AXL signaling in primary sensory neurons contributes to chronic compression of dorsal root ganglion-induced neuropathic pain in rats

Animals

Three- to four-week-old Sprague Dawley (SD) rats were served as donors for the DRG cell culture, and adult male SD rats weighing 200 to 250 g were used for the remaining experiments of this study. All animals were housed in groups of three or four under a 12:12-h light/dark cycle with water and food available ad libitum. All procedures and animal housing facilities were approved by the Institutional Animal Ethics Committee of the Xi’an Jiaotong University Health Science Center and were conducted in accordance with the ethical guidelines of the International Association for the Study of Pain. Accordingly, efforts were made to minimize animal suffering as well as the number of animals used.

Neuropathic pain models

Spinal nerve ligation (SNL) surgery was performed using an existing procedure.^18,19 Briefly, the lumbar 5 (L5) spinal nerve was exposed, ligated, and transected under 2.5% isoflurane anesthesia. The rats in the control, sham-surgery group underwent the identical surgical procedure without nerve ligation and transection.

CCD surgery was also carried out according to a previously described procedure.^1,2 Under 2.5% isoflurane anesthesia, the L4 and L5 intervertebral foramina were exposed, and two L-shaped stainless steel rods (4 mm in length and 0.6 mm in diameter) were carefully inserted into the foramen and left there to compress the L4 and L5 DRGs, respectively. The stainless steel rods were not inserted into the intervertebral foramen in the sham-surgery receiving control group.

DRG cell culture and siRNA transfection

The DRGs of three- to four-week-old SD rats were harvested and subsequently cultured for assessment of the knockdown efficiency of AXL siRNA. In detail, the harvested DRGs were digested with 0.25% trypsin solution without EDTA (Beyotime Biotechnology, Shanghai, China) after being cut into pieces with a size that allowed their passage through the tip of a 1000 μL pipettor. The digested cells were fully separated by repetitive (25×) blowing with a 1000 μL pipettor, passed through a 70-μm cell strainer, and then cultured in prewarmed Neurobasal™-A Medium (Gibco/ThermoFisher Scientific, Waltham, MA) with 10% fetal bovine serum (JR Scientific, Woodland, CA), B-27™ Supplement (1×) (Gibco/ThermoFisher Scientific), 100 units/mL penicillin, and 100 μg/mL streptomycin (Beyotime Biotechnology) in a six-well plate precoated with 50 μg/mL poly-D-lysine (Beyotime Biotechnology). The cells were incubated in an incubator (37°C; 95% O₂, 5% CO₂). After a 24-h incubation, AXL siRNA (250 pmol) or equivalent negative control (NC) siRNA was added in Lipo6000 transfection reagent (Beyotime Biotechnology) to each well. AXL siRNA (5′-GCAUGCUGAAUGAGAACAUTT-3′; 5′-AUGUUCUCAUUCAGCAUGCTT-3′) and NC siRNA (5′-UUCUCCGAACGUGUCACGUTT-3′; 5′-ACGUGACACGUUCGGAGAATT-3′) were designed and synthesized by Genepharma (Shanghai, China). Two days later, the cultured cells were harvested in radio-immunoprecipitation assay (RIPA) lysis buffer for Western blotting.

Intrathecal catheter implantation and drug administration

The procedure for intrathecal catheter implantation for drug delivery has been previously described by us in detail. ²⁰ Briefly, under 2.5% isoflurane anesthesia, a polyethylene-10 catheter was inserted into the subarachnoid space of the spinal cord. Ten microliters of siRNA, AXL inhibitor, or vehicle were injected into the catheter followed by a small air bubble and 10 μL of sterile saline. Any rats showing postoperative neurologic deficits, such as hind-paw paralysis, were excluded from the study.

