Increased local concentration of complement C5a contributes to incisional pain in mice
© Jang et al; licensee BioMed Central Ltd. 2011
Received: 2 May 2011
Accepted: 7 July 2011
Published: 7 July 2011
In our previous study, we demonstrated that local injection of complement C5a and C3a produce mechanical and heat hyperalgesia, and that C5a and C3a activate and sensitize cutaneous nociceptors in normal skin, suggesting a contribution of complement fragments to acute pain. Other studies also have shown that the complement system can be activated by surgical incision, and the systemic blockade of C5a receptor (C5aR) reduces incision-induced pain and inflammation. In this study, we further examined the possible contribution of wound area C5a to incisional pain.
Using of a hind paw incisional model, the effects of a selective C5aR antagonist, PMX53, on nociceptive behaviors were measured after incision in vivo. mRNA levels of C5 and C5aR in skin, dorsal root ganglia (DRG) and spinal cord, and C5a protein levels in the skin were quantified after incision. The responses of nociceptors to C5a were also evaluated using the in vitro skin-nerve preparation.
Local administration of PMX53 suppressed heat hyperalgesia and mechanical allodynia induced by C5a injection or after hind paw incision in vivo. mRNA levels of C5 and C5aR in the skin, but not DRG and spinal cord, were dramatically increased after incision. C5a protein in the skin was also increased after incision. In vitro C5a did not increase the prevalence of fibers with ongoing activity in afferents from incised versus control, unincised skin. C5a sensitized C-fiber afferent responses to heat; however, this was less evident in afferents adjacent to the incision. PMX53 blocked sensitization of C-fiber afferents to heat by C5a but did not by itself influence ongoing activity or heat sensitivity in afferents innervating control or incised skin. The magnitude of mechanical responses was also not affected by C5a in any nociceptive fibers innervating incised or unincised skin.
This study demonstrates that high locally generated C5a levels are present in wounds for at least 72 hours after incision. In skin, C5a contributes to hypersensitivity after incision, but increased responsiveness of cutaneous nociceptors to C5a was not evident in incised skin. Thus, high local concentrations of C5a produced in wounds likely contribute to postoperative pain.
The complement system is a biochemical cascade within the immune system most commonly associated with the enhancement of inflammation and direct attack of foreign organisms. Upon activation of the complement system, split fragments C5a and C3a augment inflammatory responses, e.g. increase blood flow and vascular permeability and facilitate migration of neutrophils and monocytes to the inflamed tissues. C5a and C3a also induce mast cells to release histamine and tumor necrosis factor-α (TNF-α), which contribute to the proliferation of the inflammatory response [1–4]. Other components of the local inflammatory response have been recognized to play roles in pain including cytokines, neuropeptides and neurotrophins . Complement fragments such as C5a may share this property.
Our previous study showed that local injection of complement C5a and C3a produce mechanical and heat hyperalgesia in vivo, and that C5a and C3a activate and sensitize cutaneous nociceptors in normal skin in vitro , suggesting complement fragments may contribute to pain. Furthermore, it has been shown that the complement system can be activated by surgical incision [7–9], and the systemic blockade of C5a receptor (C5aR) reduces incisional allodynia, edema and cytokine expression  implying a significant contribution of C5a to the inflammation and pain caused by incision.
Additional studies demonstrate that nociceptors immediately adjacent to the incision sequester NGF, have increased heat sensitivity and increase acid responsiveness [11–14]. However, important questions like whether sensitivity to complement fragments is altered in incised tissue or whether local populations of C5aR support incisional pain behaviors have remained unanswered. In this study, we tested whether the selective C5aR antagonist PMX53 can reduce incisional nociception when injected into peri-incisional skin in vivo, and if the responses of nociceptors to C5a are enhanced in incised skin when applied on the peripheral nociceptor terminals in vitro. We also examined whether the mRNA levels of C5 and C5aR are altered in skin, dorsal root ganglia (DRG) and spinal cord by incision in an attempt to further localize the likely site of action of C5a in supporting nociception after incision. C5a production in the skin after incision was directly measured as well.
Materials and methods
Male C57BL/6J mice (20-30 g and 6-12 weeks of age, Jackson Labs) that were housed in groups of 4-5 were used. Food and water available ad libitum under a 12-h light/dark cycle. Experimental protocols were approved by The Animal Care and Use Committees of the University of Iowa and the VA Palo Alto Health Care System.
Drug preparation and administration
Recombinant mouse C5a was purchased from R&D Systems, Inc. (Minneapolis, MN). The selective C5aR antagonist PMX53 (AcF-[OPdChaWR]) was the kind gift of Promics (Queensland, Australia). All drugs were dissolved in sterile 0.9% normal saline prior to use , and the PBS-vehicle was prepared in the same manner without adding drug.
