Therapeutic Benefit of Extended Thymosin β4 Treatment Is Independent of Blood Glucose Level in Mice with Diabetic Peripheral Neuropathy
Peripheral neuropathy is a chronic complication of diabetes mellitus. To investigated the efficacy and safety of the extended treatment of diabetic peripheral neuropathy with thymosin β4 (Tβ4), male diabetic mice (db/db) at the age of 24 weeks were treated with Tβ4 or saline for 16 consecutive weeks. Treatment of diabetic mice with Tβ4 significantly improved motor (MCV) and sensory (SCV) conduction velocity in the sciatic nerve and the thermal and mechanical latency. However, Tβ4 treatment did not significantly alter blood glucose levels. Treatment with Tβ4 significantly increased intraepidermal nerve fiber density. Furthermore, Tβ4 counteracted the diabetes-induced axon diameter and myelin thickness reductions and the -ratio increase in sciatic nerve. In vitro, compared with dorsal root ganglia (DRG) neurons derived from nondiabetic mice, DRG neurons derived from diabetic mice exhibited significantly decreased neurite outgrowth, whereas Tβ4 promoted neurite growth in these diabetic DRG neurons. Blockage of the Ang1/Tie2 signaling pathway with a neutralized antibody against Tie2 abolished Tβ4-increased neurite outgrowth. Our data demonstrate that extended Tβ4 treatment ameliorates diabetic-induced axonal degeneration and demyelination, which likely contribute to therapeutic effect of Tβ4 on diabetic neuropathy. The Ang1/Tie2 pathway may mediate Tβ4-induced axonal remodeling.
Diabetes affects an estimated 346 million people worldwide . Peripheral neuropathy is a long-term complication of diabetes mellitus which is associated with neurotrophic changes, degeneration, and demyelination of peripheral nerves [2, 3]. There is currently no effective treatment for preventing the development or reversing the progression of diabetic neuropathy. Thus, it is imperative to develop therapies for diabetic peripheral neuropathy.
Thymosin β4 (Tβ4), a major intracellular G-actin-sequestering 43-amino acid peptide, has multiple biological functions . Tβ4 promotes axonal regeneration and remyelination as well as vasculogenesis [5, 6]. Preclinical studies have found that treatment with Tβ4 improves neurological function outcome after central and peripheral nervous system damage [5–7]. We previously demonstrated the fact that Tβ4 remarkably improved sciatic nerve vascular function and peripheral nerve function in a model of diabetic peripheral neuropathy . However, the extended therapeutic effect of Tβ4 on axonal remodeling has not been investigated.
The angiopoietins (Ang), a family of endothelial cell growth factors, regulate vessel angiogenesis and stabilization [8, 9]. Ang1 also promotes neurite outgrowth in cultured dorsal root ganglion neurons and neuronal differentiation in neural progenitor cells [10, 11]. Overexpression of Ang1 in the brain alters neuronal dendrite configuration . Tβ4 treatment of diabetic peripheral neuropathy reverses diabetes-reduced Ang1 expression in the sciatic nerve and thereby promotes vascular remodeling .
Diabetic peripheral neuropathy is a chronic disease. In the present study, we investigated the efficacy and safety of Tβ4 for the extended treatment of diabetic peripheral neuropathy. We found that extended Tβ4 treatment ameliorates diabetic-induced intraepidermal nerve fiber and sciatic nerve impairment, which likely contributes to functional recovery of diabetic neuropathy. In addition, our data indicate that the Ang1/Tie2 pathway may mediate Tβ4-induced axonal regeneration and remyelination in diabetic neuropathy. Thus, extended Tβ4 treatment may represent a safe and effective therapeutic approach for experimental diabetic neuropathy.
2. Material and Methods
All experimental procedures were carried out in accordance with the NIH Guide for the Care and Use of Laboratory Animals and were approved by the institutional Animal Care and Use Committee of Henry Ford Hospital. Male BKS.Cg-m+/+Leprdb/J (db/db) mice (Jackson Laboratories, USA) aged 24 weeks were used. Age-matched heterozygote mice (db/m), a nonpenetrant genotype (Jackson Laboratories), were used as the control animals.
