OBJECTIVE Impairments in mitochondrial function have been proposed to play a role in the etiology of diabetic sensory neuropathy. We tested the hypothesis that mitochondrial dysfunction in axons of sensory neurons in type 1 diabetes is due to abnormal activity of the respiratory chain and an altered mitochondrial proteome.
RESEARCH DESIGN AND METHODS Proteomic analysis using stable isotope labeling with amino acids in cell culture (SILAC) determined expression of proteins in mitochondria from dorsal root ganglia (DRG) of control, 22-week-old streptozotocin (STZ)-diabetic rats, and diabetic rats treated with insulin. Rates of oxygen consumption and complex activities in mitochondria from DRG were measured. Fluorescence imaging of axons of cultured sensory neurons determined the effect of diabetes on mitochondrial polarization status, oxidative stress, and mitochondrial matrix-specific reactive oxygen species (ROS).
RESULTS Proteins associated with mitochondrial dysfunction, oxidative phosphorylation, ubiquinone biosynthesis, and the citric acid cycle were downregulated in diabetic samples. For example, cytochrome c oxidase subunit IV (COX IV; a complex IV protein) and NADH dehydrogenase Fe-S protein 3 (NDUFS3; a complex I protein) were reduced by 29 and 36% (P < 0.05), respectively, in diabetes and confirmed previous Western blot studies. Respiration and mitochondrial complex activity was significantly decreased by 15 to 32% compared with control. The axons of diabetic neurons exhibited oxidative stress and depolarized mitochondria, an aberrant adaption to oligomycin-induced mitochondrial membrane hyperpolarization, but reduced levels of intramitochondrial superoxide compared with control.
CONCLUSIONS Abnormal mitochondrial function correlated with a downregulation of mitochondrial proteins, with components of the respiratory chain targeted in lumbar DRG in diabetes. The reduced activity of the respiratory chain was associated with diminished superoxide generation within the mitochondrial matrix and did not contribute to oxidative stress in axons of diabetic neurons. Alternative pathways involving polyol pathway activity appear to contribute to raised ROS in axons of diabetic neurons under high glucose concentration.
Enhanced oxidative stress is thought to be a central pathologic feature in the etiology of diabetic peripheral neuropathy (1). To develop more targeted therapeutics toward ameliorating oxidative stress and the development of diabetic peripheral neuropathy, considerable effort has focused on identifying the cellular source of reactive oxygen species (ROS) over the past decade. Brownlee et al. (2) suggested that mitochondrial superoxide generation may be a critical feature in the onset of diabetic complications. In cultured endothelial cells, hyperglycemia induced excessive electron flux through the respiratory chain that promoted mitochondrial hyperpolarization and elevated ROS production (2,3). These investigators proposed that hyperglycemia increases mitochondrial NADH levels and that increased electron availability and/or saturation causes partial reduction of oxygen to superoxide in the proximal part of the respiratory chain (2). In support of this mechanism, epineurial arterioles serving the sciatic nerve of STZ-diabetic rats show increased levels of mitochondrial superoxide that is dependent on complex I activity (4). On the other hand, studies in diabetic retina suggest that metabolism of high glucose concentrations does not operate in a fashion that supports superoxide formation by the respiratory chain (5). Similarly, in sensory neurons from STZ-diabetic rats, the mitochondrial membrane potential is depolarized and not hyperpolarized, as observed in endothelial cells exposed to hyperglycemia (6,7). Further, lumbar dorsal root ganglia (DRG) from diabetic rats exhibit reduced respiratory chain activity that correlate with the downregulation of select proteins within the electron transport chain complexes (8). These findings are aligned with studies in diabetic heart where mitochondrial respiration and enzymatic activities are reduced (9,10). In addition, activities of citrate synthase and mitochondrial respiratory chain are decreased in the skeletal muscle of patients with type 2 diabetes (11–13).
