Evaluation of orally active poly(ADP-ribose) polymerase inhibitor in streptozotocin-diabetic rat model of early peripheral neuropathy
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- Li, F., Szabó, C., Pacher, P. et al. Diabetologia (2004) 47: 710. doi:10.1007/s00125-004-1356-0
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Poly(ADP-ribose) polymerase activation depletes NAD+ and high-energy phosphates, activates protein kinase C, and affects gene expression in various tissues. This study was designed to characterise the effects of the potent, orally active poly(ADP-ribose) polymerase inhibitor PJ34 in the Wistar rat model of early diabetic neuropathy.
Control and streptozotocin-diabetic rats were maintained with or without PJ34 treatment (30 mg·kg−1·day−1) for two weeks, after two weeks without treatment. Endoneurial blood flow was assessed by hydrogen clearance; metabolites and high-energy phosphates were assayed by enzymatic spectrofluorometric methods; and poly(ADP-ribose) was detected by immunohistochemistry.
Blood glucose concentrations were increased to a similar extent in untreated and PJ34-treated diabetic rats compared with controls. Intense poly(ADP-ribose) immunostaining was observed in the sciatic nerve of diabetic rats, but not in other groups. Final sciatic motor nerve conduction velocity and digital sensory nerve conduction velocity were reduced by 24% and 22% respectively in diabetic rats compared with controls (p<0.01 for both), and both were 98% corrected by PJ34 (p<0.01 vs diabetic group for both). In contrast, with PJ34 treatment, nerve blood flow showed a modest (17%) increase, and vascular conductance showed a tendency to increase. Free mitochondrial and cytosolic NAD+:NADH ratios, assessed from the glutamate and lactate dehydrogenase systems, phosphocreatine concentrations, and phosphocreatine:creatine ratios were decreased in diabetic rats and essentially normalised by PJ34. In both untreated and PJ34-treated diabetic rats, nerve glucose, sorbitol and fructose were increased to a similar extent. PJ34 did not affect any variables in control rats.
Short-term poly(ADP-ribose) polymerase inhibitor treatment reverses functional and metabolic abnormalities of early diabetic neuropathy. Complete normalisation of nerve blood flow is not required for correction of motor or sensory nerve conduction velocities, provided that a therapeutic agent can restore nerve energy state via direct action on Schwann cells.
KeywordsEnergy state Motor and sensory nerve conduction Nerve blood flow Oxidative and nitrosative stress Peripheral diabetic neuropathy PJ34 Poly(ADP-ribose) polymerase Rat Sorbitol pathway of glucose metabolism Streptozotocin-diabetes
motor nerve conduction velocity
nerve blood flow
sensory nerve conduction velocity
peripheral diabetic neuropathy
protein kinase C
Activation of poly(ADP-ribose) polymerase (PARP) (EC 188.8.131.52), a downstream effector of free radical and oxidant-induced DNA single-strand breakage, plays an important role in a number of pathological conditions associated with oxidative stress, i.e. cardiovascular and neurodegenerative diseases, cancer and inflammation . Growing evidence indicates that PARP activation is an early pivotal mechanism in the pathogenesis of autoimmune diabetes mellitus  and chronic diabetic complications [3, 4, 5]. Activation has been documented in beta cells and tissue sites for diabetic complications in streptozotocin (STZ)-diabetic rats and mice [2, 3, 4, 5], as well as in skin vessels of patients with diabetes mellitus , and it may lead to diabetic complications via several mechanisms. On the one hand, activation of PARP, which cleaves NAD to form nicotinamide and ADP-ribose residues, depletes NAD and ATP (or other high-energy phosphates), which are utilised for NAD regeneration from nicotinamide [1, 3, 5]. NAD depletion results in the inhibition of the glyceraldehyde 3-phosphate dehydrogenase reaction of glycolysis, and in the diversion of the glycolytic flux towards the formation of diacylglycerol, an activator of protein kinase C (PKC), and the formation of methylglyoxal, a precursor of advanced glycation end products . On the other hand, PARP controls activation of a number of transcription factors, i.e. nuclear factor-kappa B, activator protein-1, signal transducer and activator of transcription-1, octamer-1 and p53 protein via direct binding, poly(ADP-ribosyl)ation or both [8, 9]. This, in turn, up-regulates numerous genes [9, 10], including those implicated in the pathogenesis of peripheral diabetic neuropathy (PDN), such as endothelin-1 , cyclooxygenase-2 [12, 13] and inflammatory genes . Thus, PARP activation can be a trigger of multiple mechanisms implicated in diabetes-associated neuropathic changes.
