Address correspondence and reprint requests to John W. Wiley, MD, University of Michigan General Clinical Research Center, A7007 University Hospital, 1500 E. Medical Center Drive, Ann Arbor, MI 48109–0108, USA. E-mail: email@example.com
We examined the hypothesis that decreased inhibitory G protein function in diabetic neuropathy is associated with increased protein kinase C (PKC)-dependent phosphorylation of the Goα subunit. Streptozotocin-induced diabetic rats were studied between 4 and 8 weeks after onset of diabetes and compared with aged-matched healthy animals as controls. Opioid-mediated inhibition of forskolin-stimulated cyclic AMP was significantly less in dorsal root ganglia (DRGs) from diabetic rats compared with controls. Activation of PKC in DRGs from control rats was associated with a significant decrease in opioid-mediated inhibition of forskolin-stimulated cyclic AMP that was similar to the decrease in inhibition observed in DRGs from diabetic rats. Both basal and PKC-mediated labeling of Goα with 32Pi was significantly less in DRGs from diabetic rats, supporting increased endogenous PKC-dependent phosphorylation of Goα. Probing of immunoprecipitated Goα with an anti-phospho-serine/threonine specific antibody revealed a significant increase in baseline phosphorylation in diabetic DRGs. Activation of PKC produced a significant increase in phosphorylation in control DRGs but no significant increase in Goα in diabetic DRGs. Phosphorylation of PKC-α was increased, PKC-βII was unchanged and PKC-δ decreased in diabetic DRGs. These results suggest that diminished inhibitory G protein function observed in DRGs neurons from diabetic rats involves an isoform-specific PKC-dependent pathway.
Our previous studies indicated that diabetic neuropathy was associated with diminished inhibitory guanine nucleotide-binding (Gi/o) protein function in dorsal root ganglion (DRG) neurons from diabetic rats using direct measurements of opioid receptor-mediated activation of GTPase activity (Hall et al. 2001). Opioid receptors are also coupled to inhibition of adenylate cyclase in a variety of tissues, including neurons (Xie and Lewis 1997; Allouche et al. 1999). Inhibition of adenylate cyclase is mediated by Gα subunits of the Gi/o family (Simonds 1999). It is unknown whether this pathway is affected in diabetic peripheral neuropathy.
The underlying mechanism(s) responsible for impaired inhibitory G protein function in diabetic neuropathy may involve phosphorylation of G proteins by intracellular signaling molecules, such as protein kinase C (PKC) or protein kinase A (PKA) (Katada et al. 1985). Activation of PKC and phosphorylation of the alpha subunit of Gi2 was associated with impaired Gi2-mediated inhibition of adenylate cyclase in hepatocytes from streptozotocin (STZ)-induced diabetic rats (Morris et al. 1996). The existence of similar abnormalities in diabetic neuropathy has not been explored, although previous studies suggest that activation of PKC occurs in diabetic neuropathy and that impaired inhibitory G protein function is associated with increased calcium influx in acutely dissociated DRG neurons obtained from diabetic rats (Hall et al. 1996, 2001; Cameron et al. 1999).
The goals of the current study were: (i) to confirm that diabetic neuropathy is associated with diminished inhibitory G protein function. We evaluated whether opioid-mediated inhibition of forskolin-stimulated cyclic AMP production was decreased in DRGs from diabetic rats compared with controls in the absence and presence of PKC activation; (ii) to assess whether DRGs from diabetic rats demonstrated increased phosphorylation of the Goα subunit via a pathway that involved activation of PKC; and (iii) to examine whether diabetic neuropathy was associated with differential phosphorylation of PKC isoforms in DRG neurons obtained from diabetic rats.
Materials and methods
The studies described in this manuscript were approved by the University Committee on Use and Care of Animals. We employed the streptozotocin (STZ)-induced diabetic rat model in these studies. Many of the abnormalities observed in diabetic peripheral neuropathy in humans are noted in this animal model, including decreased axonal transport, reduced nerve conduction velocity and impaired axon regeneration (Stevens et al. 1994; Biessels et al. 1999). Male Sprague-Dawley rats (Charles River) aged 4–5 months were rendered diabetic by injection with 45 mg/kg STZ (Sigma, St. Louis, MO, USA) as described previously (Stevens et al. 1994; Srinivasan et al. 2000). Age-matched animals injected with vehicle served as controls. Animals injected with STZ were given 10% sucrose in water for 48 h after injection to prevent hypoglycemia and subsequently maintained on an ad lib. diet. Blood glucose levels were monitored daily until induction of diabetes, which usually occurred within 1–3 days, then bi-weekly thereafter. Animals were studied between 4 and 8 weeks after induction of diabetes. Weight and blood glucose were measured on the day of euthanasia.