Therefore, production of mitochondrial superoxide may exhibit fundamental differences in cells that are targets of diabetic complications. Indeed, the tissue-specific nature of mitochondrial remodeling in diabetes is directly underscored by results from an unbiased proteomic study that identified a differential effect of diabetes on the mitochondrial protein expression and oxidative capacity. For example, proteins associated with oxidative phosphorylation were more depressed and respiratory activity decreased in heart compared with liver mitochondria from diabetic Akita mice (14). Since DRG sensory neurons are highly susceptible to glucotoxicity (15), we examined the effect of diabetes on the mitochondrial proteome, respiratory capacity, and superoxide production. Our previous work on sensory neurons in diabetes demonstrated mitochondrial depolarization within the perikarya and lowered respiratory chain capacity (6,8); however, our objective in the current work was to relate the effects of diabetes on mitochondrial proteome expression to mitochondrial physiology and function within the axon where oxidative stress and degeneration are most clearly defined (16–18). To this end, we exploited the use of stable isotope labeling of cells in culture (SILAC) (19) to provide a set of culture-derived isotope tags (20) to serve as internal standards for a quantitative proteomic analysis. We demonstrate that in diabetes impaired respiratory chain function correlates with decreased protein expression, and in mitochondria of axons, these deficits are associated with membrane depolarization and reduced respiratory chain-derived ROS generation. These data support the conclusion that glucose-dependent superoxide production within the mitochondrial matrix is not a major contributor to oxidative stress in axons of DRG in long-term diabetes.
RESEARCH DESIGN AND METHODS
Induction, treatment, and confirmation of type 1 diabetes.
Male Sprague Dawley rats were made diabetic with a single intraperitoneal injection of 75 mg/kg STZ (Sigma, St Louis, MO). Insulin implants (two Linplant implants; Linshin Canada, Toronto, ON, Canada) were placed subcutaneously into STZ-diabetic rats after 18 weeks of diabetes and kept in place for 4 weeks. Animals were killed and tissue collected after 22 weeks of diabetes. Animal procedures followed the guidelines of the University of Manitoba Animal Care Committee using the Canadian Council of Animal Care rules.
Preparation of isolated mitochondria from DRG and isotopically labeled SC16 cells.
Mitochondrial preparations from DRG were isolated as described (8,21). Immortalized SC16 Schwann cells were cultured in low glucose Dulbecco's modified Eagle's medium containing 125 mg/l 13C6-lysine (K6) and 84 mg/l 13C6,15N4-arginine (R10) (Cambridge Isotopes, Andover, MA), 10% dialyzed FCS (Atlas Biologicals, Fort Collins, CO), and antibiotics (22). Crude mitochondria from labeled cells were obtained by differential centrifugation and purified through a discontinuous Nycodenz gradient (23). For quantitative analysis of the DRG mitochondrial proteome, the K6R10-labeled mitochondria were used as a source of culture-derived isotope tags to serve as internal standards (20). After assessing the protein concentration of the preparations, the unlabeled mitochondrial protein (K0R0) obtained from each of the control (n = 4), diabetic (n = 3), and diabetic + insulin (n = 4) treatments were mixed in a 2:1 ratio with K6R10 labeled mitochondria. Total protein (60–70 μg) was subjected to SDS-PAGE, the gel was stained with colloidal Coomassie blue, and lanes were cut into 5 × 1 cm pieces.
RP-HPLC/LTQ-FT MS/MS and protein identification and quantification criteria.
A detailed description of these parameters is provided in supplementary Table 1 in the online appendix 2 at http://diabetes.diabetesjournals.org/cgi/content/full/db10-0818/DC1. See Fig. 1 for an overview of the SILAC approach.
Adult rat DRG sensory neuron culture.
Lumbar DRG sensory neurons from adult male Sprague-Dawley rats were isolated and dissociated as described (6,16). Rats were either age-matched control or 22-week STZ-diabetic. Cells were plated onto poly-d-l-ornithine hydrobromide and laminin-coated 25-mm glass cover slips (German glass #1, Electron Microscopy Sciences, Hatfield, PA). Neurons were grown in defined Hams F-12 medium with N2 additives (no insulin), supplemented with neurotrophic factors: 0.1 ng/ml nerve growth factor, 1.0 ng/ml glial cell line-derived neurotrophic factor, and 0.1 ng/ml neurotrophin-3 (all obtained from Sigma). Neurons from control rats were cultured with 10 mmol/l d-glucose and 10 nmol/l insulin and neurons from diabetic rats were plated with 25 mmol/l d-glucose and no insulin for 1 to 3 days.