Intrathecal TP0903 (HY12963; MedChem Express, Shanghai, China) or vehicle (20% dimethyl sulfoxide) was administered 1 h before CCD surgery and then daily, from day 1 through day 5 post-CCD, TP0903 was injected intrathecally at three different doses (0.05, 0.50, and 1.00 μg). Daily doses of intrathecal AXL siRNA, NC siRNA, or vehicle control (phosphate buffer saline) were administered starting on day 3 post-CCD, for a period of five days. Lipo6000 transfection reagent (Beyotime Biotechnology) was used as a vehicle for siRNA to improve delivery efficacy and to avoid siRNA degeneration.^21,22

Behavioral testing

During behavioral tests, pain behaviors in response to mechanical stimuli, noxious heat, and cold stimuli were tested similarly as in our previous studies.^18,19,23 Paw-withdrawal thresholds (PWTs) in response to mechanical stimuli were measured using the up-down testing paradigm.^24,25 To this end, each unrestrained rat was placed in a Plexiglass chamber on an elevated mesh screen after adaptation to the experimental environment. Calibrated von Frey filaments in log increments of force (0.41, 0.69, 1.20, 2.04, 3.63, 5.50, 8.51, 15.14, and 26.0 g) were applied onto the plantar surface of the rat’s hind paws. The 2.04-g stimulus was applied first. If a positive response occurred, the next, smaller von Frey filament was used; if not, the next larger filament in the series was applied. The test was stopped when (1) a negative response to the 26.0-g filament was observed or (2) after the delivery of three more stimuli following the first positive response. The PWT was calculated using the formula provided by Dixon, that is, by converting the pattern of positive and negative responses to a 50% threshold value.^24,25

Paw-withdrawal latencies (PWLs) to noxious heat stimuli were measured with a Model 37370 Analgesic Meter (UGO, Italy).^19,23 Rats were placed on a glass plate within a Plexiglas chamber. Radiant heat stimuli were applied by a light beam to the middle of the plantar surface of each hind paw. The light beam was turned off automatically once rats showed a strong paw-withdrawal response. A stimulus cutoff time of 20 s was used to avoid tissue damage to paw. The PWL was defined as the evolved time between the start of the light beam and paw-withdrawal response. Five tests were performed at 10-min intervals for all paws, and an average PWL value was calculated for each paw.

Cold hyperalgesia was measured using a model ZH-6C cold plate (Zheng-Hua Biologic, Anhui, China). The temperature of the cold plate (diameter: 19 cm) was set at 0°C. Individual rats were placed on the cold plate inside a cylindrical transparent Plexiglas chamber (height: 28 cm, diameter: 20 cm). The response latency was measured from the moment when rats were put into a chamber until they showed a quick and strong paw flinch. A cutoff time of 60 s was used to avoid tissue damage of the animals’ paws. Each trial was repeated three times at 15-min intervals.

RNA extraction, reverse transcription, and quantitative real-time polymerase chain reaction

Rats were first anesthetized and then killed by decapitation, and both L4/L5 DRGs and L4/L5 spinal cord segments were harvested and placed into RNAlater stabilization solution (Thermo Scientific). Tissues were homogenized in a cold tissue homogenizer (Shanghai Jingxin, China), and RNA was extracted with the RNAeasy™ RNA extraction kit (Beyotime Biotechnology). RNA concentrations were quantified using a NanoDrop spectrophotometer (Thermo Scientific). Five hundred nanogram of RNA was reverse-transcribed with oligo (dT) primers using the RevertAid First Strand cDNA Synthesis Kit (Thermo Scientific) according to the manufacturer’s directions. Quantitative polymerase chain reaction (qPCR) was performed in a 20 μL volume containing 20 ng of cDNA, 250 nM forward and reverse primers, and 10 μL of BeyoFast™ SYBR Green qPCR Mix (Beyotime Biotechnology) using the AXL primer (forward: 5′-GACCTAGCTGCCAGGAACTG-3′; reverse: 5′-ACACGTCACTCTTGCTGGTG-3′) or glyceraldehyde 3-phosphate dehydrogenase (GAPDH) primer (forward: 5′-TCGGTGTGAACGGATTTGGC-3′; reverse: 5′-TCCCATTCTCGGCCTTGACT-3′) in a BIO-RAD CFX96 real-time PCR system (Bio-Rad Laboratories, Hercules, CA). The following cycle parameters were applied: initial 3-min incubation at 95°C, followed by 40 cycles with 95°C for 10 s, 60°C for 30 s, and 72°C for 30 s. All results were normalized to those obtained for GAPDH, the internal control. Ratios of mRNA levels in the ipsilateral side to the contralateral side were calculated using the △Ct method (2^−△Ct).

