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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptHHS Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
 
J Neurosci. Author manuscript; available in PMC 2013 June 5.
Published in final edited form as:
PMCID: PMC3533441
NIHMSID: NIHMS427292

Dynamic changes in heat transducing channel TRPV1 expression regulate mechanically insensitive, heat sensitive C-fiber recruitment after axotomy and regeneration

Abstract

Peripheral injury leads to a significant increase in the prevalence of mechanically insensitive, heat sensitive C-fibers (CH) that contain the heat transducing TRPV1 channel in mice. We have recently shown that this recruitment of CH fibers is associated with increased expression of the receptor for GDNF family neurotrophic factor artemin (GFRα3), and that in vivo inhibition of GFRα3 prevented the increase in TRPV1 expression normally observed following axotomy. Here we have directly tested the hypothesis that the recruitment of functional CH-fibers following nerve regeneration requires enhanced TRPV1 levels. We utilized in vivo siRNA-mediated knockdown to inhibit the injury-induced expression of TRPV1 coupled with ex-vivo recording to examine response characteristics and neurochemical phenotypes of different functionally defined cutaneous sensory neurons after regeneration. We confirmed that inhibition of TRPV1 did not affect the axotomy induced decrease in CPM heat threshold, but transiently prevented the recruitment of CH neurons. Moreover, a recovery of TRPV1 protein was observed following resolution of siRNA-mediated inhibition that was correlated with a concomitant rebound in CH neuron recruitment. Thus dynamic changes in TRPV1 expression, not absolute levels, may underlie the functional alterations observed in CH neurons and may contribute to the development of heat hyperalgesia after nerve injury.

INTRODUCTION

Transient receptor potential vanilloid type I (TRPV1) is a well-known heat transducing channel involved in behavioral heat hyperalgesia following peripheral injuries (Caterina et al 1997; 2000; Davis et al 2000). We have recently found that this channel is specifically contained in a small subset of murine cutaneous C-fibers that are mechanically insensitive but heat sensitive (CH; Lawson et al 2008). TRPV1 knockout mice, which do not develop heat hyperalgesia after inflammation (Caterina et al 1997), do not have CH-fibers (Lawson et al 2008; Koerber et al 2010), suggesting that the presence or changes in these particular afferents are crucial for the development of inflammation induced heat hypersensitivity., Heat hyperalgesia following nerve regeneration has been well documented in humans (e.g. Head and Sherren 1905). In addition we have previously shown that both axotomy and regeneration (Jankowski et al 2009a) and peripheral inflammation (Jankowski et al 2012) induce a significant increase in the proportion of functional CH-fibers relative to that seen in uninjured mice, suggesting that changes in these fibers could contribute to heat hyperalgesia in both types of injury.

In our previous studies we have also obtained results suggesting possible mechanisms responsible for this recruitment of normally mechanically and thermally insensitive fibers to CH-fibers. For example, axotomy of the saphenous nerve was found to induce the expression of the GDNF neurotrophic factor family member artemin in the skin with a corresponding increase in its receptor (GFRα3) in the DRGs during nerve regeneration (Bennett et al 2000; Orozco et al 2001; Jankowski et al 2009a). This subsequently caused an increase in TRPV1 expression corresponding with reinnervation (Jankowski et al 2009a). The change in GFRα3 expression was found to be essential for the observed CH fiber recruitment after axotomy and regeneration, and this correlated with the delayed increase in TRPV1 expression. Thus we hypothesized that the injury-induced increase in artemin/ GFRα3 signaling resulted in increased levels of TRPV1, which in turn was directly responsible for the observed CH-fiber recruitment (Jankowski et al 2010).

Here, we sought to directly test this hypothesis using our in vivo siRNA knockdown strategy by injecting siRNAs targeting TRPV1 during saphenous nerve regeneration. The effects of the blockade of TRPV1 expression on the functional response properties and neurochemical phenotypes of regenerated fibers was determined using an ex vivo preparation (Jankowski et al 2009a; 2010).

METHODS

Animals

Experiments were conducted using adult (4–6 weeks) male Swiss Webster mice (Hilltop Farms, Scottdale, PA). All procedures were approved by the Institutional Animal Care and Use Committee at the University of Pittsburgh and used in accordance with institutional AAALAC approved practices.