Determination of oxidative stress in axons.
Cultured neurons from control or diabetic rats were either 1) imaged in real time for intracellular ROS by loading with 1.2 μmol/l 5-(and-6)-chloromethyl-2′7′-dichlorodihydrofluorescein diacetate acetyl ester (CM-H2DCFDA), or 2) fixed and stained for adducts of 4-hydroxy-2-nonenal (4-HNE) (a product of lipid peroxidation), as previously described (16). To study the role of polyol pathway in ROS production, cultures were treated acutely with the specific sorbitol dehydrogenase (SDH) inhibitor, SDI-158 (24) (10 μmol/l; a gift from Dr. Nigel Calcutt, University of California San Diego).
Assessment of mitochondrial membrane potential in cultured neurons.
Cultured DRG neurons were loaded with 3.0 nmol/l tetramethyl rhodamine methyl ester (TMRM; Molecular Probes, Eugene, OR) for 1 h and the fluorescence signal in the axons detected with a Carl Zeiss LSM510 confocal inverted microscope (X100 objective; excitation at 540 nm and emission >560 nm). The TMRM was used in subquench mode—in which decreased fluorescence intensity indicates reduced mitochondrial inner membrane potential (25). Antimycin A and oligomycin (Sigma) were injected into the culture media to a final concentration of 10 μmol/l and 1 μmol/l, respectively, at 1 min after baseline fluorescence measurements. All axons in each field were assessed as the average of fluorescence pixel intensity per axon length using the Carl Zeiss software package (16).
Intramitochondrial ROS measurement.
Intramitochondrial ROS generation, mainly superoxide, was detected using the fluorescent MitoSOX red dye (Molecular Probes, catalog #M36008). Lumbar DRG neurons were loaded with 400 nmol/l of MitoSOX red (in 100% anhydrous DMSO; Molecular Probes) for 15 min with or without 1.0 μmol/l oligomycin at 37°C, and then washed three times with F-12 and excited at 514 nm and emission >560 nm.
Respiratory chain function.
Oxygen consumption was determined at 37°C using the OROBOROS Oxygraph-2K (OROBOROS Instruments GmbH, Innsbruck, Austria) (8). Mitochondria from freshly isolated and intact lumbar DRG were resuspended in KCl medium (80 mmol/l KCl, 10 mmol/l Tris-HCl, 3.0 mmol/l MgCl2, 1.0 mmol/l EDTA, 5.0 mmol/l potassium phosphate, pH 7.4). Various substrates and inhibitors of the mitochondrial respiratory chain complexes were used as described (8). Enzymatic activities in lumbar DRG mitochondrial preparations were performed spectrophotometrically as previously described (8).
When appropriate, data were subjected to one-way ANOVA with post hoc comparison using the Tukey test or regression analysis with a one-phase exponential decay parametric test with the Fisher parameter (GraphPad Prism 4, GraphPad Software, San Diego, CA). In all other cases, two-tailed Student t tests were performed. To determine the threshold for statistical significance for the proteomic data, proteins showing at least a 20 or 25% increase or decrease were grouped and compared with the entire dataset using a Kruskal-Wallis nonparametric ANOVA and the Dunn multiple comparison test. This analysis indicated that a minimum difference of 25% was necessary for a value to be considered statistically different from the dataset.
STZ-diabetic rats did not suffer weight loss during the study, but they showed reduced weight gain after 22 weeks of STZ-diabetes compared with age-matched controls (Table 1). Persistence of diabetes was indicated by elevated nonfasting blood glucose and glycated hemoglobin levels (Table 1). STZ-diabetic rats that received insulin supplementation for the final 4 weeks of a 22-week period of diabetes showed a partial, but statistically significant, recovery of body weight, blood glucose, and glycated hemoglobin levels.