2.2. Tβ4 Treatment
db/db mice at age of 24 weeks were treated with Tβ4 at a dose of 30 mg/kg (RegeneRx Inc., USA, intraperitoneal injection, i.p.), daily for 16 weeks (/group). db/db mice (/group) of the same age were treated with same volume of saline and were used as a control group. Age-matched db/m mice, treated with saline (/group), were used as additional control groups. All mice were sacrificed 16 weeks after onset of treatment. Doses of Tβ4 were selected based on published studies .
Blood glucose levels were measured from the mouse tail vein by using an instant check meter (Roche Diagnostics, USA). Electrophysiological measurements, functional tests, blood glucose levels, and body weight were performed before treatment and then every 4 weeks until sacrifice. All procedures and analyses were performed by investigators who were blinded to the experimental group.
2.3. Neurophysiological Measurements
Sciatic nerve conduction velocity was assessed with orthodromic recording techniques, as previously described [13–15]. Briefly, mice were anesthetized with ketamine/xylazine (i.p., 100/10 mg/kg). The stimulating electrodes were plated at the knee and sciatic notch. Triggered single square wave current pulses were delivered using an isolated pulse stimulator (Model 2100, A-M Systems, USA). The simultaneous electromyographies were recorded by two sterilized electrodes placed in the dorsum of the foot with a Grass Amplifier (Model P5, Grass Instruments, USA). During the measurements, animal rectal temperature was kept at °C using a feedback controlled water bath. Motor nerve conduction velocity (MCV) and sensory nerve conduction velocity (SCV) were calculated according to a published study .
2.4. Measurement of Thermal Sensitivity
To examine the sensitivity to noxious heat, plantar test was measured using a thermal stimulation meter (IITC model 336 TG combination tail-flick and paw analgesia meter; IITC Life Science, USA) according to published methods . Briefly, mice were placed within a plexiglass chamber on a transparent glass surface and allowed to acclimate for at least 20 min. The meter was activated after placing the stimulator directly beneath the plantar surface of the hind paw. The paw-withdrawal latency in response to the radiant heat (15% intensity, cut-off time 30 sec) was recorded. At least five readings per animal were taken at 15 min intervals, and the average was calculated .
2.5. Tactile Allodynia Test
To examine tactile allodynia, we employed Von Frey filaments (Stoelting, USA) to stimulate paw withdrawal according to published protocols [17, 18]. Briefly, a series of filaments with force that ranged from 0.4 to 6.0 g were applied to the plantar surface of the left hindpaw with pressure causing the filament to buckle. A paw withdrawal in response to each stimulus was recorded and a 50% paw withdrawal threshold was calculated according to a published formula [17, 18].
2.6. Staining Myelin Sheets
The sciatic nerves were harvested at the mid-thigh level and fixed in the 2.5% glutaraldehyde and 0.5% sucrose (Sigma, USA) on PBS buffer for 6–8 hours and then immersed in 2% osmium tetroxide (Sigma) for 2 hours. The specimens were then dehydrated with numerous alcohol passages and embedded in paraffin . Semithin transverse sections (2-μm thick) were cut and stained with 1% toluidine blue and three semithin sections per mouse were analyzed.
The sciatic nerves were fixed in 4% paraformaldehyde for immunohistochemistry and then embedded in paraffin according to a published protocol . Three cross sections (6-μm-thick) or three longitudinal sections (6-μm-thick) at 60 μm apart per animal were used .
Epidermal foot pads from left hind feet were fixed in Zamboni’s fixative for 2 hours, washed in PBS, and then kept in 30% sucrose/PBS overnight at 4°C. The samples were embedded in OCT compound and stored at −80°C. Three longitudinal 20-μm-thick footpad sections from each mouse were prepared.