Saphenous nerve axotomy

Mice were anesthetized by 3% isofluorane inhalation. A small incision was made at the mid-thigh level. The saphenous nerve was transected without disturbing the surrounding tissue. The wound was closed using 7.0 silk sutures and animals were allowed to survive for 28–84 days.

siRNA injections

siRNAs were designed and conjugated to Penetratin-1 (Pen-siRNA) as described previously (Davidson et al 2004; Jankowski et al 2006, 2009b; 2010). Mice were anesthetized as described above and the previously transected saphenous nerve was exposed proximal to the lesion. Pen-siRNAs were first heated to 65°C for 5 minutes to increase solubility. Then at two and three weeks after cutting the nerve, 0.1–0.2µl of 90µM Penetratin-1 linked control (PenCON) or TRPV1 targeting (PenV1) siRNAs were injected into the saphenous nerve (Jankowski et al., 2009b).

RNA Isolation and Realtime PCR

Animals were anesthetized with a mixture of ketamine (90mg/kg) and xylazine (10mg/kg) and perfused with ice cold 0.9% NaCl prior to dissection of DRGs. RNA isolation from the L2/L3 DRGs, reverse transcription and SYBR Green realtime PCR was performed according to our previous reports (Jankowski et al. 2009, 2010, 2012). Expression of TRPV1, GFRα3, Sox11, ATF3 and GAPDH were analyzed. Ct values for genes of interest were normalized to GAPDH and changes in expression are calculated as a ΔΔCt value according to the manufacturer’s specifications. Fold change is described as 2ΔΔCt (Applied Biosystems) and 2-fold change equals 100% change.

Western Blot

Pooled L2/L3 DRGs from eight naïve and eight nerve injured mice from each experimental condition and time point were used for western blotting analysis according to modified protocols described in our previous reports (Jankowski et al 2009, 2010, 2012). After transfer, PVDF membranes were incubated first in a 1:1 mixture of LiCor blocking buffer and PBS and then in primary antibodies overnight at 4°C (TRPV1: 1:100; Santa Cruz; GAPDH: 1:2000; ProSci Inc.). Antibody binding was visualized using 680nm or 800nm infrared dye conjugated donkey anti-rabbit or donkey anti-chicken secondary antibodies (1:10,000; LiCor) and detection using the LiCor Odyssey Imager (LiCor). Settings for detection were consistent between runs with the gain set at 1.0. Immunoreactive bands were analyzed by densitometry and quantified using NIH Image J analysis software. Band intensity was normalized to GAPDH and reported as a percent change

Ex-vivo preparation

The ex-vivo preparation has been described previously (McIlwrath et al 2007; Lawson et al 2008). Briefly, mice were anesthetized (Ketamine: 90mg/kg and Xylazine: 10mg/kg; i.m.) and transcardially perfused with oxygenated (95% O2–5% CO2) artificial CSF (aCSF; in mM: 1.9 KCl, 1.2 KH2PO4, 1.3 MgSO4, 2.4 CaCl2, 26.0 NaHCO3, and 10.0 D-glucose) containing 253.9mM sucrose at 12–15°C. The spinal cord and right hindlimb was excised and placed in a circulating bath of oxygenated aCSF. Hairy skin of the right hindpaw, saphenous nerve, T13-L5 DRGs and spinal cord were isolated and transferred to a separate recording chamber containing chilled oxygenated aCSF in which the sucrose was replaced with 127.0mM NaCl and warmed to 31°C. The skin was pinned out on a stainless steel grid located at the bath/air interface while the epidermis stayed dry.

DRG cells were impaled with quartz microelectrodes containing 5% Neurobiotin (Vector Laboratories, Burlingame, CA) in 1M potassium acetate. Electrical search stimuli were delivered through a suction electrode on the nerve. Cutaneous receptive fields (RF) were localized with a blunt glass stylus and von Frey hairs. When no mechanical RF was found, a thermal search was conducted by applying cold (~ 0°C) then hot (~52°C) saline to the skin

Response characteristics were determined by first applying computer-controlled mechanical stimulation (Aurora Scientific) using a 1 mm diameter plastic disc: 5s square waves of 1, 5, 10, 25, 50 and 100mN were applied to the RF. Next a digitally controlled thermal stimulus was applied using a 3mm2 contact area Peltier element (Yale Univ. Machine Shop). Thermal stimulus consisted of rapid cooling to 4°C, return to baseline, then a 12s heat ramp from 31–52°C. A 30s recovery was employed between stimulations. Recorded responses were analyzed offline (Spike2 software, Cambridge Electronic Design). Selected cells were iontophoretically labeled with Neurobiotin. Peripheral conduction velocity was calculated using spike latency and the distance between stimulating and recording electrodes.