Support for the important role of PARP in PDN was generated by our recent study using PARP-deficient mice and two structurally diverse PARP inhibitors, 3-aminobenzamide and 1,5-isoquinolinediol, in the rat model . However, neither of these are orally active compounds, which makes them unsuitable for chronic experiments. Among other PARP inhibitors, the potent orally active PARP inhibitor PJ34 (the hydrochloride salt of N-(-oxo-5,6-dihydro-phenanthridin-2-yl)-N,N-dimethylacetamide [3, 15]) has been that most extensively studied with regard to diabetic complications [3, 4, 7, 15, 16]. Long-term evaluation of the effect of PJ34 on diabetic retinopathy is in progress (T.S. Kern, personal communication). In contrast to other PARP inhibitors, i.e. nicotinamide and 3-aminobenzamide, PJ34 is highly potent and specific [3, 15], and does not have direct antioxidant properties in concentrations up to 10 mmol/l . This study aimed to evaluate the effects of PJ34 on established functional and metabolic abnormalities of early PDN.
Materials and methods
Unless otherwise stated, all chemicals were of reagent grade quality and were purchased from Sigma (St. Louis, Mo., USA). Methanol (HPLC grade), perchloric acid, hydrochloric acid and sodium hydroxide were obtained from Fisher Scientific (Pittsburgh, Pa., USA). Ethyl alcohol (200 proof dehydrated alcohol, USP punctilious) was purchased from McCormick Distilling (Weston, Mo., USA). We purchased β-d-glucose, sorbitol (NF) and d-fructose (USP) from Pfanstiehl Laboratories (Waukegan, Ill., USA). Reagents for immunohistochemistry were purchased from Vector Laboratories (Burlingdale, Calif., USA).
Male Wistar rats (Charles River, Wilmington, Mass., USA), with body weights of 250 to 300 g, were fed a standard rat chow (PMI Nutrition, Brentwood, Mo., USA) and had free access to drinking water. STZ-diabetes was induced as described previously [5, 17, 18]. Blood samples for measurements of glucose were taken from the tail vein approximately 48 h after the STZ injection, and the day before the animals were killed. The rats with blood glucose concentrations of 13.8 mmol/l or more were considered diabetic. The experimental groups comprised control and diabetic rats with or without PJ34 treatment (30 mg·kg body weight−1·day−1 in the drinking water). The treatment began after the initial two weeks without treatment. The duration of treatment was also two weeks. The experiments were performed in accordance with regulations specified by the National Institutes of Health “Principles of Laboratory Animal Care, 1985 Revised Version” and the University of Michigan Protocol for Animal Studies.
We have previously reported [19, 20] that a number of anaesthetics distort the profile of peripheral nerve metabolites, whereas sedation by a short exposure to CO2 (approximately 15–20 s) with immediate cervical dislocation preserves high-energy phosphate levels in the range of those obtained after decapitation without any narcosis. For this reason, two different sets of animals were used for functional and metabolic studies. The functional studies measured nerve blood flow (NBF), motor nerve conduction velocity (MNCV) and sensory nerve conduction velocity (SNCV). Measurements of MNCV and SNCV were taken at the onset (prior to induction of diabetes) and at the 2-week time point (beginning of interventions) in rats anaesthetised with a mixture of ketamine and xylazine (45 mg/kg body weight and 15 mg/kg body weight respectively, both i.p.). For final NBF, MNCV and SNCV measurements, rats were anaesthetised with inactin (65–85 mg/kg body weight, i.p.). Sciatic MNCV and digital SNCV measurements were taken before the assessment of NBF on the contralateral nerve. In all measurements, body temperature was monitored by a rectal probe and maintained at 37 °C with a warming pad. Hind limb skin temperature was also monitored by a thermistor and maintained between 36 and 38 °C by radiant heat. For metabolic studies, the animals were sedated by CO2 in a specially designed chamber  and immediately killed by cervical dislocation. The left nerves were rapidly dissected, carefully blotted with fine filter paper to remove any accompanying blood, and frozen in liquid nitrogen for subsequent measurements of glycolytic and tricarboxylic acid cycle intermediates and variables of energy state. The right nerves were divided into two parts. Segments of approximately 50 mg were frozen in liquid nitrogen for subsequent measurements of the sorbitol pathway intermediates. The remaining parts were fixed in 10% formalin and later used for immunohistochemistry.