The following primary antibodies were used: polyclonal rabbit anti-myelin basic protein (MBP, 1 : 400, Dako Denmark, USA), polyclonal antineurofilament, heavy chain (NF-H, 1 : 1000, Thermo Scientific, USA), polyclonal rabbit anti-Ang1 (1 : 2000; Abcam, USA), polyclonal rabbit anti-S100 (1 : 400, Abcam, USA), and polyclonal rabbit anti-protein gene product 9.5 (PGP 9.5, 1 : 1,000; MILLIPORE, USA). Rabbit or goat IgG was used as a negative control. Sections were counterstained with 4′,6-diamidino-2-phenylindole (DAPI) (1 : 5000, Thermo Scientific, USA).
2.8. Image Acquisition and Quantification
Image analysis was performed using a computer imaging analysis system (MicroComputer Imaging Device, MCID, Imaging Research Inc., UK) .
For morphometric analysis of sciatic nerves, three sections spaced as 60 μm interval for each staining were used for analysis from each mouse, and three fields of the view per section were randomly imaged under a 100x oil immersion objective (BX40; Olympus Optical, Japan). Myelinated fiber diameter, axon diameter, and myelin sheath thickness were measured. The -ratio (the quotient axon diameter/fiber diameter) was calculated to measure the degree of myelination. At least 200 myelinated fibers were measured per animal [13, 21].
Intraepidermal nerve fiber profiles were digitized under a 40x objective (Carl Zeiss Axiostar Plus Microscope, USA) via the MCID system. The number of nerve fibers crossing the dermal-epidermal junction was counted and the density of nerves is expressed as fibers/mm length of section . Representative images of intraepidermal nerve fibers were obtained by a laser-scanning confocal microscope (Zeiss LSM 510 NLO, Carl Zeiss, Germany).
For quantization of MBP, NF-H, and Ang1 immunoreactive, cross sections or longitudinal sections were digitized. Data are presented as the percentage of immunoreactive area within the total imaged area.
All analysis was conducted with the examiner who was blinded to the identity of the samples being studied.
2.9. Cell Culture
A normal glucose medium (NG) was defined as a medium containing 5 mM glucose, while a high glucose medium (HG) was referred to as a medium containing 30 mM glucose, which was chosen to match glucose levels prevalent in uncontrolled diabetic patients . These glucose concentrations have been used for the in vitro hyperglycemia experiments by others [24, 25].
To examine the effect of Tβ4 on Schwann cells, primary mouse Schwann cells (MSCs) were cultured according to the manufactures’ instructions (ScienCell Research Laboratories, USA).
2.10. Conditioned Media
To collect conditioned medium from MSCs, 2.5 × 106 cells were plated onto a 100-mm-diameter dish in 10 mL of defined medium. The cells were cultured under the normal glucose or high glucose conditions in the presence or absence of Tβ4 (100 ng/mL) for 48 hours. The supernatant (conditioned medium) was collected, concentrated 10 times using 10 kD centrifugal filters (Amicon Ultra-15; Nihon Millipore, USA), and frozen at −80°C until use.
2.11. Primary Culture of DRG Neurons and Evaluation of Neurite Outgrowth
DRG neurons were harvested from 18–20 weeks diabetic db/db mice and nondiabetic db/m mice. Cultures were prepared according to a previously described procedure [26, 27] with some modifications. Briefly, DRG neurons were removed stripped of meninges and dissociated by a combination of Ca2+- and Mg2+-free Hanks balance salt solution (HBSS) containing 0.125% trypsin and 0.1% collagenase–A digestion for 30 min, and then mechanically triturated for ~20 times. Isolated DRG neurons were seeded on glass coverslips coated with laminin and plated at a density of 2,000 cells/well in a 24 well-plate in Neurobasal-A medium (Invitrogen, USA), 2% B-27 (GIBCO, USA), 2 mM GlutaMax, and 1% antibiotic-antimycotic. To evaluate the direct effect of Tβ4 on neurite outgrowth of DRG neurons, DRG neurons were cultured in DRG culture medium with or without Tβ4 (100 ng/mL) under normal glucose and high glucose condition. To evaluate the effects of conditional medium harvested from Tβ4 activated Schwann cells on neurite outgrowth, DRG neurons were cultured in DRG culture medium with one-tenth of the conditioned medium. After a 3-day culture, DRG neurons were performed for NF-H with Cy3 for neurite outgrowth measurement. To trace the neurite outgrowth of fluorescently labeled neurons, the fluorescent photomicrographs were captured at 20x magnification with a digital camera. Neurite outgrowth was measured in 20 neurons per coverslip. The total neurite lengths of each positive neuron were measured using MCID analysis system . The average length of neurite outgrowth was presented.