To quantitatively assess the effect of diabetes and insulin therapy on the mitochondrial proteome of lumbar DRG, we labeled SC16 immortalized Schwann cells with isotopic forms of lysine (K6) and arginine (R10) and isolated labeled mitochondria to serve as internal standards (Fig. 1A). We examined the quantitative accuracy of this approach by mixing the K6R10:K0R0 mitochondria in ratios of 0.75:1, 1.5:1, and 3:1. The K6/K0 or R10/R0 ratios for individual peptides were obtained from MaxQuant analysis, and a linear response was observed after plotting the average peptide ratio obtained from each mixture against the known mixing ratio (supplementary Fig. 1 in online appendix 1). A 25% decrease in protein expression was quantifiable. Unlabeled (K0R0) DRG mitochondria from the three treatments were then individually mixed in a 2:1 ratio with the K6R10 mitochondria prior to SDS-PAGE and LTQ-FT MS/MS analysis. From more than 43,600 identified peptides, 12,785 SILAC pairs were sequenced and ∼60% identified. After culling out contaminants (n = 30), reverse-decoy hits (n = 13), and proteins identified by only a single unique peptide, we identified 672 proteins, of which 334 (49.6%) were quantified by at least one unique peptide identified in samples from at least two animals (supplementary online Table 1). The median number of quantified ratios for the three treatments was: control (n = 5), diabetic (n = 8), and diabetic + insulin (n = 7). Of the total proteins identified, 206 (30%) were annotated as mitochondrial/glycolytic and 151 were quantified (73%).
To provide a global view of the effect of diabetes and insulin therapy on protein expression, the expression ratios were binned and a frequency distribution assessed (Fig. 1B). In general, diabetes had a more pronounced effect on decreasing protein expression. Insulin therapy induced a rightward shift toward normalizing expression and promoted a significant increase in protein expression. Pathway analysis found that the proteins associated with mitochondrial dysfunction, oxidative phosphorylation, and ubiquinone biosynthesis (primarily complex I proteins) were the most significantly over-represented and showed the greatest percentage of proteins that underwent significant downregulation (Table 2). Consistent with the diabetic phenotype, proteins associated with ketone body biology were also over-represented and diabetes increased the expression of succinyl-CoA:3-ketoacid-CoA transferase one (SCOT), which is critical in acetoacetate clearance.
To determine if diabetes and insulin therapy had a distinct effect on mitochondrial versus nonmitochondrial proteins, the expression ratios for each protein were plotted against each treatment (Fig. 1C). This analysis indicated that diabetes has little effect on the majority of mitochondrial and nonmitochondrial proteins that were quantified (the region between solid and dotted lines). With rare exception, insulin therapy did not decrease protein expression, but led to a significant increase in the expression of numerous nonmitochondrial proteins (green shading). Enrichment analysis of proteins in this region using the Biological Networks Gene Ontology (BiNGO) plugin of Cytoscape found that the cluster frequency for proteins annotated to the biologic process of translation was 36.1%, a sevenfold enrichment. We also noted a small group of proteins that were significantly increased by diabetes but whose expression was unchanged by insulin (blue shading). BiNGO analysis of this subset of proteins indicated that small G protein signaling and protein transport were the enriched processes.
Diabetes caused a statistically relevant change in 27% of quantified mitochondrial proteins, and insulin therapy had an ameliorative effect that, in general, normalized this decrease (Fig. 1C, yellow shading). Consistent with another proteomic study of heart mitochondria (14), bioinformatic analysis found that proteins associated with canonical pathways of mitochondrial dysfunction and oxidative phosphorylation were over-represented and mainly decreased in expression (Table 3). Representative examples from a diabetic animal show a 51% decrease in the complex I protein, NADH dehydrogenase Fe-S protein 3 (NDUFS3) and a 29% decline of Mn superoxide dismutase (Mn-SOD) (Fig. 2A and B). However, insulin therapy improved the deficits in NDUFS3 and Mn-SOD expression (Fig. 2C) as previously characterized using Western blotting (8,16). On the other hand, diabetes did not alter the expression of ATP synthase α (supplementary Fig. 2 in supplementary online appendix 1).
Lumbar DRG from age-matched control and 22-week-old STZ-diabetic rats were analyzed for rates of oxygen consumption as shown in Fig. 3A. Respiratory chain activity, whether coupled or uncoupled, was significantly depressed in diabetic samples. In agreement with the proteomic data and oxygen consumption results, the enzymatic activities of rotenone-sensitive NADH-cytochrome c reductase (complex I) and cytochrome c oxidase (COX; complex IV), as well as the Krebs cycle enzyme, citrate synthase, were significantly decreased in STZ-diabetic rats compared with control (supplementary Table 2).