Western blotting

The collected ipsilateral and contralateral L4/L5 DRGs and spinal dorsal horns were put into AllProtect™ Nucleic Acid and Protein Stabilization Reagent for Animal Tissue (Beyotime Biotechnology) and stored at −20°C for subsequent analysis. The tissues were homogenized with ice-cold RIPA lysis buffer (50 mM Tris, 150 mM NaCl, 1% NP-40, 0.25% sodium deoxycholate, 1 mM phenylmethylsulfonyl fluoride; pH7.4) with a protease-/phosphatase-inhibitor cocktail (Beyotime Biotechnology) using a Shanghai Jingxin tissue homogenizer (Shanghai Jingxin). After the crude homogenate was centrifuged at 4°C for 15 min at 1000 g, the supernatants were collected to assess cytosolic protein levels. Protein concentrations were measured using a Bradford Protein Assay Kit (Beyotime Biotechnology). Equal sample amounts were heated for 5 min at 99°C and loaded onto an 8% sodium dodecyl sulfate-polyacrylamide electrophoresis separation gel. The proteins were then electrophoretically transferred onto a nitrocellulose membrane, and the membrane was blocked with 3% nonfat milk in Tris-buffered saline containing 0.1% Tween-20 and followed by primary and secondary antibodies incubations. The primary antibodies including rabbit anti-phosphorylated AXL (anti-p-AXL) (phosphor Tyr697, 1:1000; GeneTex, Irvine, CA), rabbit anti-AXL (1:1000; Bioss, Peking, China), rabbit anti-mTOR (1:1000; Cell Signaling Technology, Danvers, MA), and mouse anti-β-actin (1:2000; Santa Cruz Biotechnology, Santa Cruz, CA) were incubated overnight at 4°C. The secondary antibodies including horseradish peroxidase-conjugated antirabbit and antimouse secondary antibody (1:3000; EMD Millipore, Darmstadt, Germany) were incubated at 25°C for 2 h. The proteins on the membrane were detected using western peroxide reagent and luminol/enhancer reagent (Immobilon Western Chemiluminescent HRP Substrate; EMD Millipore) and visualized using the Champchemi System with SageCapture software (Sagecreation Service for Life Science, Beijing, China). The intensity of blots was quantified by NIH ImageJ software. Each blot from the targeted protein was normalized relative to the corresponding β-actin blot. The average value of the control groups was set as 100% after normalization. The relative levels of the targeted protein at the different time points and/or the treated groups were determined by dividing the normalized values from these groups by the average value of the control group.