2.12. Schwann Cell Proliferation and Migration
To investigate the effect of Tβ4 on Schwann cell proliferation, Schwann cells were seeded in a 24-well dish at a density of 1 × 104 cells/well and incubated in normal and high glucose with Tβ4 at concentration 100 ng/mL for 72 hours. BrdU (10 μmol/L) was added 12 hours prior to termination of the experiments. The cells were fixed for BrdU immunostaining. The number of BrdU positive cells was counted in 5 fields of view under a 20x objective.
To examine the effect of Tβ4 on migration of mouse Schwann cells, a modified Boyden’s chamber assay was employed, as described previously . Briefly, the polycarbonate filter (8 μm pore size) (Neuro Probe Inc., USA) was coated with 50 μg/mL fibronectin (Chemicon, USA) and 0.1% gelatin (Sigma) and placed between upper and lower chambers. The cells were preincubated in normal and high glucose levels with Tβ4 at concentration of 100 ng/mL in the presence or absence of the anti-Tie2 inhibitor (5 μM) for 72 hours. Cell suspensions (5 × 104 cells per well) were placed in the upper chamber, and the lower chamber was filled with medium containing human recombinant nerve growth factor (100 ng/mL, R&D Systems). The chamber was incubated for 5 hours at 37°C and 5% CO2. Migrating cells caught in the membrane were then stained using hematoxylin and eosin (Anatech LTD, USA). The number of cells that migrated through the filter was counted in 5 fields of view under a 40x objective.
2.13. Lactate Dehydrogenase (LDH) Cytotoxicity Assay
To determine cytotoxicity levels, the CytoTox 96 Non-Radioactive Cytotoxicity Assay kit (Promega, USA) was used following standard protocol. LDH levels were measured after 48-hour incubation period and LDH activity was detected by a plate reader at OD 490 nm. Data are presented as percentage of LDH level in the media to total LDH [9, 28].
2.14. Elisa Assay
To examine the effect of hyperglycemia on Ang1, Ang1 levels in supernatants were measured using an Elisa specific to detect mouse Ang1 according to the manufacturer’s instructions (http://www.mybiosource.com/, USA).
2.15. Western Blot Analysis
Western blot was performed according to published methods . Briefly, equal amounts of proteins were loaded on 10% SDS-polyacrylamide gel. After electrophoresis, the proteins were transferred to nitrocellulose membranes, and the blots were subsequently probed with the following antibodies: polyclonal rabbit anti-Ang1 (1 : 1000; Abcam). For detection, horseradish peroxidase-conjugated secondary antibodies were used (1 : 2000) followed by enhanced chemiluminescence development (Pierce, USA). Normalization of results was ensured by running parallel Western blot with β-actin antibody. The optical density was quantified using an image processing and analysis program (Scion Image, USA).
2.16. Statistical Analysis
For functional tests, data were evaluated for normality. Ranked data or nonparametric approach will be considered if the data are not normally distributed. The repeated measure analysis of variance (ANCOVA) was considered with dependent factor of time and independent factor of groups. The analysis started testing for group by time interaction, followed by the testing the main effect of group and subgroup analyses. Two-sample -test or analysis of variance (ANOVA) was used to study the group difference on immunostaining, biochemistry, and Western blot, respectively. The data are presented as mean ± SE. A value of was taken as significant.