Isolated thoracic and lumbar DRG neurons were aseptically removed using techniques described previously (Hall et al. 1995). All studies were performed on the same day that the DRGs were removed from the animals.
Cyclic AMP assay
Measurement of cyclic AMP activity was performed using a cyclic AMP [3H] assay kit (Amersham Pharmacia Biotech, Piscataway, NJ, USA; code TRK432) (Tovey et al. 1974). Control and diabetic rat DRGs were treated in vitro with the opioid agonist, [D-Ala(2), N-MePhe(4), Gly(5)-ol]-enkephalin (DAMGO), 1 µm for 5 min, followed by 3 µm forskolin + DAMGO for 25 min in the presence or absence of phorbol esters, 12-O-tetradecanoylphorbol-13-acetate (TPA), 500 nm pre-treatment for 60 min. In some studies, the inactive analog, 4-α phorbol, was used as a control. DRGs were extracted by homogenization in buffer containing 4 mm EDTA. Samples were mixed with assay reagents and placed in scintillation vials for counting. Blank cpm were determined, as were cpm of samples bound in the absence of unlabeled cAMP (Co). After subtracting the blank cpm from Co to give the blank-corrected cpm (Cx), the ratio of Co/Cx was calculated and plotted against pm of cAMP/tube. The latter value was obtained by comparing values against a standard curve generated using serial dilutions of known concentrations of cAMP.
Phosphorylation studies with 32Pi
These studies were patterned after Morris et al. (1996). Minced thoracic and lumbar DRGs from one animal (usually 20–24 ganglia) were pre-incubated in a 1.5 mL tube for 60 min at 37°C in 200 µL minimal essential medium (MEM) supplemented with 2 mCi of [32Pi] (NEN LifeScience, Boston, MA, USA), 2.5% bovine serum albumin (BSA), 2.5 mm CaCl2, 10 mm glucose supplemented with the phosphatase inhibitor beta-glycerophosphate (10 mm; Sigma). In some studies, phorbol ester, phorbol 12, 13-dibutyrate (PDBu, 500 nm for 60 min) ± the membrane-permeable PKC inhibitor NPC-15437 (10 µm) or 8-bromo-cyclic AMP (2 mm for 60 min), were added to the buffer during the incubation period. Some samples were treated with the inactive phorbol, 4α-phorbol (500 nm for 60 min). The DRGs were harvested by centrifugation (12 000 g for 10 s). Lysis buffer [one tablet of proteinase inhibitor-cocktail (Roche, Mannheim, Germany) in 50 mL 20 mm HEPES/100 mm NaCl buffer, plus 0.1% Triton X 100] was added, and the tissue was homogenized to release the proteins.
Immunoprecipitation, gel electrophoresis and autoradiography of Goα
Homogenized DRG tissue was briefly centrifuged to eliminate the cell debris, and the supernatant fluid was treated with anti-Goα polyclonal antibody [Santa Cruz Biotechnology, Santa Cruz, CA, USA; it has no cross-reactivity with other members of the inhibitory G protein (Gi) family], mixed with 10% protein G agarose (Sigma) for purified the Goα. The mixture was incubated for 60 min at room temperature or overnight at 4°C. Immune complexes were collected as protein G agarose pellets by centrifugation (12 000 g for 5 s); the pellets were washed three times in a 20 mm HEPES, 100 mm NaCl buffer (pH 7.2), and were finally re-suspended in the buffer and placed in a boiling water bath for 5 min. Samples were then centrifuged (12 000 gfor 5 s) and the supernatant fluids taken for sodium dodecyl sulfate–polyacrylamide gel electrophoresis (SDS/PAGE). This was performed at 50 mA for 2 h in 10% acrylamide gels. After electrophoresis, gels were dried and subjected to autoradiography. Gels were scanned and analyzed quantitatively using a Molecular Dynamic, ImageQuant System (Bio-Rad Laboratories, Hercules, CA, USA). In some experiments, Giα was immunoprecipitated using a pan anti-Giα antibody at a dilution of 1 : 1000 (Santa Cruz Biotechnology). Immunoprecipitated samples were processed as described above. While validating the immunoprecipitation methodology, we tested (n = 6) for the presence of Goα in the supernatant fluid after centrifugation of the protein G pellets and observed negligible levels, confirming that Goα was reproducibly and reliably bound to the pellets.