For local injection of C5aR antagonist in the incisional model, injection (30 μg/15 μl) was performed 1 hour prior to paw incision. The same administration protocol was repeated 2 hours before each test session in the time course studies. The 2 hour time point was the point of maximal analgesic effect as determined in preliminary studies. For studies involving antagonism of the direct local effects of C5a, intraplantar injection of 10 μl C5a solution (200 ng) was accomplished using a 30 gauge needle and a microsyringe (Hamilton, Reno, NV). In these studies involving the systemic administration of C5aR antagonist, the concentration of PMX53 was adjusted so that a 3 mg/kg dose could be administered subcutaneously in the skin of the back in a 100 μl volume; PMX53 was administered 30 minutes prior to local C5a administration. This dose of PMX53 had been shown to be effective and selective in other studies [10, 15]. Vehicle injections were used in all studies.
In the electrophysiology study, we tested C5a 0.1 and 1 μg/ml. Because only one concentration of C5a could be applied to each fiber, full dose-response curves were not attempted. The higher concentration sensitized C-fibers to heat in normal skin in our previous study . The lower C5a concentration was included in this study to determine if there were enhanced responses in incised tissue. To ensure C5aR antagonism in the in vitro preparation, 0.9 μg/ml (1 μM) PMX53 was selected based on previous observations evaluating the potency of this compound in blocking C5a-induced leukocyte activation .
Mice were anesthetized with 1.5-2.0% isoflurane delivered through a nose cone, and the hindpaw of mouse was sterilized with 10% povidone-iodine. Plantar incision of hind paw in mice was performed as described previously by our labs [10, 17–19]. Briefly, a 0.5 cm incision was made through skin and fascia of the plantar hindpaw with a number 11 scalpel blade. The incision was started 0.2 cm from the proximal edge of the heel and extended distally. The underlying muscle was elevated with curved forceps, leaving the muscle origin and insertion intact. After hemostasis, the wound edges were opposed with a single 6.0 nylon mattress suture and the wound was covered with antibiotic ointment. For hairy skin incision, 0.5 cm incision was made with a number 11 surgical blade on the dorso-medial skin of the left hindpaw in the area innervated by the saphenous nerve. The skin was then closed with two subcutaneous mattress sutures with 6-0 nylon and covered with an antibiotic ointment. In some cases, the skin from both the left and right hindpaws were incised and utilized to minimize the number of animals required for the fiber recordings. In both plantar and hairy skin incision, control mice without incision underwent a sham procedure that consisted of anesthesia, antiseptic preparation, and application of the antibiotic ointment without an incision.
Mechanical nociceptive thresholds were assayed using von Frey filaments according to the "up-down" algorithm described by Chaplan et al.  as we described previously [21, 22]. Mice were placed on wire mesh platforms in clear cylindrical plastic enclosures of 10 cm diameter and 30 cm height. After 20 minutes of acclimation, von Frey fibers of sequentially increasing or decreasing stiffness were applied to the plantar surface of the right hindpaw and left in place for 5s using sufficient force to slightly bend the filament. Withdrawal of the hindpaw from the fiber was scored as a response. When no response was obtained, the next higher force in the series was applied to the same paw. If a response was obtained, a less stiff fiber was next applied. Testing proceeded in this manner until 4 fibers had been applied after the first one causing a withdrawal response allowing the estimation of the mechanical withdrawal threshold using a curve fitting algorithm .
Paw withdrawal response latencies to noxious heat stimulation were measured using the method of Hargreaves et al.  as we have modified for use with mice . In this assay, mice were placed on a temperature-controlled glass surface (29°C) in a clear plastic enclosure similar to those described for mechanical testing. After 30 min of acclimation, a beam of focused light was directed towards the same area of the hindpaw as described for the von Frey assay. A 20 s cutoff was used to prevent tissue damage. In these experiments, the light beam intensity was adjusted to provide an approximate 10 s baseline latency in control mice. Three measurements were made per animal per test session separated by at least one minute.
Analysis of C5 and C5aR mRNA
Mice were sacrificed at specific time points by CO2 asphyxiation. The skin tissue surrounding the incision with approximate 1.5-mm margins was excised. Spinal cord lumbar segments (L3-S1) were harvested by extrusion and rapid dissection on a pre-chilled surface. Dorsal root ganglia (DRG) were dissected using low power binocular magnification. All tissues were quick frozen in liquid nitrogen and stored at -80°C.
For RNA and real-time polymerase chain reaction (PCR), total RNA was isolated from skin, spinal cord and DRG using the RNeasy Mini Kit (Qiagen, Valencia, CA) according to the manufacturer's instructions. The purity and concentration were determined spectrophotometrically. The mRNA samples were reverse transcribed into complementary DNA (cDNA) using a First Strand cDNA Synthesis Kit (Invitrogen, Carlsbad, CA). Real-time PCR was performed in an ABI prism 7900HT system (Applied Biosystems, Foster City, CA). All PCR experiments were performed using the SYBR Green I master kit (Applied Biosystems). The primer sets for C5aR and 18S mRNA and the amplification parameters were described previously . Melting curves were performed to document single product formation and agarose electrophoresis confirmed product size. The C5a primers were purchased from SABiosciences (SABiosciences, Valencia, CA). As negative controls, RNA samples that were not reversibly transcribed were run. Data were normalized by 18S mRNA expression.