3.1. Extended Tβ4 Treatment Improves Neurological Functional Outcome in Diabetic db/db Mice
Diabetic peripheral neuropathy is a chronic disease. We first test whether extended, that is, 16 weeks, Tβ4 treatment improves neurological function in diabetic neuropathy. Electrophysiological recording showed that treatment of db/db mice aged 24 weeks with Tβ4 (30 mg/kg) for 16 weeks significantly improved the MCV and SCV in the sciatic nerve compared with db/db mice treated with saline (Figures 1(a) and 1(b)). This increase in MCV and SCV started 4 weeks after treatment and persisted for 16 weeks during treatment, which was associated with substantial improvement in response to sensory function measured by the thermal and mechanical latency with plantar tests and tactile allodynia test, respectively (Figures 1(c) and 1(d)). Treatment with Tβ4 did not significantly alter blood glucose levels but increased animal body weight (Tables 1 and 2). These data indicate that extended Tβ4 treatment improves neurological outcomes without alteration of blood glucose levels.
(c) Plantar Test
(d) Von Frey Test
3.2. Extended Tβ4 Treatment Promotes Axonal Regeneration and Remyelination in Peripheral Nerves
To examine whether the extended Tβ4 treatment affects distal nerve fibers, morphometric changes of nerve fibers were analyzed. Compared to nondiabetic db/m mice, diabetic db/db mice at age of 40 weeks exhibited substantial reduction of PGP 9.5 positive IENFs which is consistent with published studies showing loss of distal sensory nerve fibers in db/db mice and in patients with type II diabetes [31–33]. However, age-matched db/db mice treated with extended Tβ4 did not show significant reduction of IENFs compared to nondiabetic mice (Figure 2). Using toluidine-blue stained thin sections, we further analyzed morphometric changes of the sciatic nerve. Diabetic db/db mice treated with saline showed significant reduction in sciatic nerve fiber diameter and myelin sheath thickness and a significant increase in -ratio (axon diameter/fiber diameter). In contrast, extended Tβ4 treatment completely reversed the sciatic nerve morphology changed by diabetes to levels comparable to nondiabetic db/m mice (Table 3 and Figures 3(a) to 3(c)). Moreover, double immunofluorescent staining showed that extended Tβ4 treatment significantly increased the number of NF-H positive sciatic nerves and MBP positive myelination (Figures 3(d) to 3(h)). Collectively, these data suggest that extended Tβ4 treatment enhances myelinated sciatic nerves and IENFs in diabetic mice.
3.3. Tβ4 Increases DRG Neuron Neurite Outgrowth and Schwann Cell Proliferation and Migration
To investigate the direct effect of Tβ4 on DRG neurons, a widely used in vitro model of primary DRG neurons was employed . Under a regular glucose condition (5 mM glucose) which is comparable to a normal plasma glucose level measured in vivo, DRG neurons harvested from diabetic db/db mice at age of 18–20 weeks exhibited considerable reduction of neurite outgrowth compared to age-matched DRG neurons from nondiabetic db/m mice, whereas addition of Tβ4 into DRG neurons from db/db mice significantly promoted neurite growth (Figure 4). These data suggest that diabetic DRG neurons are not able to grow their fibers even under a normal glucose condition, while Tβ4 can promote neurite growth of these diabetic DRG neurons. We then cultured DRG neurons harvested from nondiabetic mice under a high glucose condition (30 mM) and found that high glucose conditions blocked neurite growth, whereas Tβ4 suppressed high glucose-induced inhibitory effect on neurite outgrowth (Figure 4). These data further support that Tβ4 can enhance neurite growth of DRG neurons under hyperglycemia conditions. Reduction of Schwann cells affects myelination . We thus examined whether high glucose affects Schwann cell survival and proliferation. High glucose did not significantly affect Schwann cell survival measured by LDH assay ( versus in NG). However, high glucose significantly decreased the number of BrdU positive Schwann cells (Figures 5(h), 5(i), 5(j), 5(k), 5(l), and 5(n)). Moreover, a Boyden chamber assay revealed that high glucose decreased Schwann cell migration (Figure 5(o)). However, addition of Tβ4 in the presence of high glucose significantly attenuated the inhibitory effect of the high glucose on Schwann cell proliferation and migration (Figures 5(i), 5(j), 5(n), and 5(o)). These data suggest that, in addition to DRG neurons, Tβ4 promotes Schwann cell proliferation and migration under hyperglycemia condition.