Adult sensory neurons were cultured for 1 day from age-matched controls and 22-week-old STZ-diabetic rats and loaded with TMRM. This dye was used at a subquench concentration where a decrease in fluorescence signal intensity indicated reduced mitochondrial inner membrane potential (25). The live neurons were exposed to a combination of antimycin A (inhibitor of complex III) and oligomycin (inhibitor of ATP synthase), and the fluorescence signal in axons detected by confocal microscopy. Antimycin A blocks electron transfer leading to mitochondrial depolarization, whereas oligomycin inhibits the ATPase and prevents reverse pumping of protons and associated generation of a proton gradient. Therefore, the mitochondrial membrane potential (and associated proton gradient) is completely dissipated in the presence of both these drugs. In the presence of antimycin A + oligomycin, the rate of mitochondrial depolarization was more rapid in axons of normal neurons compared with diabetic neurons (Fig. 3B–D). This suggests that prior to the addition of antimycin A + oligomycin, the axonal mitochondria were more highly polarized in the normal neurons compared with the diabetic neurons. Mitochondrial physiology was further investigated by treating cultured neurons from control and diabetic rats with oligomycin alone. Blockade of the ATPase results in a buildup of the transmembrane proton gradient and induces hyperpolarization of the mitochondrial inner membrane, as indicated by elevated TMRM fluorescence (Fig. 4A) (26). In normal neurons, a transient hyperpolarization was observed, followed by a recovery due to adaption of the respiratory chain. For example, uncoupling proteins become active and dissipate the proton gradient under a high inner membrane potential (27). Diabetic neurons exhibited a significantly greater level of hyperpolarization upon oligomycin application and the adaptive response was impaired.
We determined if the respiratory chain was contributing to oxidative stress in diabetic neurons by loading cells with the mitochondrially-targeted ROS detector, MitoSOX red. A subset of diabetic neurons was pretreated with oligomycin to hyperpolarize the inner mitochondrial membrane and maximize loading of MitoSOX red into the mitochondrial matrix. Neurons were treated with the uncoupler, carbonylcyanide-p-trifluoromethoxyphenylhydrazone (FCCP), to dissipate the transmembrane electrochemical gradient and enhance the rate of electron transfer. Increased respiratory chain activity leads to augmented electron leakage and associated generation of ROS, primarily superoxide. In normal neurons this was demonstrated with elevated FCCP-induced MitoSOX red fluorescence (Fig. 4F and G). Diabetic neurons, with or without prior oligomycin treatment, exhibited lower MitoSOX red fluorescence intensities indicative of reduced levels of superoxide being generated by the respiratory chain.
Parallel cultures demonstrated elevated oxidative stress in axons of diabetic neurons under 25 mmol/l glucose versus control neurons as exhibited by raised dichlorodihydrofluorescein (DCF) fluorescence and enhanced staining for adducts of 4-HNE (Fig. 5A–F). Subsets of these cultures were treated acutely with the specific SDH inhibitor, SDI-158, to investigate the role of the polyol pathway in ROS production. Figure 5G and H shows that blockade of high glucose-dependent sorbitol production results in reduced ROS generation in axons of diabetic neurons.
The results show that respiratory chain components of the mitochondrial proteome are downregulated in DRG in diabetes and this phenotypic alteration was associated with impairment in respiratory chain activity. In addition, for the first time, this study demonstrates that altered mitochondrial proteome expression is linked to altered mitochondrial physiology in axons of diabetic neurons. And finally, although oxidative stress was present in axons of diabetic neurons, the results show that polyol pathway activity, not aberrant respiratory chain function, contributes to generation of ROS.
We used SILAC to provide a set of culture-derived isotope tags (20) to serve as internal standards for quantifying the effect of diabetes on the composition of the mitochondrial proteome from DRG. One advantage of culture-derived isotope tags is the quantitative accuracy that can be achieved relative to label-free approaches (28), especially for low abundant proteins. Despite our small sample size, a 25% change in expression was sufficient to reach statistical significance, and the number of mitochondrial proteins that exceeded this threshold was similar to that previously reported in mitochondria isolated from heart tissue of diabetic Akita mice (14). Further, the results of our unbiased quantification were in close agreement with those obtained by targeted immunoblot analyses for COX subunit IV, NDUFS3, ATP synthase, and Mn-SOD in two prior studies (8,16).