Sciatic endoneurial nutritive NBF was assessed by microelectrode polarography and hydrogen clearance  as we have already described . Nutritive NBF was taken as the slow component of the curve. An average of two measurements at different sites was used to determine nutritive NBF. Sciatic MNCV and hind limb digital SNCV were measured as previously described .
The steady-state concentrations of glutamate, α-ketoglutarate, ammonia, pyruvate, lactate, ATP, phosphocreatine (PCr), creatine (Cr), glucose, sorbitol and fructose were assayed spectrofluorometrically by enzymatic procedures as already described [17, 18, 19, 20]. Free mitochondrial and cytosolic NAD+:NADH ratios were calculated from the steady-state metabolite concentrations and equilibrium constants of the glutamate dehydrogenase and lactate dehydrogenase systems [17, 19].
Assessment of poly(ADP-ribose) immunoreactivity.
All immunohistochemical samples were coded and examined by a single investigator in a blinded fashion. Paraffin-embedded, 5-micron-thick longitudinal sections of sciatic nerve were deparaffinised in xylene and rehydrated in decreasing concentrations of ethanol followed by a 5-min incubation period in PBS. Sections were treated with 0.3% hydrogen peroxide for 15 min to block endogenous peroxidase activity and then rinsed briefly in PBS. Non-specific binding was blocked by incubating the slides for 1 h in 0.25% Triton/PBS containing 2% horse serum. To detect poly(ADP-ribose), a routine histochemical procedure was applied as previously described . Mouse monoclonal anti-poly(ADP-ribose) antibody and isotype-matched control antibody were applied in a dilution of 1:400 for 1 h at room temperature.
The results are expressed as means ± SEM. Data were subjected to equality of variance F test, and then to log transformation, if necessary, before one-way analysis of variance. Where overall significance was attained, individual between-group comparisons were made using the Student-Newman-Keuls multiple range test. Results were considered significant at a p value of 0.05 or less. When between-group variance differences could not be normalised by log transformation (datasets for body weight, plasma glucose and some metabolic parameters), the data were analysed by non-parametric Kruskal-Wallis one-way analysis of variance, followed by the Bonferroni-Dunn test for multiple comparisons.
Body weights and blood glucose concentrations in control and diabetic rats with and without PJ34 treatment
Body weight (g)
Blood glucose (mmol/l)
Control + PJ34
Diabetic + PJ34
Motor nerve and sensory nerve conduction velocities at the onseta and after two weeks in rat experimental groups
After 2 weeks
After 2 weeks
Control + PJ34
Diabetic + PJ34
The diabetes-induced 50% reduction in sciatic endoneurial nutritive NBF was reversed by 67% through PJ34 treatment (Fig. 2c). The diabetes-associated 80% decrease in mean systemic blood pressure was corrected by PJ34 to a level that was not significantly different from control or diabetic rats (Fig. 2d). The diabetes-induced 37% deficit in endoneurial vascular conductance (Fig. 2e), i.e. NBF normalised for blood pressure, tended to increase with PJ34 treatment, but the difference from the untreated group was not statistically significant.
Nerve metabolite concentrations and free mitochondrial and cytosolic NAD+:NADH ratios in control and diabetic rats with and without PJ34 treatment
Control + PJ34
Diabetic + PJ34
Free mitochondrial and cytosolic NAD+:NADH ratios were lower in diabetic rats than in the control group (p<0.01 for both). The decrease in both ratios was essentially corrected by PJ34 (p<0.01 vs untreated diabetic group). PJ34 did not affect the redox state of mitochondrial or cytosolic NAD couples in control rats.