3.4. Tβ4 Activated Schwann Cells Promote DRG Neuron Neurite Outgrowth
Schwann cells provide a microenvironment favoring axonal regeneration in the peripheral nervous system . We then investigated whether Tβ4 activated Schwann cells secrete soluble factors that consequently improve DRG neurite outgrowth. DRG neurons harvested from nondiabetic db/m mice or diabetic db/db mice were incubated with conditioned media collected from Schwann cells that were cultured under regular and high glucose conditions with or without Tβ4. Compared to the conditioned medium collected from Schwann cells cultured under regular glucose condition, the conditioned medium derived from Schwann cells cultured under high glucose condition resulted in significant suppression of neurite outgrowth of DRG neurons derived from nondiabetic mice. In contrast, the conditioned medium collected from Schwann cells treated with Tβ4 under high glucose condition promoted neurite outgrowth in nondiabetic DRG neurons (Figures 5(a), 5(b), 5(c), and 5(m)). Moreover, the conditioned medium collected from Schwann cells treated with Tβ4 under normal glucose condition promoted neurite outgrowth in diabetic DRG neurons (Figures 5(e), 5(f), and 5(m)). These data suggest that soluble factors secreted by Schwann cells interact with DRG neurons in mediate neurite outgrowth.
We previously demonstrated that a proangiogenic protein, Ang1, plays an important role in mediating development of diabetic sciatic nerve damage . We thus examined whether Ang1 is involved in interaction between Schwann cells and DRG neurons to develop diabetic neuropathy. Consistent with our previous findings, we found that Tβ4 treatment abolished diabetic-reduced Ang1 expression in the diabetic sciatic nerve, measured by Western blot (Figure 6(j)). Double immunofluorescent staining showed that NF-H positive sciatic nerve and S100 positive Schwann cells were Ang1 positive (Figures 6(a) to 6(f)). Western blot analysis revealed that Ang1 protein was substantially decreased in diabetic sciatic nerve tissue compared to nondiabetic one (Figure 6(j)). To further examine whether glucose levels affect Ang1 expression in DRG neurons and Schwann cells, DRG neurons harvested from nondiabetic db/m mice and Schwann cells were cultured under normal and high glucose conditions. Immunocytochemistry showed that DRG neurons were Ang1 positive under regular glucose condition and that the high glucose substantially decreased Ang1 positive DRG neurons (Figures 6(g), 6(h), 6(i), and 6(k)). Incubation of DRG neurons with Tβ4 under high glucose condition significantly increased Ang1 positive DRG neurons (Figure 6(k)). Moreover, Elisa showed substantial reduction of Ang1 protein in supernatants harvested from Schwann cells cultured under high glucose condition compared to the supernatants collected from Schwann cells under regular glucose condition (Figure 6(l)), while Tβ4 reversed the effect of the high glucose on reduction of Ang1 protein (Figure 6(l)). These data indicate that high glucose downregulates Ang1 expression in DRG neurons and Schwann cells, which can be reversed by Tβ4.
To examine the cause effect of Ang1 on DRG neurons and Schwann cells, DRG neurons and Schwann cells were treated with Ang1 (100 ng/mL). Ang1 significantly increased DRG neurite outgrowth (Figures 4(d) and 4(i)) and Schwann cell proliferation (Figures 5(l) and 5(n)) and migration when cultured with the high glucose (Figure 5(o)). Using the neutralizing antibody against Tie2, we then blocked the Ang/Tie2 pathway in the presence of Tβ4. The antibody suppressed Tβ4 promoted neurite outgrowth of DRG neurons (Figures 4(e), 4(h), and 4(i); Figures 5(d), 5(g) and 5(m)) and Schwann cell proliferation (Figures 5(k) and 5(n)) and migration (Figure 5(o)) under high glucose condition. These data suggest that Ang1 mediates the effect of diabetes and Tβ4 on biological function of DRG neurons and Schwann cells.