Tissue processing and analysis of recorded cells

DRGs containing injected cells were immersion fixed with 4% paraformaldehyde in 0.1M phosphate buffer (PB) for 30 min at 4°C. Ganglia were embedded in 10% gelatin, postfixed in 4% paraformaldehyde, and cryoprotected in 20% sucrose. Frozen sections (60µm) were reacted with fluorescently-tagged (FITC) avidin to label Neurobiotin-filled cells (Vector Laboratories) and processed for IB4 binding (AlexaFluor 647; Molecular Probes, Eugene, OR) and TRPV1 (1:2000; Alomone) immunohistochemistry. Fluorescent staining was determined using sequential scanning on an Olympus FluoView™ 500 confocal microscope (Olympus America Inc).

Data analysis

One-way ANOVA and posthoc analysis (Tukey) were used to analyze differences in firing rate along with mechanical and thermal thresholds. Differences in fiber prevalence and immunostaining were determined by Fisher’s Exact analysis. Percent changes in mRNA were determined to be statistically significant by ANOVA with post hoc analysis (Tukey). Statistical analyses were performed on raw Ct data and represented for ease of presentation as a percent change. P-values were set at p<0.05.

RESULTS

We first verified that TRPV1 gene expression could be specifically inhibited by TRPV1-targeting (PenV1) siRNAs injected into the saphenous nerve after axotomy. At 28 days following axotomy and regeneration, TRPV1 mRNA was found to be significantly increased in the DRGs after injection of non-targeting (PenCON) siRNAs (36%±13%), similar to what had previously been shown after axotomy alone (Jankowski et al 2009a). Injection of targeting PenV1 siRNAs significantly inhibited the axotomy-induced increase in TRPV1 mRNA (−13%±5%; Fig. 1a). At the 70 day time point, however, both PenCON injection plus axotomy (74%±15%) and PenV1 plus axotomy (52%±10%) showed enhanced levels of TRPV1 in the DRGs relative to naïve mice, similar to the levels detected after axotomy alone (87%±21%; Jankowski et al 2009a; Fig. 1b). RT-PCR results were then verified at the protein levels (Fig. 1c,d; 28d: Axotomy: 25%; PenCON plus axotomy: 43% and PenV1 plus axotomy: −32%; 70d: Axotomy: 49%; PenCON plus axotomy: 32% and PenV1 plus axotomy: 47%).

Figure 1
Realtime PCR and western blotting analysis of dorsal root ganglia (DRGs) 28 and 70 days after axotomy of the saphenous nerve with or without injection of control (PenCON) or TRPV1 targeting (PenV1) siRNAs

TRPV1 knockdown does not alter the axotomy-induced decrease in CPM heat threshold

A total of 225 cutaneous sensory neurons were intracellularly recorded and physiologically characterized from 40 nerve injured adult Swiss-Webster mice. The results from these two experimental groups were compared with each other and to previously published results from naïve and axotomized SW mice (Jankowski et al 2009a). Neurons with a conduction velocity of < 1.2 m/s were classified as C-fibers (Kress et al 1992) and all others were classified as A-fibers. For these experiments we have focused our analyses specifically on the population of regenerated C-fibers.

We found no statistical difference between time points (4–6 and 10–12 weeks) for each of the experimental conditions in relation to polymodal C-fiber (CPM: mechanical and heat or mechanical, heat and cold sensitive) mechanical threshold, heat threshold or maximal firing rate during the heat ramp; therefore the data is combined for ease of presentation. After regeneration of the saphenous nerve in PenCON injected mice, CPM thermal thresholds were significantly reduced to 39.1±0.6°C (p<0.01) compared to previous naïve data (42.6±0.5°C); similar to that seen after axotomy alone (39.2±0.7°C; Jankowski et al 2010). A comparable reduction in threshold was detected in mice that received PenV1 siRNA injection (40.3±0.6°C; p<0.01; Fig. 2a). The maximal firing rate of CPM neurons during the heat ramp was increased after PenCON plus axotomy (7.8±1.1Hz; p<0.01) relative to naïves (3.9±0.4Hz) similar to the significant increase shown after axotomy alone (5.9±0.9 Hz; Jankowski et al 2010). While the maximal firing rate of CPM neurons was still elevated in mice injected with PenV1 siRNAs plus axotomy, it was not significantly different from naïve values (5.1±0.5Hz; p=0.06; Fig. 2b). Importantly the increase in firing rate was not different from that observed following axotomy alone (p=0.3). Consistent with our previous reports (Jankowski et al 2009a, 2010), CPM mechanical threshold was not altered under any condition (Naïve: 20.8±2.2mN; Axotomy: 24.2±3.8mN; PenCON plus axotomy: 24.2±4.8mN; PenV1 plus axotomy: 25.2±3.2mN).