Immunofluorescence

The L4/L5 DRGs were removed after transcardial perfusion with 100 mL of perfusion buffer, followed by 250 mL of 4% paraformaldehyde in 0.1M phosphate buffer. Subsequently, the tissues were postfixed, dehydrated, and then cut at 20 μm using a Leica CM3050 S cryostat. All DRG sections were placed directly on gelatin-covered slides. For single labeling of p-AXL, DRG sections were incubated overnight at 4°C with rabbit anti-p-AXL antibody (1:100; Genetex) after blocking with 10% normal goat serum. The sections were then incubated with goat antirabbit antibody conjugated to Alexa Fluor 488 (1:200; Abcam, Cambridge, MA) for 2 h at room temperature. For double labeling of p-AXL or AXL with DRG cell markers, DRG sections were incubated with rabbit anti-p-AXL antibody (1:100; Genetex) or anti-AXL antibody (1:200; Absin, Shanghai, China) and mouse anticalcitonin gene-related peptide (CGRP, 1:50; Abcam), mouse antineurofilament-200 (NF200, 1:500; Sigma, St. Louis, MO), or mouse antiglutamine synthetase (GS, 1:500; EMD Millipore), overnight at 4°C, followed by goat antirabbit antibody conjugated to Alexa Fluor 488 (1:200; Abcam) and goat antimouse antibody conjugated to Cy3 (1:200; Abcam) for 2 h at room temperature. For double labeling of p-AXL or AXL with biotinylated isolectin B4 (IB4, 1:100; Sigma), Alexa Fluor 488-conjugated goat antirabbit antibody (1:200; Abcam) and Cy3-conjugated Avidin (1:200; Abcam) were used as the second antibodies. The primary antiserum was omitted to obtain control DRG sections. The slides were coverslipped with SouthernBiotech Fluoromount-G (SouthernBiotech, Birmingham, AL) or antifade mounting medium with 4′,6-diamidino-2-phenylindole (Beyotime Biotechnology). The single-labeled pictures were made by an Olympus BX53 fluorescence microscope, and double-labeled pictures were made using a Nikon C2 confocal microscope (Nikon, Tokyo, Japan). All pictures were quantified using NIH ImageJ Software.

Statistical analysis

The animals were randomly allocated to the various treatment groups. The number of rats was six per group in the behavioral, three per group in Western blotting, and five per group in immunofluorescence experiments. The data were statistically analyzed using SigmaPlot 12.5 software (San Jose, CA) by two-tailed, paired Student’s t test for two-group comparisons, one-way analysis of variance (ANOVA) for comparisons of more than two groups, and two-way repeated measure ANOVA for results from the behavioral tests. Whenever ANOVAs showed a significant difference, post hoc Tukey tests were performed for pairwise comparisons between means. All of the results were given as means ± standard error of the mean. Tests yielding P < 0.05 were considered to be statistically significant.

Increased AXL expression in injured DRGs

The expression and distribution of p-AXL and AXL in naive L4/L5 DRGs were examined by immunofluorescence (Figure 1(a)). Primary antibodies were omitted to obtain NC for p-AXL and AXL immunostaining (Figure 1(a)). Quantitative analysis showed that approximately 42.0 ± 4.7% of DRG neurons was positive for p-AXL and 51.8 ± 4.0% for AXL. All detectable p-AXL-positive neurons were small to medium (<1200 μm²) in cross-sectional area. About 64.5% of p-AXL-positive neurons were small (<600 μm²) and the remaining were medium in size (Figure 1(b)). In all AXL-positive neurons, about 49.0% of them were small (<600 μm²), 35.5% were medium (<1200 μm²), and 15.4% were large in cross-sectional area (Figure 1(c)). Usually, NF200 was used to label medium/large neurons with myelinated A-fibers, CGRP for small DRG peptidergic neurons, and IB4 for small nonpeptidergic DRG neurons.^26,27 Examination of the expression and distribution of p-AXL in naive L4/L5 DRGs by double-labeling immunofluorescence with NF200, CGRP, or IB4 (Figure 1(d)) demonstrated that p-AXL was dominantly expressed in IB4- or CGRP-positive DRG neurons. Of the p-AXL-positive neurons, 72.7 ± 3.6% showed colocalization with IB4 and 30.3 ± 2.5% with CGRP. None of the p-AXL-positive DRG neurons were NF200-positive (Figure 1(d); Table 1). However, AXL was colocalized not only with IB4 and CGRP but also with NF200 in naive L4/L5 DRGs (Figure 1(e)). Approximately 45.0 ± 5.1% of AXL-positive neurons were colocalized with IB4, 26.7 ± 5.6% with CGRP, and 27.5 ± 3.7% with NF200 (Figure 1(e); Table 1). Moreover, by using GS as the marker for DRG satellite glial cells,^18,21 neither p-AXL nor AXL was detected in DRG satellite glial cells (Figure 1(d) and (e)).