In this study, we demonstrate that extended Tβ4 treatment of diabetic mice improves neurological function of diabetic neuropathy, and the improvement is closely associated with amelioration of sciatic nerve axonal and myelin damage and an increase of intraepidermal nerve fiber density. In vitro experiments indicate that the Ang1/Tie2 signaling pathway likely mediates the effect of Tβ4 on axonal regeneration and remyelination.
Diabetic peripheral neuropathy is a chronic disease . The goal of the current study was to assess the efficacy and safety of extended Tβ4 treatment on diabetic peripheral neuropathy. We found that administration of Tβ4 at 30 mg/kg for 16 consecutive weeks starting at animal aged 24 weeks substantially increased intraepidermal nerve fiber density, which was associated with considerable improvement of responses to thermal and mechanical stimuli. Diabetic db/db mice develop impairment of sciatic nerve conduction velocity starting at 8–14 weeks of age, while morphometric changes of axonal and myelin damage occur after 20 weeks of diabetes, which resemble human diabetic peripheral neuropathy . Retraction of intraepidermal axons contributes to distal loss of sensation observed in diabetic peripheral neuropathy . Thus, our data indicate that extended Tβ4 treatment is effective by enhancing regeneration of distal epidermal axons.
The present study suggests that the effect of Tβ4 on amelioration of diabetic peripheral neuropathy is unlikely related to hyperglycemia because the extended Tβ4 treatment did not reduce glucose levels. Our in vitro data indicate that primary DRG neurons harvested from diabetic mice cannot reverse their biological functions even when these cells were cultured under a physiological glucose condition. However, Tβ4 could overcome the detrimental effect of hyperglycemia on DRG neurons and Schwann cells. Our findings are consistent with studies published by others, demonstrating dissociation between hyperglycemia and peripheral neuropathy . Use of insulin to control glucose levels in the physiological range fails to ameliorate diabetic peripheral neuropathy .
In addition to distal epidermal axons, Tβ4 treatment reduced axonal and myelin damage of the sciatic nerve. Morphological analyses reveal that the reductions in sciatic nerve fiber diameter and myelin thickness and increases in -ratio, which is a reliable ratio for assessing axonal myelination in diabetic mice, were markedly restored by extended Tβ4 treatment. Therapies targeting axonal remodeling have been shown to enhance recovery of neurological function in experimental diabetic neuropathy. Treatment of db/db mice with gangliosides improves axonal morphometry and nerve conduction velocity . Based on the present data together with published studies, we speculate that extended treatment with Tβ4 could normalize the distal epidermal axons and the morphology of the sciatic nerve which in turn ameliorates nerve conduction velocity (NCV) and sensory function damaged by diabetes.
In the peripheral nervous system, Schwann cells regulate peripheral nerve remyelination and regeneration by their capacity to proliferate and migrate [39, 40]. Many neurotrophic factors regulate axonal remodeling. Ang1 is interesting because it not only promotes angiogenesis, but also acts as a neurotrophic factor on neurons . The present study shows that hyperglycemia downregulates Ang1 expression in DRG neurons and Schwann cells, which contributes suppression of DRG neuron neurite outgrowth and Schwann cell proliferation and migration. Tβ4 reverses the effect of hyperglycemic-reduced Ang1 expression by facilitating neurite outgrowth in DRG neuron and proliferation and migration of Schwann cells. Thus, our data indicate that Ang1 mediates Tβ4-improved DRG neuron and Schwann cell biological function.