Similar to a previous gene array study delineating alterations in mRNA expression in DRG from diabetic rats (29), the magnitude of changes observed in the mitochondrial proteins were rather modest and averaged 0.44 ± 0.16-fold in either direction. Interestingly, the gene array study reported that after 2 months of diabetes, no modification occurred in gene expression of enzymes associated with the tricarboxylic acid cycle. We also observed no changes in pyruvate dehydrogenase and in six of eight of the tricarboxylic acid cycle enzymes at the protein level, the exceptions being fumarate hydratase and succinyl Co-A ligase. Similarly, with the exception of hexokinase 1, the remaining glycolytic enzymes were not altered, in agreement with mRNA expression studies at 2 months of diabetes (29). We previously reported that hexokinase 1 localizes to mitochondria of DRG (30) and this protein was reproducibly detected in the heavy mitochondrial fraction of all animals. Interestingly, although the hexokinase gene and protein expression were not modified after 2–3 months of diabetes in two studies (29–30), expression was decreased after 22 weeks of diabetes in the present study. Since this was the only glycolytic enzyme that significantly changed, it is tempting to speculate that its lowered expression also has a function separate from glucose metabolism. In this regard, sensory neurons from diabetic adult animals have an impaired ability to support neurite development (16) and directly inhibiting hexokinase activity blocks neurotrophin-induced neuritogenesis (31).
In the cardiac system, diminished mitochondrial respiratory function caused by diabetes has also been identified by proteomic and gene array techniques (14,32). These broad changes in gene expression could be triggered by altered activity of key upstream regulators. For example, in human skeletal muscle in type 2 diabetes, the transcriptional regulator NRF-1 and the transcriptional coactivator peroxisome proliferator-activated receptor-γ coactivator 1 α (PGC-1α) were downregulated and corresponded with reduced expression of proteins that regulate cellular energy metabolism, including mitochondrial biogenesis and oxidative phosphorylation (33,34). In fact, our preliminary data demonstrated a significant reduction in activity of AMP kinase, a regulator of PGC1-α, in DRG in type 1 diabetic rodents (manuscript in preparation).
Initial exposure to high glucose concentration over 1 to 4 weeks in DRG in diabetic rats is linked to upregulation of glycolytic pathway expression (mRNA) (29). Studies in endothelial or Schwann cells demonstrate that acute exposure to glucose elevates ROS and respiratory chain activity, respectively (2,23). Therefore, in the short term, hyperglycemia triggers enhanced glycolysis and associated respiratory chain activity (and possibly ROS). However, in the longer term, the high intracellular glucose concentration provides an ample supply of ATP via several nonmitochondrial-dependent pathways. Consequently, the metabolic phenotype of the cell adapts and functions in the absence of a dependence on the tricarboxylic acid cycle and oxidative phosphorylation for ATP production, possibly by initiating a process homologous to the “Crabtree effect” (35). Thus, rates of electron donation to the respiratory chain are suboptimal in neurons in long-term diabetic rats and may predispose to lower rates of mitochondrial respiratory chain activity and oxidative phosphorylation. Key metabolic activity sensors and/or regulators such as AMPK and NRF-1 are putative candidates for this modulation, although it is unlikely that subsequently adapted metabolism of glucose is channeled through glycolysis in isolation. In this regard, elevated glucose flux through the aldehyde and aldose reductase pathway could be critical (24,36). For example, studies in lens (37), retina (5), and cardiac tissue (38) in medium- to long-term animal models of type 1 diabetes show that parts of the glycolytic pathway function are depressed.
