; 14: 495–502.
26. Pecqueur C, Alves-Guerra MC, Gelly C, Levi-Meyrueis C, Couplan E, Collins S, Ricquier D, Bouillaud F, Miroux B. Uncoupling protein 2, in vivo distribution, induction upon oxidative stress, and evidence for translational regulation. J Biol Chem. 2001; 276: 8705–8712.
27. Vidal-Puig AJ, Grujic D, Zhang CY, Hagen T, Boss O, Ido Y, Szczepanik A, Wade J, Mootha V, Cortright R, Muoio DM, Lowell BB. Energy metabolism in uncoupling protein 3 gene knockout mice. J Biol Chem. 2000; 275: 16258–16266.
28. Echtay KS, Murphy MP, Smith RA, Talbot DA, Brand MD. Superoxide activates mitochondrial uncoupling protein 2 from the matrix side: studies using targeted antioxidants. J Biol Chem. 2002; 277: 47129–47135.
29. Echtay KS, Roussel D, St-Pierre J, Jekabsons MB, Cadenas S, Stuart JA, Harper JA, Roebuck SJ, Morrison A, Pickering S, Clapham JC, Brand MD. Superoxide activates mitochondrial uncoupling proteins. Nature. 2002; 415: 96–99.[CrossRef][Medline] [Order article via Infotrieve]
30. Peterson LR, Herrero P, Schechtman KB, Racette SB, Waggoner AD, Kisrieva-Ware Z, Dence C, Klein S, Marsala J, Meyer T, Gropler RJ. Effect of obesity and insulin resistance on myocardial substrate metabolism and efficiency in young women. Circulation. 2004; 109: 2191–2196.
31. Scheuermann-Freestone M, Madsen PL, Manners D, Blamire AM, Buckingham RE, Styles P, Radda GK, Neubauer S, Clarke K. Abnormal cardiac and skeletal muscle energy metabolism in patients with type 2 diabetes. Circulation. 2003; 107: 3040–3046.
 |
|
 |
|
  Z. Lu, I. Scott, B. R. Webster, and M. N. Sack The Emerging Characterization of Lysine Residue Deacetylation on the Modulation of Mitochondrial Function and Cardiovascular Biology Circ. Res., October 23, 2009; 105(9): 830 - 841. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 L. J. Rijzewijk, R. W. van der Meer, H. J. Lamb, H. W.A.M. de Jong, M. Lubberink, J. A. Romijn, J. J. Bax, A. de Roos, J. W. Twisk, R. J. Heine, et al. Altered myocardial substrate metabolism and decreased diastolic function in nonischemic human diabetic cardiomyopathy studies with cardiac positron emission tomography and magnetic resonance imaging. J. Am. Coll. Cardiol., October 13, 2009; 54(16): 1524 - 1532. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 H. Bugger and E. D. Abel Rodent models of diabetic cardiomyopathy Dis. Model. Mech., September 1, 2009; 2(9-10): 454 - 466. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 M. Schwarzer and T. Doenst Letter to the editor: "Does a reduction in ADP-limited respiration indicate impaired mitochondrial function?" Am J Physiol Heart Circ Physiol, August 1, 2009; 297(2): H889 - H889. [Full Text] [PDF]
|
|
|
|
 |
|
 J. J. Wright, J. Kim, J. Buchanan, S. Boudina, S. Sena, K. Bakirtzi, O. Ilkun, H. A. Theobald, R. C. Cooksey, K. V. Kandror, et al. Mechanisms for increased myocardial fatty acid utilization following short-term high-fat feeding Cardiovasc Res, May 1, 2009; 82(2): 351 - 360. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 S. Boudina, H. Bugger, S. Sena, B. T. O'Neill, V. G. Zaha, O. Ilkun, J. J. Wright, P. K. Mazumder, E. Palfreyman, T. J. Tidwell, et al. Contribution of Impaired Myocardial Insulin Signaling to Mitochondrial Dysfunction and Oxidative Stress in the Heart Circulation, March 10, 2009; 119(9): 1272 - 1283. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 A. W. Norris, M. F. Hirshman, J. Yao, N. Jessen, N. Musi, L. Chen, W. I. Sivitz, L. J. Goodyear, and C. R. Kahn Endogenous Peroxisome Proliferator-Activated Receptor-{gamma} Augments Fatty Acid Uptake in Oxidative Muscle Endocrinology, November 1, 2008; 149(11): 5374 - 5383. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 H. Bugger, S. Boudina, X. X. Hu, J. Tuinei, V. G. Zaha, H. A. Theobald, U. J. Yun, A. P. McQueen, B. Wayment, S. E. Litwin, et al. Type 1 Diabetic Akita Mouse Hearts Are Insulin Sensitive but Manifest Structurally Abnormal Mitochondria That Remain Coupled Despite Increased Uncoupling Protein 3 Diabetes, November 1, 2008; 57(11): 2924 - 2932. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