The regeneration of myelinated nerve fibers depends on interactions between Schwann cells and axons . Schwann cells provide a microenvironment favoring axonal regeneration due to secretion of neurotrophic factors [42–44]. Hu et al. reported that Schwann cells promote neurite outgrowth of DRG neurons by secreting NGF . The present study showed that Ang1 in conditioned medium from Tβ4-stimulated Schwann cells enhances DRG neurite outgrowth. Hence, Ang1 participates in the crosstalk between Schwann cells and axons during axonal remodeling. We previously demonstrated that Tβ4 upregulates Ang1 in blood vessels, which leads to restoration of vascular function in the diabetic sciatic nerve . The present study showed that Tβ4 also upregulates Ang1 in DRG neurons and Schwann cells under hyperglycemia condition. Others have shown that Ang1 improves regeneration of nerve fibers in diabetic ob/ob mice . Thus, activation of the Ang/Tie2 pathway by Tβ4 likely facilitates axonal regeneration and remyelination, leading to improvement of peripheral nerve function under diabetic neuropathy. However, other potential neurotrophic factors may also be involved in Tβ4-enhanced axonal remodeling, and further studies are warranted.
In summary, our results demonstrate that extended Tβ4 treatment is an effective and safe therapeutic approach to ameliorate experimental diabetic neuropathy. The Ang1/Tie2 signaling pathway likely plays a significant role in the therapeutic effect of Tβ4 on diabetic neuropathy.
The content is solely the responsibility of the authors and does not necessarily represent the official view of the National Institutes of Health.
Conflict of Interests
The authors declare that there is no conflict of interests regarding the publication of this paper.
This work was supported by the Dykstra Foundation and NINDS Grants RO1 AG037506, and RO1 NS075156, and NIDDK RO1 DK097519. The authors thank Cynthia Roberts and Qing-e Lu for their technical assistance.
World Health Organization (WHO), Media Centre Diabetes Fact Sheet, World Health Organization, 2010, http://www.who.int/mediacentre/factsheets/fs312/en/.
Q. D. Wu, J. H. Wang, F. Fennessy, H. P. Redmond, and D. Bouchier-Hayes, “Taurine prevents high-glucose-induced human vascular endothelial cell apoptosis,” American Journal of Physiology: Cell Physiology, vol. 277, no. 6, pp. C1229–C1238, 1999.View at: Google Scholar
L. Wang, Z. G. Zhang, R. L. Zhang, and M. Chopp, “Activation of the PI3-K/Akt pathway mediates cGMP enhanced-neurogenesis in the adult progenitor cells derived from the subventricular zone,” Journal of Cerebral Blood Flow & Metabolism, vol. 25, no. 9, pp. 1150–1158, 2005.View at: Publisher Site | Google Scholar
M. Lindberger, H. D. Schröder, M. Schultzberg et al., “Nerve fibre studies in skin biopsies in peripheral neuropathies. I. Immunohistochemical analysis of neuropeptides in diabetes mellitus,” Journal of the Neurological Sciences, vol. 93, no. 2-3, pp. 289–296, 1989.View at: Publisher Site | Google Scholar
D. M. Levy, G. Terenghi, X.-H. Gu, R. R. Abraham, D. R. Springall, and J. M. Polak, “Immunohistochemical measurements of nerves and neuropeptides in diabetic skin: relationship to tests of neurological function,” Diabetologia, vol. 35, no. 9, pp. 889–897, 1992.View at: Publisher Site | Google Scholar
J. Yamauchi, J. R. Chan, and E. M. Shooter, “Neurotrophins regulate Schwann cell migration by activating divergent signaling pathways dependent on Rho GTPases,” Proceedings of the National Academy of Sciences of the United States of America, vol. 101, no. 23, pp. 8774–8779, 2004.View at: Publisher Site | Google Scholar
G. Sobue, “The role of Schwann cells in peripheral nerve degeneration and regeneration—NGF-NGF receptor system,” Rinshō Shinkeigaku, vol. 30, no. 12, pp. 1358–1360, 1990.View at: Google Scholar
J. Hu, J. Zhou, X. Li, F. Wang, and L. Hezuo, “Schwann cells promote neurite outgrowth of dorsal root ganglion neurons through secretion of nerve growth factor,” Indian Journal of Experimental Biology, vol. 49, no. 3, pp. 177–182, 2011.View at: Google Scholar