Western immunoblot analysis
Western analysis was performed using methods similar to those described previously (Hall et al. 2001). Whole DRGs were homogenized and the protein content was determined using a Lowry assay system (Bio-Rad). Protein (25 µg) was added to each lane. Samples were separated using 10% (for Goα studies) or 7.5% (for PKC studies) polyacrylamide Ready Gel (Bio-Rad) and electrotransfered to a polyvinylidene fluoride (PVDF) microporus membrane. Isoform-specific antibodies to Goα or PKC in 5% non-fat Carnation milk at a dilution factor of 1 : 1000 (unless otherwise stated) were added to the membranes. Secondary antibody conjugated to horseradish peroxidase enhanced chemiluminescence(ECL + Plus, western blotting detection reagents, Amersham Pharmacia Biotech) was used to counterstain the bands. Protein bands were then analyzed using ImageQuant software (Molecular Dynamics, Bio-Rad). For experiments determining the expression of Goα in diabetic and control tissue, purified Goα was used as a standard and results normalized to staining produced by 0.5 µg Goα.
Assessment of phosphorylation of Goα using an anti-phospho-serine/threonine specific antibody
To examine directly whether the alpha subunit of Go undergoes increased phosphorylation in diabetic neuropathy, we probed immunoprecipitated Goα from control and diabetic rats with an anti-phospho-serine/threonine antibody (ChemCon, Temecula, CA, USA; 1 : 2000 dilution). In some experiments, the DRGs were treated with phorbol ester (PDBu, 500 nm, 60 min) to assess the effect of PKC activation on the level of phosphorylation in DRGs from control and diabetic rats. Some tissue samples were treated with the inactive analog, 4-α phorbol, as a control.
Assessment of PKC-α, PKC-βII and PKC-δ phosphorylation in DRGs using anti-phospho-site specific antibodies
These studies were performed using membrane preparations reported previously (Hall et al. 2001). Comparative studies were also performed to examine the level of phosphorylation with immunoprecipitated proteins using isoform specific antibodies and, subsequently, probing the level of phosphorylation with anti-phospho-site specific antibodies. Whole cell proteins (20 µg/sample) were incubated with anti-PKC-α, anti-PKC-βII (Santa Cruz Biotechnology) or anti-PKC-δ (Upstate Biotechnology, Lake Placid, NY, USA), plus protein G beads for immunoprecipitation (IP) (4°C overnight). Purified proteins were loaded on 10% gel after IP, then processed for gel transferring and milk blocking (Carnation). Membranes were exposed to anti-phospho-PKC-α (Ser 657) antibody (1 : 1000), anti-phospho-PKC-βII (Ser 660) antibody (1 : 1000) (Santa Cruz Biotechnology) or anti-phospho-PKC-δ (Thr 505) antibody (1 : 1000, Cell Signaling Technology, Berverly, MA, USA) at 4°C overnight. Samples were subsequently treated with secondary antibody at room temperature for 1 h.
Data were analyzed using an unpaired t-test. Significance was accepted at the p < 0.05 level. Results are presented as mean ± SE.
Animals were studied at 4–6 months of age, 4–8 weeks following induction of diabetes with STZ. The diabetic rats used in the current studies demonstrated similar elevations in blood glucose and reduction in body weight as our previous studies that documented diminished nerve conduction velocity reversed by treatment with insulin (Srinivasan et al. 2000). Blood glucose ranged from 300 to 550 mg/dL in STZ-injected animals. We observed no significant difference in results obtained from rats with diabetes for 4 weeks versus 8 weeks.