ROS production linked to enhanced electron leakage from the respiratory chain induced by uncoupling, and theoretically comprising superoxide, was lower in the axons of neurons from diabetic rats (Fig. 4B–E), confirming our mitochondrial physiology and proteomics work. This was also in spite of generally elevated ROS levels in axons (Fig. 5A–F). The studies in Figs. 4 and 5G provide preliminary evidence that the sources of ROS in axons of diabetic neurons are not from aberrant respiratory chain function, but in part from polyol pathway activity. The latter pathway has been proposed as a source of ROS through a putative sorbitol accumulation-dependent NADPH oxidase route in previous studies (24,36). Downregulation of the respiratory chain machinery would be predicted to lead to depolarization of the mitochondrial membrane (Fig. 3B–D), reduced rates of respiratory chain activity (8) (Fig. 3A and supplementary Table 2), and associated diminished electron leakage. The lower rate of loss of polarization status subsequent to uncoupling in Fig. 3C was not the result of resistance to uncoupling in the diabetic neurons since complementary measures of respiratory chain activity show lower rates of electron transfer in diabetic neurons; also, see Fig. 1 in Chowdhury et al. (8). These findings differ from those in cultured endothelial cells where high glucose concentration enhanced mitochondrial membrane potential and induced elevated ROS (2–3). Figure 4A reveals that oligomycin treatment caused a greater level of mitochondrial inner membrane hyperpolarization above baseline in diabetic neurons compared with normal neurons, further highlighting that adult sensory neurons with a history of diabetes and under high glucose concentration behave differently to endothelial cells. The adaption of mitochondria in normal neurons to hyperpolarization was not observed in diabetic neurons, again stressing the aberrant phenotype of mitochondrial physiology. Uncoupling proteins such as adenine nucleotide transporters (ANT1/2) contribute to the dissipation of a high mitochondrial membrane potential (27) and expression was depressed in diabetic mitochondria (supplementary Table 1).
In conclusion, our proteomics data reveal a range of altered expression profiles in the mitochondrial proteome of DRG from diabetic rats. This modified expression pattern was associated with aberrant mitochondrial respiratory chain physiology and function. Under high glucose concentration, the neuron cell body perceives that mitochondrial function can be downgraded; however, this may ignore the unique high-energy requirements of the nerve ending and contribute to distal axon degeneration. For example, growth cone motility that underpins axonal plasticity and regeneration in the skin has an exceedingly high demand for ATP because of significant levels of actin treadmilling (39). Impaired respiratory chain function did not elevate ROS generation, even though oxidative stress was observed in axons. In fact, the lower rates of respiratory chain activity were linked to mitochondrial membrane depolarization, improper adaption to oligomycin-induced membrane hyperpolarization, and reduced levels of superoxide derived from electron leakage during electron transport. In axons of neurons from long-term diabetic rats, sites of ROS production colocalize with the mitochondrial compartment (16,40). Therefore, alternative mitochondrial-related sources of ROS should be considered. For example, NADPH oxidase has been localized to the mitochondrial compartment of kidney cortex and mesanglial cells and mediates elevated ROS under high glucose concentration (41).
This work was supported by grants from the Juvenile Diabetes Research Foundation (#1-2008-280) and the National Institutes of Health to R.T.D. (grants NS-054847 and DK-073594). E.A. was supported by a grant from the National Science and Engineering Research Council (#3311686-06) to P.F. and subsequently by a postgraduate scholarship from the Manitoba Health Research Council. S.K.R.C. and E.Z. were supported by grants to P.F. from the Canadian Institutes for Health Research (#MOP-84214) and the Juvenile Diabetes Research Foundation (#1-2008-193). D.R.S. was supported by a grant to P.F. from the Manitoba Health Research Council. This work was also funded by the St. Boniface General Hospital and Research Foundation.
No potential conflicts of interest relevant to this article were reported.
E.A. and E.Z. contributed equally to the fluorescence imaging experiments described in Figs. 3⇑–5. E.A. performed preparation of mitochondrial samples for proteomic analysis. S.K.R.C. performed the mitochondrial respiration and complex activity studies. D.R.S. was responsible for induction of diabetes and maintenance of all animal groups, analysis of blood glucose/glycated hemoglobin, and dissection of DRG for mitochondrial measurements. R.T.D. designed and performed the proteomic analysis and contributed to writing and editing the manuscript. P.F. designed the animal and tissue culture studies and contributed to writing and editing of the manuscript.
The authors thank Dr. Gordon Glazner, University of Manitoba, and St. Boniface Hospital Research Centre for permitting access to the Carl Zeiss LSM 510.
The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked “advertisement” in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.
- Received June 10, 2010.
- Accepted September 20, 2010.
- © 2011 by the American Diabetes Association.
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