Nerve energy state in control and diabetic rats with and without PJ34 treatment
Control + PJ34
Diabetic + PJ34
Nerve sorbitol pathway intermediate concentrations in control and diabetic rats with and without PJ34 treatment
Control + PJ34
Diabetic + PJ34
“The neuropathic changes are reversible until they affect the phenotype of neurons and Schwann cells” (D. R. Tomlinson, personal communication). The validity of this postulate is supported by numerous reversal studies with inhibitors of aldose reductase  and PKC , with antioxidants  and with other agents, all indicating that consequences of diabetic hyperglycaemia such as increased sorbitol pathway activity, oxidative stress and PKC activation do not cause irreversible changes in the peripheral nervous system, at least in the early stage of PDN. More recently, it has been shown that intervention even further downstream than hyperglycaemia, at the level of oxidative-stress-initiated, mitogen-activated protein kinase signalling cascade, successfully restores normal nerve function . The reversal of functional and metabolic abnormalities of early PDN has been achieved in this study and in our previous study  with several structurally diverse inhibitors of the enzyme PARP, a downstream effector of DNA oxidative damage .
Activation of PARP is a response to increased free radical and oxidant (peroxynitrite) generation  present in neural elements and vasa nervorum of the peripheral nervous system [5, 25]. A number of studies, including those from our group, provide evidence of increased lipid peroxidation [17, 18, 19, 26], impaired oxidative defence [17, 18, 19, 20, 26], and superoxide formation [27, 28] in the peripheral nerve. Furthermore, recent findings [27, 29] indicate increased formation of peroxynitrite, a product of the reaction between superoxide anion radicals and nitric oxide, in experimental models and human subjects with PDN. Studies with the potent peroxynitrite decomposition catalyst FP15 [30, 31] suggest that peroxynitrite is primarily responsible for enhanced poly(ADP-ribosyl)ation in a number of pathological conditions associated with oxidative stress. We have recently found that FP15 administered at the very low dose of 5 mg/kg for one week after two months of untreated STZ-diabetes completely reverses peripheral nerve nitrotyrosine and poly(ADP-ribose) accumulation, as well as MNCV and SNCV deficits of early PDN in the mouse model (I. G. Obrosova and C. Szabó, unpublished).
Poly(ADP-ribose) accumulation, the product of PARP activation, is found in all major tissue sites for diabetic complications, including in the vascular endothelium [3, 4], myocardium , retina [16, 32] and kidney  in rat and mouse models of STZ-diabetes. Recent findings, including those from our group, revealed the presence of diabetes-associated PARP activation in dorsal root ganglion neurons  and endothelial and Schwann cells of the peripheral nerve . Growing evidence implicates PARP in the pathogenesis of chronic diabetic complications including endothelial and myocardial dysfunction [3, 4], peripheral  and autonomic  neuropathy, and early retinopathy [16, 32, 34]. Direct evidence that PARP activation plays a role in diabetic nephropathy is still missing, although we have recently demonstrated that PARP activation is responsible for the overexpression of endothelin-1 and endothelin A and B receptors , the important players in diabetic kidney disease .