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Figure 1.

Expression of p-AXL and AXL in DRG. (a) The expression of p-AXL, AXL, and negative control without primary antibodies in naive L4/L5 DRGs. Histogram shows the distribution of p-AXL (b) and AXL (c) somata in naive L4/L5 DRGs. N = 3 rats, 6 to 8 slices per rat. (d) The colocalization of p-AXL with IB4, CGRP, NF200, or GS. (e) The colocalization of AXL with IB4, CGRP, NF200, or GS. Arrows: examples of double-labeled neurons. Scale bars: 100 μm (a); 25 μm (c and d). IB4: isolectin B4; CGRP: calcitonin gene-related peptide; NF200: neurofilament-200; p-AXL: phosphorylated AXL; GS: glutamine synthetase.

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Table 1.

The percentage of p-AXL- and AXL-positive neurons in three DRG neuron types (IB4-, CGRP-, or NF200-positive DRG neuron).

	IB4	CGRP	NF200
p-AXL	72.7 ± 3.6%	30.3 ± 2.5%	0
AXL	45.0 ± 5.1%	26.7 ± 5.6%	27.5 ± 3.7%

IB4: isolectin B4; CGRP: calcitonin gene-related peptide; NF200: neurofilament-200; p-AXL: phosphorylated AXL.

Next, we examined the changes of p-AXL and AXL expression in neuropathic pain models. AXL mRNA levels were increased in injured DRGs in both SNL- and CCD-induced neuropathic pain rats. In SNL rats, AXL mRNA in injured DRGs increased to 2.86-fold levels relative to the sham group on day 7 after surgery (P < 0.01, Figure 2(a)). In CCD rats, AXL mRNA increased to 3.21, 3.12, and 4.91-fold levels in compressed DRGs on days 3, 7, and 14, respectively (F_(3,15) = 9.13, P < 0.01, Figure 2(b)). Both p-AXL and AXL protein levels were increased significantly on days 7 and 14 (F_(3,15) = 9.13, P < 0.01) but not on day 3 after CCD surgery (Figure 2(c)). The ratio of p-AXL to AXL was increased only on day 7 after surgery (Figure 2(c)). The expression levels of p-AXL and AXL were unaltered in the contralateral DRGs or the ipsilateral spinal cord at any of the examined time points (Figure 2(d) and (e)). Accordingly, the percentage of p-AXL-positive neurons and AXL-positive neurons in compressed DRGs was increased by 13.2% and 13.9%, respectively, relative to that of sham-operated DRGs (55.2 ± 5.3% vs. 42.0 ± 4.7%, P < 0.01, Figure 3(a) and (b); 65.7 ± 4.3% vs. 51.8 ± 4.0%, P < 0.01, Figure 3(c) and (d)).

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Figure 2.

Expression changes of AXL mRNA and AXL protein in the DRG and spinal dorsal horn in neuropathic pain models. (a) The amount of AXL mRNA was increased in the ipsilateral L5 DRG on day 7 in the SNL-induced neuropathic pain model. N = 5 rats per group. **P < 0.01 versus the sham group by two-tailed unpaired Student’s t test. (b) The amount of AXL mRNA was increased in the ipsilateral L4/L5 DRG on days 3, 7, and 14 in CCD-induced neuropathic pain model. N = 3 or 4 rats/time point. One-way ANOVA (expression vs. time points) followed by post hoc Tukey tests, *P < 0.05, **P < 0.01 versus day 0 (sham group). (c) The protein amount of p-AXL and total AXL increased in the ipsilateral L4/L5 DRGs after CCD surgery. N = 3 or 4 rats/time point. One-way ANOVA (expression vs. time points) followed by post hoc Tukey test, *P < 0.05, **P < 0.01 versus day 0 (sham group). No significant changes in p-AXL and total AXL were observed in the contralateral L4/L5 DRGs (d) and the ipsilateral L4/L5 spinal dorsal horns (e) at all observed time points after CCD surgery. DRG: dorsal root ganglion; CCD: chronic compression of DRG; SNL: spinal nerve ligation; p-AXL: phosphorylated AXL.