Opioid (DAMGO)-mediated inhibition of forskolin-stimulated cyclic AMP production was significantly reduced in DRGs from diabetic rats compared with controls. Treatment with phorbol-ester reversed DAMGO-mediated inhibition of forskolin-stimulated cyclic AMP in control DRGs
Our previous studies suggested that inhibitory G protein (Gi/Go) function was reduced in diabetic neuropathy (Hall et al. 2001). One objective of the current studies was to generate additional evidence that inhibitory G protein function is impaired in diabetic peripheral neuropathy by measuring opiate-mediated inhibition of forskolin-stimulated production of cyclic AMP. It is relevant that the expression of opioid receptors was not altered in DRGs from diabetic rats compared with controls (Hall et al. 2001). Application of the preferential mu-opioid receptor agonist DAMGO (1 µm) inhibited forskolin (3 µm)-induced cyclic AMP production that was significantly decreased in DRGs from diabetic rats compared with controls (Fig. 1a). Basal levels of cyclic AMP were 1.2 ± 0.3 (control) and 1.5 ± 0.5 (diabetic) pm/tube. Treatment with forskolin increased the cyclic AMP levels to 4.8 ± 0.6 (control; n = 8) and 5.1 ± 0.7 (diabetic; n = 8) pm/tube (Fig. 1b). Pre-treatment with the opioid agonist DAMGO decreased forskolin-stimulated cyclic AMP levels by 20 ± 3% in control DRGs (Fig. 1a; n = 8, p < 0.05) but had no significant effect in diabetic DRGs [4 ± 1.8% decrease; not significant (NS); n = 8; Fig. 1b].
Pre-treatment with phorbol ester (TPA, 500 nm for 60 min) reversed opioid-mediated inhibition of forskolin-induced cyclic AMP levels in DRGs from control rats. (Fig. 1a). Treatment with the inactive phorbol ester analog, 4-α phorbol (500 nm for 60 min), had no significant effect on opioid-mediated inhibition of forskolin-stimulated cyclic AMP levels.
Protein levels of Goα in DRG soma from control and diabetic rats were similar
There was no significant difference in the expression of Goα in DRGs from control and diabetic rats when measured by semi-quantitative western blot analysis (Fig. 2a). This indicates that alterations in phosphorylation and function of Go are unlikely to be due to altered levels of the α subunit in diabetic DRGs.
Baseline endogenous phosphorylation of Goα was significantly greater in DRGs from diabetic rats
Endogenous phosphorylation of Goα was assessed by incubating acutely harvested DRGs from control and diabetic rats with 32Pi, and subsequently immunoprecipitating Goα with a specific antibody (Fig. 2b). Since exogenously-administered 32Pi labels phosphorylation sites on Goα not occupied by unlabeled Pi, we interpreted a decrease in labeling with 32Pi as indicating that endogenous unlabeled phosphate groups already occupied more sites. In experiments run in parallel with identical amounts of 32Pi label and protein concentrations, immunoprecipitated Goα in DRGs from diabetic rats demonstrated significantly less labeling with 32Pi (decreased by 40 ± 8%) when compared with non-diabetic controls (n = 5, p < 0.05). Since there was no change in Goα protein levels, this result suggested that the level of endogenous phosphorylation of Goα was significantly increased in diabetes.
Endogenous PKC-dependent phosphorylation of Goα was significantly increased in DRGs from diabetic rats
We next assessed PKC-dependent phosphorylation in DRGs from control and diabetic rats (Fig. 3). Freshly-harvested DRGs from control and diabetic rats were incubated with 32Pi with and without PDBu (500 nm for 60 min). Counts were expressed as a percentage of the untreated controls. Phorbol ester-mediated phosphorylation (32Pi) of Goα in DRGs from control rats was significantly greater than that observed in DRGs from diabetic rats (n = 5, p < 0.05) (Fig. 3a), suggesting that fewer endogenous phosphorylation sites were occupied in control tissue. Treatment with the inactive phorbol analog, 4-α phorbol, had no significant effect. Pre-treatment of DRGs with the membrane-permeable PKC inhibitor, NPC-15437 (10 µm), caused a substantial reduction in PDBu-mediated phosphorylation (32Pi) of Goα (Fig. 3b, p < 0.05), confirming that PDBu-mediated phosphorylation of Goα involved activation of PKC.