Figure 2
Heat thresholds and maximal firing rates of CPM neurons after axotomy

TRPV1 knockdown alters the recruitment of CH neurons induced by axotomy and regeneration

CH fibers showed no significant changes in thermal threshold at any time points tested after axotomy under any condition (Naïve: 41.0±1.6°C; Combined Time Points: Axotomy: 44.0±1.3°C; PenCON + Axotomy: 39.6±1.9°C; PenV1 + Axotomy: 37.9±1.9°C; p<0.2 relative to naives). As shown previously following axotomy alone (Jankowski et al., 2009a; 2010) 4–6 weeks after nerve cut, there was a significant increase in the proportion of CH fibers relative to naïve mice in the PenCON plus axotomy condition (5% vs 18%; p<0.02). This recruitment of CH fibers after axotomy however, was blocked by inhibition of TRPV1 expression (PenV1 + Axotomy: 10%; p<0.1) at this time point (Fig. 3a–c). However at the 10–12 week time point (Fig. 3d,e), the proportion of CH-fibers was significantly increased in this group (18%; p<0.02) matching that seen in axotomy alone (Jankowski et al 2009a; 2010) and PenCON plus axotomy (23%; p<0.001). This rebound in CH-fibers corresponded with the rebound of TRPV1 levels at this later time point (Fig. 1)

Figure 3
Phenotypes of C-fibers before and after axotomy of the saphenous nerve

Immunohistochemical characterization of cutaneous CPM and CH neurons after regeneration

A total of 39 C-fibers were intracellularly labeled, recovered and imunohistochemically characterized in nerve injured mice from the two conditions. There were no differences in immunolabeling for either marker between time points under any condition; therefore, we combined immunostaining results from the time points for ease of presentation. Overall, most CPM fibers (7 of 12) bound IB4 in mice with PenCON siRNA injection plus axotomy and 12 of 18 CPM neurons bound IB4 in the PenV1 plus axotomy condition. Surprisingly, 8 of 13 CPM neurons under control conditions were immunoreactive for TRPV1, which was significantly higher than that observed following axotomy plus PenV1 injections (4 of 18 CPMs were TRPV1 positive). This percentage of TRPV1 positive CPM fibers following PenCON injections here was also significantly higher than that observed previously following axotomy alone (Jankowski et al., 2009) and axotomy plus PenCON injections which utilized a different injection paradigm (Jankowski et al., 2010).

The increase in TRPV1+ CPM fibers following control siRNA injection raised the possibility that this injection paradigm (i.e. injections at 2 and 3 weeks after axotomy) may have resulted in additional damage possibly accelerating the gain of mechanical sensitivity in these previously mechanically insensitive CH fibers. We thus examined the expression of two transcription factors, Sox11 and ATF3, whose expression levels are known to increase dramatically following nerve injury (e.g. Jankowski et al 2006, 2008; Tsujino et al 2000) and two receptors, GFRα3 and P2Y1, that have been shown to play a role in the gaining of mechanical sensitivity by these fibers (Jankowski et al., 2010, 2012). However, we found no changes in the expression of these genes in the L2,3 DRG at four weeks after axotomy with PenCON injections at 2 and 3 weeks compared with axotomy alone (Sox11 −2±13%; ATF3 −17±30%; GFRα3 −1±17%; P2Y1 11±22%; n=4 for all comparisons). We also were able to verify previous data on CH neurons as all of these fibers (six) under both conditions stained positively for TRPV1 (Lawson et al 2008; Jankowski et al 2009a, 2010).

DISCUSSION

It has been previously shown that enhanced artemin levels in the skin can regulate TRPV1 expression in the DRGs (Elitt et al 2006). We and others have also previously shown that peripheral nerve axotomy increased artemin levels in the skin and increased levels of its receptor GDNF family receptor α3 (GFRα3) in the appropriate DRGs (Bennett et al 2000; Jankowski et al 2009a; 2010). In addition, we found that by 4 weeks after nerve cut, there was a significant increase in the expression of TRPV1 (Jankowski et al., 2009). Recently we have shown that inhibition of the axotomy-induced increase in GFRα3 blocked the observed recruitment of CH neurons and the increase in TRPV1 expression following regeneration (Jankowski et al 2010). These results suggested that putative enhanced signaling through the artemin/GFRα3 pathway after regeneration caused changes in TRPV1 expression, leading to CH neuron recruitment.