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Figure 3.

Expression changes of p-AXL- and AXL-positive neurons in the DRG in CCD-induced neuropathic pain model. (a and b) The percentage of p-AXL-positive (+) neurons increased in compressed L4/L5 DRGs of CCD rats. The value on each histogram shows the ratio of p-AXL (+) neurons to total counted neurons in DRG slices. N = 5 rats/group. **P < 0.01 versus the sham group by two-tailed unpaired Student’s t test. (c and d) The percentage of AXL-positive (+) neurons increased in compressed L4/L5 DRGs of CCD rats. The value on each histogram shows the ratio of AXL (+) neurons to total counted neurons in DRG slices. N = 3 rats/group. **P < 0.01 versus the sham group by two-tailed unpaired Student’s t test. Scale bar: 50 μm. CCD: chronic compression of dorsal root ganglion; p-AXL: phosphorylated AXL.

Inhibition of AXL activation attenuates CCD-induced pain hypersensitivities

Increases in the p-AXL/AXL ratio indicate a potential role of AXL receptor activation in the pathological mechanisms induced by DRG compression. We used a selective and effective AXL receptor inhibitor TP0903 to assess whether AXL mediated CCD-induced neuropathic pain. It has been reported that CCD could induce mechanical and thermal pain hypersensitivities as early as day 2 and last for over 35 days.^1–3 We observed the effect of repeated TP0903 (0.05, 0.50, or 1.00 μg) on CCD induced the changes in paw-withdrawal responses to mechanical, thermal, and cold stimuli on days 4 and 6 post-CCD. TP0903 or vehicle solution was intrathecally administered 1 h before CCD or sham surgery and once daily for five days after CCD or sham surgery. On days 4 and 6, ipsilateral PWTs to mechanical stimuli, PWLs to thermal stimuli, and response latencies to cold stimuli in the CCD plus vehicle group were decreased significantly compared to the sham-operation plus vehicle group (Figure 4(a)). Repeated injections of 0.50 and 1.00 μg TP0903 reversed these decreases in latency (Figure 4(a) to (c)). Also on days 4 and 6 after CCD surgery, PWTs to mechanical, PWLs to thermal, and positive response latencies to cold stimulation were much higher on the ipsilateral side of the TP0903 plus CCD group than in the CCD plus vehicle group (Figure 4(a): F_(15,191) = 10.38, Figure 4(b): F_(15,191) = 7.33, Figure 4(c): F_(15,191) = 16.96, **P < 0.01, vs. Sham + Veh, ^##P < 0.01, vs. CCD + Veh). The 0.05 μg dose of TP0903 did not affect the CCD-induced decreases in paw-withdrawal responses (Figure 4(a) to (c)). Moreover, the 1 μg dose of TP0903 did not alter basal paw-withdrawal responses to mechanical, thermal, and cold stimuli in sham-operated rats (P > 0.05, Figure 4(a) to (c)). These results indicate that the AXL inhibitor, TP0903, exhibited analgesic effects on CCD-induced pain hypersensitivities to mechanical, thermal, and cold stimuli.

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Figure 4.

Effects of AXL inhibitor TP0903 on CCD-induced nociceptive hypersensitivities. The dose of TP0903 (0.05, 0.5, or 1 μg) or vehicle solution was intrathecally administered 1 h before CCD or sham surgery and once daily for five days after CCD or sham surgery. The doses of 0.5 and 1 μg inhibited (a) the decrease of PWTs to mechanical stimulation, (b) PWLs to thermal stimulation, and (c) positive response latencies to cold stimulation on the ipsilateral side of CCD rats. N = 6 rats/group. Two-way repeated measure ANOVA (effect vs. group × time interaction) followed by post hoc Tukey tests, **P < 0.01 versus the corresponding time point in the Sham + Veh group. ^##P < 0.01 versus the corresponding time point in the CCD + Veh group. PWT: paw-withdrawal threshold; PWL: paw-withdrawal latency; CCD: chronic compression of dorsal root ganglion.