In our study, the PARP inhibitor PJ34 essentially normalised MNCV and SNCV deficits and important metabolic abnormalities of early PDN such as free mitochondrial and cytosolic NAD+:NADH ratios, and energy deficiency. All these effects were specific to diabetic animals. In contrast, the effect of PARP inhibitor on nerve perfusion, manifested by a 17% increase in NBF and the absence of a significant increase in vascular conductance, was modest. While studies from several groups [17, 22, 23, 27, 28, 36], including one from our laboratory , suggest that vascular factor plays an important role in MNCV and SNCV deficits in PDN, growing evidence indicates that the aetiology of diabetes-induced nerve dysfunction is far more complex, and involves both vascular and non-vascular mechanisms. In particular, in diabetic and galactosaemic transgenic mice overexpressing aldose reductase (AR) specifically in the Schwann cells of the peripheral nerve under the control of the rat myelin protein zero promoter, there was a significantly greater reduction in MNCV than in the corresponding groups of non-transgenic mice with normal AR content . Nerve function, but not NBF, has been preserved in the normal range in diabetic rats treated with the neurotrophic factor, prosaposin , or with sonic hedgehog protein . All of these effects [37, 38, 39] have been observed in rats and mice with relatively early PDN and diabetes-like galactose-induced neuropathy lacking the signs of nerve demyelination, and are probably related to reversible modifications of the metabolic and neurotrophic state of the neural elements of the peripheral nervous system, i.e. neurons and Schwann cells. In our previous study , use of the vasodilator α1-adrenoceptor antagonist prazosin to prevent diabetes-induced nerve perfusion deficit as manifested by normal vascular conductance failed to preserve normal mitochondrial oxidative capacity. The latter is quite understandable in light of recent findings suggesting the dependence of inner mitochondrial membrane potential on insulin-dependent neurotrophic support , which is likely to be unrelated to the state of perfusion, but which is affected by intracellular oxidative stress [26, 41]. Our present findings demonstrate that inhibition of diabetes-induced PARP activation, which is known to be responsible for NAD depletion [1, 3] and down-regulation of glyceraldehyde 3-phosphate dehydrogenase (or insufficient up-regulation as in the peripheral nerve) , as well as for decreased rates of glycolysis and mitochondrial oxidation , restores normal nerve energy state, the metabolic variable that correlates best with nerve conduction [5, 17, 18, 20]. Unfortunately, the specific mechanisms by which diabetes disrupts electric impulse transmission in the peripheral nerve are not understood, which impedes the investigation of the role of any neuronal or Schwann cell factor, e.g. oxidative stress or poly(ADP-ribosyl)ation in diabetes-associated nerve conduction slowing. Future studies with PARP-antisense oligodeoxynucleotides delivered in viral vectors to specific elements of the peripheral nervous system could further elucidate the role of vascular and non-vascular, i.e. neuronal and Schwann cell, PARP in the pathogenesis of PDN. PARP antisense oligodeoxynucleotides have already been successfully employed by several laboratories [42, 43].
The relation between PARP and the sorbitol pathway of glucose metabolism is interesting in light of some recent developments in the field of diabetic complications. According to the “unifying concept” of diabetic complications , oxidative stress, and in particular mitochondrial superoxide production, is responsible for increased AR activity, formation of advanced glycation end products and activation of PKC. Recently, it has been reported that hyperglycaemia-induced activation of at least two of these mechanisms, i.e. glycation and PKC, is mediated via PARP-activation-linked inhibition of glycolysis associated with increased formation of methylglyoxal and diacylglycerol . The role of PARP in diabetes-induced sorbitol pathway hyperactivity has never been explored. At the same time, growing evidence generated in studies with aldose reductase inhibitors [18, 45, 46] and antioxidants , as well as AR-overexpressing [36, 47] and AR-knockout mice , indicates that AR activation precedes and is largely responsible for enhanced oxidative stress in tissue sites for diabetic complications. Furthermore, a recent study of endothelial cells exposed to high glucose concentrations , and the studies of our group on the peripheral nerve, retina and kidneys of diabetic rats (I. G. Obrosova and P. Pacher, unpublished) suggest that AR is also a key player in peroxynitrite-induced nitrosative stress, which is a major contributor to PARP activation. The fact that PJ34 had no effect on diabetes-associated accumulation of peripheral nerve sorbitol pathway intermediates is consistent with the localisation of PARP downstream from increased AR activity and oxidative-nitrosative stress in the pathogenesis of PDN and other diabetic complications.
In conclusion, this short-term study with the orally active PARP inhibitor, PJ34, saw the reversal of established functional and metabolic abnormalities of early PDN in the STZ-diabetic rat model. Chronic experiments are needed to establish whether PARP inhibitors are effective against demyelination, nerve fibre loss and other indices of advanced PDN, and whether or not long-term suppression of PARP, the enzyme involved in DNA repair , is associated with adverse side effects. If not, it could be a novel approach for the prevention and treatment of diabetic complications.
The study was supported by the American Diabetes Association Research Grant and the National Institutes of Health Grant DK59809-01 (both to I. G. Obrosova), the Juvenile Diabetes Research Foundation Center for the Study of Complications of Diabetes Grant 4-200-421 (to I. G. Obrosova and M. J. Stevens), and the National Institutes of Health Grant HL/DK 71215-01 (to C. Szabó).