Here, using a previously established in vivo siRNA-mediated knockdown strategy (Jankowski et al 2009b), we tested whether the increase in TRPV1 expression alone could be responsible for CH neuron recruitment after regeneration. In vivo siRNA-mediated inhibition of injury-induced changes in TRPV1 expression blocked the normal recruitment of CH neurons without altering the injury induced decrease in CPM heat threshold four weeks after injury-Interestingly, upon rebound of the expression of TRPV1 in the DRGs at 10–12 weeks, we found a recovery of CH neuron recruitment in the mice that received TRPV1 targeting siRNA injection plus axotomy while the decrease in CPM heat threshold was unaffected. These results in conjunction with our previous report (Jankowski et al 2010) strongly suggest that dynamic changes in TRPV1 expression and not absolute levels tightly regulate the number of functional CH neurons in mice after injury.

Changes in TRPV1 expression after regeneration and the acquisition of mechanical sensitivity in the CH fiber population

In previous studies we obtained results suggesting that axotomy and successful regeneration (Jankowski et al., 2009a) lead to the acquisition of mechanical sensitivity in normally mechanically insensitive CH fibers, which is similar to what has been hypothesized in human chronic pain states (e.g. Orstavik et al 2003). In addition to blocking CH fiber recruitment, knockdown of the increase in GFRα3 expression following axotomy also blocked this change as no CPM fibers stained positively for TRPV1 (Jankowski et al., 2010). Here we found that TRPV1 knockdown resulted in the same percentage of TRPV1 positive CPM fibers seen following axotomy alone or with axotomy and control siRNA injections in our previous studies (Jankowski et al., 2009; 2010). This would suggest that the increase in TRPV1 expression following regeneration does not play a major role in the acquisition of mechanical sensitivity. This conclusion is also supported by the fact that following inflammation we have observed the same change in mechanical sensitivity without an apparent change in TRPV1 expression (Jankowski et al 2012). Together these findings suggest that while dynamic expression of TRPV1 is required for the gaining of heat sensitivity, it does not play a pivotal role in the acquisition of mechanical sensitivity normally seen following peripheral injury (Jankowski et al. 2009a; 2010, 2012).

However, it is important to note that in these experiments, we also observed an increase in TRPV1 positive CPM fibers following control siRNA injections that was significantly higher than the number of such fibers following TRPV1 targeted siRNA injections. Thus, we cannot rule out a potential role for TRPV1 in the gaining of mechanical sensitivity in these fibers. We have examined the possibility that the injection paradigm may have caused additional injury to the nerve which in turn could accelerate the acquisition of mechanical sensitivity. However, there were no changes in the expression of ATF3 or Sox11 transcription factors suggesting that as we documented in our earlier studies, these injections do not cause any significant injury to the nerve fibers. In addition we have recently suggested two other possible players in this acquisition of mechanical sensitivity; GFRα3 and the purinergic receptor P2Y1. Inhibition of GFRα3 was found to completely block the increase in TRPV1 positive CPMs after regeneration (Jankowski et al 2010) while inhibition of the expression of the P2Y1 receptor after inflammation has been shown to increase the numbers of TRPV1 immunopositive CPM neurons (Jankowski et al 2012). However, expression levels of neither receptor were altered after the two PenCON injections. On the other hand, we recently hypothesized that in the subpopulation of CH cells that contain both P2Y1 and TRPV1, P2Y1 expression may be decreased, but this decrease would not be discernable when measuring expression levels across the whole DRG. Thus it will be important to determine the expression levels in individual characterized cells in the future to fully understand the mechanisms of how this and other subpopulations of sensory neurons may alter peripheral response properties after injury and the receptors that may be involved. Nevertheless, the results presented here strongly suggest that an increase in TRPV1 levels is necessary for the increase in functional CH neurons following nerve injury and regeneration, but it also appears that this increase in TRPV1 expression is not necessary for these fibers to gain mechanical sensitivity following regeneration.

Acknowledgements

This research was supported by NS 023725; NS 052848 (HRK) and F32 NS 061487 (MPJ).

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