Knockdown of DRG AXL relieves CCD-induced pain hypersensitivities

In order to assess the relationship between total AXL-protein expression and neuropathic pain, we examined the effect of DRG AXL knockdown on CCD-induced pain hypersensitivities in rats by intrathecally administering AXL siRNA. First, the knockdown efficiency of AXL siRNA was confirmed in vitro by DRG cell culture. As shown in Figure 5(a), transfection of AXL siRNA (125 nM) was associated with a 50% decrease in total AXL expression relative to NC siRNA treatment (P < 0.01). In the subsequent in vivo experiment, AXL siRNA or NC siRNA was administered intrathecally once daily for five days starting on day 3 postsurgery. As expected, AXL expression increased significantly in ipsilateral L4/L5 DRGs in the CCD plus vehicle group. AXL siRNA (5 μM/10 μL), but not NC siRNA (5 μM/10 μL), reversed the upregulation of CCD-induced AXL expression in the ipsilateral compressed L4/L5 DRGs (F_(4,19) = 21.67, **P < 0.01 vs. Sham + Veh, ^##P < 0.01 vs. CCD + Veh; Figure 5(b)). However, the basal expression of AXL in the ipsilateral L4/L5 DRGs was not affected by AXL siRNA in the sham plus AXL siRNA group compared with the sham plus vehicle group (Figure 5(b)). This result, which we also found in previous studies,^18,21 may be due to a low expression level of target genes in the basal condition.

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Figure 5.

AXL siRNA suppressed AXL expression in vitro and in vivo. (a) The amount of AXL was markedly decreased by AXL siRNA (Si, 250 nM) treatment in DRG cell culture. N = 3 repeats (six wells from three rats) per treatment. **P < 0.01 versus NC siRNA by two-tailed unpaired Student’s t test. (b) Intrathecal injection of AXL siRNA (10 μM in 10 μL) blocked the increase of AXL induced by CCD and did not affect the basal level of AXL in the sham group. The first injection was administered on day 3 post-CCD and repeated once daily for five days, and ipsilateral L4/L5 DRGs were harvested on day 8 post-CCD. N = 3 rats/time point. One-way ANOVA (effect vs. the treated groups) followed by post hoc Tukey tests, *P < 0.05 versus the Sham + Veh group. ^##P < 0.01 versus the CCD + Veh group. NC: negative control; DRG: dorsal root ganglion; CCD: chronic compression of DRG.

All paw-withdrawal responses were tested on days 6 and 8 after sham or CCD surgery. PWTs to mechanical stimulation, PWLs to thermal stimulation, and positive latencies to cold stimulation were significantly decreased on the ipsilateral side in the CCD plus vehicle group (**P < 0.01, vs. Sham + Veh, Figure 6(a) to (c)). These decreases were reversed by repeated intrathecal injection of AXL siRNA (Figure 6(a): F_(8,119) = 25.20, Figure 6(b): F_(8,119) = 32.92, Figure 6(c): F_(8,119) = 29.99, ^##P < 0.01, vs. CCD + Veh) but not by NC siRNA administration (P > 0.05, Figure 6(a) to (c)). Neither AXL siRNA nor NC siRNA changed the basal level of paw-withdrawal responses to mechanical, thermal, or cold stimuli (Figure 6(a) to (c)). These results suggested a potential role of both activated AXL and total AXL in CCD-induced pain hypersensitivity.

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Figure 6.