Increased phosphorylation of Goα in DRGs from diabetic rats was confirmed using an anti-phospho-serine/threonine specific antibody. Treatment with phorbol ester increased phosphorylation in control DRGs but did not significantly alter phosphorylation in diabetic DRGs
To examine directly whether Goα undergoes increased phosphorylation in DRGs from diabetic rats, we probed the immunoprecipitated alpha subunit of Go from control and diabetic rats using an anti-phospho-serine/threonine specific antibody. The level of phosphorylation of Goα was significantly greater (45 ± 8%, p > 0.05, n = 4) in DRGs from diabetic rats compared with controls (Fig. 4). Treatment with phorbol ester (PDBu, 500 nm for 60 min) caused a significant increase in phosphorylation (35 ± 7%, p > 0.05, n = 4) in control DRGs but did not significantly change the level of phosphorylation in diabetic DRGs. These results provide direct evidence that Goα undergoes increased phosphorylation in diabetic peripheral neuropathy, and that the pathway may involve activation of PKC. Treatment with the inactive phorbol ester analog, 4-α phorbol, had no significant effect on the level of phosphorylation.
Activation of cyclic AMP-dependent protein kinase A (PKA) did not increase phosphorylation of Goα in DRG
It is possible that the increased level of endogenous phosphorylation in diabetic DRGs might be due to other kinases, such as cyclic AMP-dependent PKA. To test whether PKA-mediated phosphorylation was involved, freshly-harvested DRGs from control and diabetic rats were incubated with 8-bromo-cAMP (2 mm for 60 min) in the presence of 32Pi(Fig. 5a). Goα was immunoprecipitated and subjected to electrophoresis. There was no significant change in the level of phosphorylation of immunoprecipitated Goα in DRGs from control or diabetic rats (n = 5). To confirm that PKA was activated in our assay, we tested 8-bromo-cAMP-mediated phosphorylation (32Pi) of Giα in excised rat liver under similar conditions (Fig. 5b). Previous reports indicate that PKA phosphorylates the inhibitory G protein, Giα, in rat hepatocytes (Bushfield et al. 1990). Treatment with 8-bromo-cAMP resulted in a significant (p < 0.05) increase in phosphorylation of Giα (32 ± 3%) over basal levels (n = 4), indicating that the 8-bromo-cAMP treatment conditions used in our assay were sufficient to activate PKA-dependent phosphorylation in liver tissue.
Endogenous phosphorylation of PKC-α was significantly increased in DRGs from diabetic rats
Western blot analysis revealed that protein levels of PKC-α were not significantly different in DRGs from control and diabetic rats (Fig. 6a). However, DRGs from diabetic rats demonstrated a significant fourfold increase in phosphorylation of PKC-α at Ser 657, as measured by a phospho-specific antibody (Fig. 6b).
Endogenous phosphorylation of PKC-βII was not increased in DRGs from diabetic rats
Western blot analysis indicated that protein levels of PKC-βII were not significantly different in DRGs from control and diabetic rats (Fig. 6c). In contrast to PKC-α, phosphorylation of PKC-βII at Ser 660 was not significantly different in DRGs from control and diabetic rats (Fig. 6e).
Endogenous phosphorylation of PKC-δ was decreased in DRGs from diabetic rats
Western blot analysis revealed that protein levels of PKC-δ were not significantly different in DRGs from control and diabetic rats (Fig. 6e). However, DRGs from diabetic rats demonstrated a significant decrease (41 ± 7%) in phosphorylation of PKC-δ (Thr 505), as measured by a phospho-specific antibody (Fig. 6f).
We demonstrated previously that opioid-mediated activation of inhibitory G protein function was significantly impaired in DRGs from diabetic rats (Hall et al. 2001). The diminished efficacy of opioids in diabetes was not likely due to a decrease in opioid receptor number because [3H]-naloxone binding was not affected by diabetes. In this manuscript we have added the following complementary observations regarding inhibitory G protein function in DRGs from control and diabetic rats: (i) opioid-mediated inhibition of forskolin-stimulated cyclic AMP levels in diabetic DRGs was significantly decreased compared with controls; and (ii) activation of PKC resulted in decreased opioid-mediated inhibition of forskolin-stimulated cyclic AMP levels in control DRGs but did not significantly change the attenuated effect of opioid application in diabetic DRGs. These observations provide additional evidence that diabetes is associated with impaired inhibitory G protein function, and that activation of PKC reproduces in control DRGs the abnormalities in opioid function observed in diabetic DRGs.
We hypothesized that the decreased inhibitory G protein function in diabetic peripheral neuropathy involved increased phosphorylation of Goα via a PKC-dependent pathway. The following observations support this hypothesis.
(I) Protein levels of Goα were similar in DRGs from control and diabetic rats.