I. Tabbi-Anneni, J. Buchanan, R. C. Cooksey, and E. D. Abel Captopril Normalizes Insulin Signaling and Insulin-Regulated Substrate Metabolism in Obese (ob/ob) Mouse Hearts Endocrinology, August 1, 2008; 149(8): 4043 - 4050. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 R. Harmancey, C. R. Wilson, and H. Taegtmeyer Adaptation and Maladaptation of the Heart in Obesity Hypertension, August 1, 2008; 52(2): 181 - 187. [Full Text] [PDF]
|
|
|
|
 |
|
 E. D. Abel, S. E. Litwin, and G. Sweeney Cardiac Remodeling in Obesity Physiol Rev, April 1, 2008; 88(2): 389 - 419. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
J.-a Kim, Y. Wei, and J. R. Sowers Role of Mitochondrial Dysfunction in Insulin Resistance Circ. Res., February 29, 2008; 102(4): 401 - 414. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
R. M. Witteles and M. B. Fowler Insulin-Resistant Cardiomyopathy: Clinical Evidence, Mechanisms, and Treatment Options J. Am. Coll. Cardiol., January 15, 2008; 51(2): 93 - 102. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
E. H. Koh, J.-Y. Park, H.-S. Park, M. J. Jeon, J. W. Ryu, M. Kim, S. Y. Kim, M.-S. Kim, S.-W. Kim, I. S. Park, et al. Essential Role of Mitochondrial Function in Adiponectin Synthesis in Adipocytes Diabetes, December 1, 2007; 56(12): 2973 - 2981. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
S. Boudina, S. Sena, H. Theobald, X. Sheng, J. J. Wright, X. X. Hu, S. Aziz, J. I. Johnson, H. Bugger, V. G. Zaha, et al. Mitochondrial Energetics in the Heart in Obesity-Related Diabetes: Direct Evidence for Increased Uncoupled Respiration and Activation of Uncoupling Proteins Diabetes, October 1, 2007; 56(10): 2457 - 2466. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
D. J. Durgan, M. W. S. Moore, N. P. Ha, O. Egbejimi, A. Fields, U. Mbawuike, A. Egbejimi, C. A. Shaw, M. S. Bray, V. Nannegari, et al. Circadian rhythms in myocardial metabolism and contractile function: influence of workload and oleate Am J Physiol Heart Circ Physiol, October 1, 2007; 293(4): H2385 - H2393. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 H.-X. Hao, C. M. Cardon, W. Swiatek, R. C. Cooksey, T. L. Smith, J. Wilde, S. Boudina, E. D. Abel, D. A. McClain, and J. Rutter PAS kinase is required for normal cellular energy balance PNAS, September 25, 2007; 104(39): 15466 - 15471. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
G. D. Lopaschuk, C. D.L. Folmes, and W. C. Stanley Cardiac Energy Metabolism in Obesity Circ. Res., August 17, 2007; 101(4): 335 - 347. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
S. Boudina and E. D. Abel Diabetic Cardiomyopathy Revisited Circulation, June 26, 2007; 115(25): 3213 - 3223. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
W. Hsueh, E. D. Abel, J. L. Breslow, N. Maeda, R. C. Davis, E. A. Fisher, H. Dansky, D. A. McClain, R. McIndoe, M. K. Wassef, et al. Recipes for Creating Animal Models of Diabetic Cardiovascular Disease Circ. Res., May 25, 2007; 100(10): 1415 - 1427. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
E. Nisoli, E. Clementi, M. O. Carruba, and S. Moncada Defective Mitochondrial Biogenesis: A Hallmark of the High Cardiovascular Risk in the Metabolic Syndrome? Circ. Res., March 30, 2007; 100(6): 795 - 806. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
J. G. Duncan, J. L. Fong, D. M. Medeiros, B. N. Finck, and D. P. Kelly Insulin-Resistant Heart Exhibits a Mitochondrial Biogenic Response Driven by the Peroxisome Proliferator-Activated Receptor-{alpha}/PGC-1{alpha} Gene Regulatory Pathway Circulation, February 20, 2007; 115(7): 909 - 917. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
D. An and B. Rodrigues Role of changes in cardiac metabolism in development of diabetic cardiomyopathy Am J Physiol Heart Circ Physiol, October 1, 2006; 291(4): H1489 - H1506. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 S. Boudina and E. D. Abel Mitochondrial uncoupling: a key contributor to reduced cardiac efficiency in diabetes. Physiology, August 1, 2006; 21: 250 - 258. [Abstract] [Full Text] [PDF]
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