Effect of AXL siRNA on CCD-induced nociceptive hypersensitivities. All siRNAs (10 μM in 10 μL vehicle solution) or vehicle solutions were intrathecally administered from day 3 to day 7 once daily for five days. Intrathecal injection of AXL siRNA (Si) but not NC siRNA reversed the decrease of PWTs to mechanical stimulation (a), PWLs to thermal stimulation (b), or positive response latencies to cold stimulation (c) on the ipsilateral side of CCD rats. N = 6 rats/group. Two-way repeated measure ANOVA (effect vs. group × time interaction) followed by post hoc Tukey tests. **P < 0.01 versus the corresponding time point in the Sham + Veh group. ^##P < 0. 01 versus the corresponding time point in the CCD + Veh group. NC: negative control; PWT: paw-withdrawal threshold; PWL: paw-withdrawal latency; CCD: chronic compression of dorsal root ganglion; siRNA: small interfering RNA.

mTOR mediates the intracellular effect of AXL

We found that the expression of AXL in injured DRGs was upregulated in rats with CCD-induced neuropathic pain, and intracellular mTOR signaling participated in the peripheral mechanism underlying neuropathic pain. Specifically, p-AXL was primarily located on IB4-positive neurons and CGRP-positive neurons in DRG. Inhibition of AXL activity, or interference of AXL expression in DRG, can effectively alleviate pain sensitivities in CCD rats. While previous studies have indicated that AXL activated the PI3K/Akt signaling pathway, ⁹ we examined whether AXL activated, or otherwise influenced, mTOR signaling, a downstream target of PI3K/Akt that is involved in morphine tolerance and neuropathic pain development.^15–17 Our previous work have shown that mTOR expression increased in the compressed DRGs after CCD surgery. ²⁸ We further confirmed that the expression of phosphorylated mTOR (p-mTOR) and total mTOR increased in ipsilateral DRGs on day 7 and day 14 (p-mTOR: F_(3,11) = 7.40, P < 0.05; mTOR: F_(3,11) = 14.93, P < 0.01) but not on day 3 after CCD surgery (Figure 7(a)). The ratio of p-mTOR to mTOR does not change at any detected time points (Figure 7(a)), suggesting that the change of mTOR activation is totally due to the increased total mTOR protein. Daily intrathecal injection of either TP0903 (1 μg per day; Figure 7(b)) or AXL siRNA (5 μM in 10 μL vehicle solution per day; Figure 7(c)) reversed the increase of p-mTOR (Figure 7(b): F_(2,13) = 12.8, P < 0.01; Figure 7(c): F_(2,13) = 12.2, P < 0.01) and mTOR expression (Figure 7(b): F_(2,13) = 16.9, P < 0.01; Figure 7(c): F_(2,13) = 17.0, P < 0.01) in CCD rats. However, the ratio of p-mTOR to mTOR does not change at any treated groups compared with the sham plus vehicle group. This result suggests that AXL enhanced mTOR signaling, thus involved in peripheral mechanisms of neuropathic pain.

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Figure 7.

Mediation by the intracellular signaling molecule, mTOR, of nociceptive effects of AXL. (a) The protein amount of p-mTOR and total mTOR increased in the ipsilateral L4/L5 DRGs on days 7 and 14 after CCD surgery. N = 3 rats/time point. One-way ANOVA (expression vs. time points) followed by post hoc Tukey test, *P < 0.05, **P < 0.01 versus day 0 (sham group). Repeatedly intrathecal injection of (b) TP0903 (1 μg) or (c) AXL siRNA (Si, 5 μM in 10 μL vehicle solution) reduced mTOR expression in compressed DRGs of CCD rats. N = 3 rats/time point. One-way ANOVA (effect vs. the treated groups) followed by post hoc Tukey tests, *P < 0.05, **P < 0.01, versus the Sham + Veh group; ^##P < 0.01 versus the CCD + Veh group. DRG: dorsal root ganglion; CCD: chronic compression of DRG; mTOR: mammalian target of rapamycin.