(II) Baseline labeling of Goα in the presence of 32Pi was significantly less in DRGs from diabetic rats compared with controls, implying that more sites were occupied by endogenous phosphorylation in diabetic rats. As the level of Goα was unchanged, it is unlikely that this result was due simply to altered expression of Go.
(III) Phorbol ester-mediated phosphorylation of Goα in the presence of 32Pi was significantly less in DRGs from diabetic rats compared with controls. Phorbol ester-mediated phosphorylation of Goα was prevented by the membrane-permeable PKC inhibitor, NPC-15437, supporting the specific involvement of a PKC-dependent pathway.
(IV) Direct assessment of phosphorylation of immunoprecipitated Goα using an anti-phospho-serine/threonine specific antibody revealed that the baseline phosphorylation was significantly increased in diabetic DRGs compared with controls. Treatment with phorbol ester increased the level of phosphorylation of Goα in control DRGs but did not have a significant effect in DRGs from diabetic rats.
(V) Increased phosphorylation was not likely the result of PKA-mediated effects, as treatment of DRGs with 8-bromo-cyclic AMP was not associated with a significant increase in phosphorylation of Goα in the presence of 32Pi, whereas phosphorylation of hepatocyte Giα was increased.
(VI) DRGs from diabetic rats demonstrated increased phosphorylation of PKC-α, no change in phosphorylation of PKC-βII and decreased phosphorylation of PKC-δ. The protein levels of these three isoforms were unchanged in DRGs from diabetic rats compared with controls. This last observation suggests that diabetic peripheral neuropathy is associated with differential activation of PKC isoforms.
Our results suggest that diabetes mellitus may have region-specific effects on neuronal function. For example, opioid-mediated G-protein activation in the pons and medulla were unaltered in STZ-induced diabetic mice and the non-obese diabetic mouse model, despite an attenuation of opioid effect on tail flick response to pain (Ohsawa et al. 1999; Pieper et al. 2000). This discrepancy could be explained by differences between rats and mice in metabolic pathways affected by diabetes, or the relatively modest changes occurring in CNS function in early diabetes mellitus when compared with peripheral nerve function (Biessels et al. 1999).
Heterotrimeric G proteins are an integral component of post-receptor signal transduction (Birnbaumer et al. 1990). The specific functions of the heterogeneous α and β/γ subunits of Gi/Go are an active area of investigation. Inhibitory G protein alpha subunits combine with effector sites on the intracytoplasmic domain of specific receptor populations that are coupled to Gi/Go (Iiri et al. 1998). The Gα subunits also regulate activation of adenylate cyclase (Simonds 1999). Inhibitory β/γ subunits modulate calcium channel function by combining with an effector site on the 1–11 intra-cytoplasmic loop of the voltage-gated calcium channel (De Waard et al. 1997; Garcia et al. 1998). G proteins are themselves targets for modulation of function by intracellular proteins that regulate G protein stimulation (RGS) under physiological and pathophysiological conditions (Huailing and Neubig 2001). Our results suggest that inhibitory G protein function in DRGs can also be regulated by activation of PKC.
Reports of the direction and magnitude of changes in total PKC in diabetic neuropathy have been conflicting, with some investigators reporting increased levels of expression and/or activation, and other investigators reporting opposite results (Cameron et al. 1999; Ways and Sheetz 2001). Much of the controversy can be explained by either tissue-specific changes in the levels of PKC, and/or the likelihood that diabetes differentially affects the expression and/or activity of PKC isoforms. A previous report suggested that the STZ-induced diabetic rat demonstrated enhanced phosphorylation of hepatocyte Gi2α exclusively at PKC-dependent sites (Morris et al. 1996). This could result from increased PKC activity, a decrease in phosphatase activity, or a combination of both. We have not identified the specific amino acids on the alpha subunit of Go in DRGs that undergo increased phosphorylation in diabetic neuropathy. Phorbol ester-mediated activation of protein kinase C was associated with phosphorylation at Ser 144 on Gi2α in hepatocytes from diabetic rats that correlated with a decrease in GTP-dependent inhibition of adenylate cyclase (Bushfield et al. 1990; Morris et al. 1996).
Our observation that diabetes had differential effects on PKC isoforms has support from other reports. Differential expression of PKC isoforms in sciatic nerve and spinal cord of diabetic rats has been reported (Roberts and Mclean 1997). PKC-α isoform translocated from cytosolic to particulate fraction, while levels of PKC-βII isoform were reduced in the cytosolic fraction, and the βI and γ-isoforms were unaffected. Increased PKC activity has been implicated in the pathogenesis of other diabetic complications, including retinopathy and nephropathy (Ways and Sheetz 2001). In contrast, Mathew et al. (1997) observed that the level of PKC-α in sciatic nerve from the Zucker diabetic fatty rat (a model of type 11 diabetes) was significantly reduced. We detected no changes in the protein levels of immunoreactive PKC-α, -βII or -δ in DRGs from diabetic rats using semi-quantitative western blot analysis. However, we did observe a marked increase in phosphorylation of immunoprecipitated PKC-α, no change in PKC-βII and a decrease in PKC-δ using anti-phospho-site specific antibodies. These observations provide support that PKC isoforms are differentially activated in diabetic peripheral neuropathy. The anti-phospho-specific PKC-α antibody we employed recognizes phosphorylated Ser 657, the PKC-βII antibody recognizes phosphorylated Ser 660 and the PKC-δ antibody recognizes Thr 505. Phosphorylation of PKC-α at Ser 657 appears to control accumulation of active enzyme and contributes to its phosphatase-resistant state (Bornancin and Parker 1996). Phosphorylation of PKC-βII at Ser 660, part of the conserved carboxyl-terminal hydrophobic motif, regulates the catalytic and regulatory domains of PKC that are associated with higher affinity binding of ATP and Ca2+ (Edwards and Newton 1997). Phosphorylation of PKC-δ at Thr 505 (part of the activation loop) does not appear to be a requirement for basal or activator-dependent enzymatic activity but may contribute to enzyme activation along with phosphorylation of the adjacent residue Tyr 512 (Konishi et al. 2001). Our results with PKC-δ are similar to those of Sakaue et al. (2003) who observed that the level of phosphorylated PKC-δ, but not total PKC-δ, decreased in DRGs from diabetic rats. Additional studies will be required to clarify whether other known isoforms of PKC are differentially expressed and activated in this model of diabetic neuropathy. For example, Cesare et al. (1999) observed specific involvement of PKC-ε in sensitization of the neuronal response to painful heat. It is noteworthy that this group did not observe expression of PKC-α in DRGs obtained from 3- to 5-day-old neonatal rats using an antibody from Life Technologies (Gibco). In contrast, Khasar et al. (1999) did identify PKC-α in mouse DRGs using the same antibody as the one we employed from Santa Cruz Biotechnology.
Our results suggest that the pathway mediating impaired inhibitory G protein function in diabetic peripheral neuropathy involves activation of PKC and phosphorylation of the alpha subunit of Go. The PKC-dependent pathway may involve direct or indirect phosphorylation of Goα. Previous studies support phorbol ester-mediated phosphorylation of Gi2α in intact acutely-harvested hepatocytes from diabetic STZ rats (Morris et al. 1996). However, this study did not examine whether PKC was acting directly or indirectly to phosphorylate Gi2α. Kozasa and Gilman (1996) observed that catalytic PKC directly phosphorylates G12α and Gzαin vitro, but neither Goα nor Gi2α were targets for phosphorylation by PKC. It is possible that additional pathways may be involved in PKC-dependent phosphorylation of Goα. Exposure to phorbol esters activates the mitogen-activated phosphorylation (MAP) kinase pathway and extracellular signal-regulated kinases in several tissues, including neurons (Stariha and Kim 2001). It is not known whether either selective activation of MAP kinase is associated with phosphorylation of Goα or blockade of this pathway affects PKC-dependent phosphorylation of Goα. It is noteworthy that using the Scansite consensus searching method with high stringency, neither G protein alpha o subunit (rGNAO) nor G protein alpha i1 subunit (GNAI1) demonstrate consensus PKA or PKC sites. This suggests that PKC may be acting indirectly to phosphosphorylate Goα.
In summary, we have presented a body of data in support of the interpretation that impaired inhibitory G protein function in diabetic neuropathy involves a pathway that includes activation of PKC and phosphorylation of the Goα subunit. These observations may provide a mechanistic basis for the increase in calcium influx observed in diabetic peripheral neuropathy and suggest potential targets for therapeutic interventions (Ahlgren and Levine 1994; Nakamura et al. 1999; Carter 2000).
We thank Suquing Wang for her expert technical assistance. These studies were supported by NIH grants RO145820 and R01 56997 to JWW.