Analysis of C5a in the skin
Skin tissue harvest and protein isolation
Mice were euthanized at the time points specified in the figures. The skin tissue surrounding incision with approximate 1.5 mm margins was excised, and skin specimens were placed into phosphate-buffered saline containing a protease inhibitor cocktail (Roche Complete, Roche Diagnostics, Mannheim, Germany), and frozen at -80°C until analysis. For protein isolation these samples were first cut into small pieces with microscissors then disrupted using a Polytron Device (Brinkmann Instruments Inc, Westbury, NY). The samples were then centrifuged at 10,000 rpm at 4°C for 10 min. The supernatant was carefully pipetted into a fresh 1.5 ml tube, which was the material used for protein analysis. Protein concentration was evaluated with a DC Protein Assay kit (Bio-Rad Laboratories, Hercules, CA).
The complement anaphylatoxin C5a level in the skin of the wound site was determined by a mouse C5a DuoSet ELISA Kit according to the instruction provided by the company (R&D Systems, Minneapolis, MN). Briefly, the ELISA plate was coated with capture antibody, and followed by washing with washing buffer. After blocking of non-specific binding sites with blocking buffer, the plate was incubated with 100 μl of each sample or C5a standard in duplicate. After incubation and subsequent washing, detection antibody was added, followed by washing and incubation with streptavidin-HRP at 400 ng/ml. Substrate Solution was added into each well for the color reaction, and the reaction was stopped by addition of stop solution and the absorbance read at 450 nm in microplate reader.
In vitrosingle fiber recordings
One day after hairy skin incision or sham incision, mice were killed using CO2 inhalation, and the hairy skin from the dorso-medial hind paw was shaved and excised with the innervating saphenous nerve. Attached connective tissue, muscle and tendon were removed. To ensure a sufficient length of axon for recording, the nerve was dissected up to the lumbar plexus. The dissected skin-nerve preparation was fixed in a perfusion chamber with the epidermal side down. The chamber was continuously superfused with a "synthetic interstitial fluid" (SIF) , a solution consisting (mM) of 107 NaCI, 26.2 NaHCO3, 9.64 sodium gluconate, 5.5 glucose, 7.6 sucrose, 3.48 KCI, I .67 NaH2PO4, 1.53 CaCl2, 0.69 MgSO4 at 31 ± 1°C, which was bubbled with a mixture of 95% O2 and 5% CO2. The nerve, attached to the skin, was drawn through one small hole to the recording chamber, which was filled with paraffin oil. The nerve was placed on a fixed mirror, the sheath was removed and nerve filaments repeatedly teased to allow single fiber recordings to be made using platinum electrodes, one for recording and the other for reference. The reference electrode was grounded to the perfusion chamber. Single nociceptive afferent fibers were recorded extracellularly with a differential amplifier (DAM50, Harvard Apparatus, Holliston, MA). Neural activity was amplified and filtered using standard techniques. Amplified signals were relayed to an oscilloscope and an audio monitor and then into PC computer via a data acquisition system (spike2/CED1401 program). Action potentials collected on a computer were analyzed off-line with a template matching function of spike 2 software (version 4.24).
The search strategy was mechanical stimulation by a fire-polished glass rod; thus, all were mechanosensitive fibers. The conduction velocity of the axon was determined by monopolar or bipolar electrical stimulation through an epoxy-coated electrode with an uninsulated tip. The supramaximal square wave pulses (0.2-2 ms duration; 0.5 Hz) were delivered at the mechanosensitive site of the receptive field. The distance between receptive field and the recording electrode (conduction distance) was measured and divided by the latency of the action potential. The single fibers were classified as being either C- or A-fibers if their conduction velocity was slower than 1.2 m/s or between 1.2 and 8.0 m/s, respectively. The fast conducting (greater than 8.0 m/s) and rapidly adapting fibers were excluded. In this study, C-fibers were investigated for mechanical and heat responses; A-fibers surrounding the incision were included only for mechanical response experiments. In previous experiments [11, 13], C-fiber afferents with receptive fields within 2 mm of the incision were sensitized to heat and acid. We emphasized recording fibers from sham control skin and fibers innervating ≤ 2 mm from the incision. Some fibers from incised skin had receptive fields > 2 mm from the incision, these were analyzed separately.
The mechanosensitive receptive field of each fiber was isolated by placing a hollow metal cylinder with silicone grease which was added to prevent leakage from the bath into the receptive field. After a 2 min baseline recording, the SIF solution inside the ring was replaced with C5a (1 or 0.1 μg/ml) or PBS-vehicle in a 100 μl volume and fiber activity was recorded for 2 min.
In other experiments, after a 2 min baseline recording, the SIF solution inside the ring was replaced with PMX53 1.8 μg/ml in a 50 μl volume. After a 2 min exposure to PMX53, C5a 2 μg/ml or PBS-vehicle in a 50 μl volume was added into the ring so that the final concentration of PMX53 was 0.9 μg/ml combined with C5a 1 μg/ml (final concentration) or PBS-vehicle in a total volume of 100 μl. Then fiber activity was recorded for 2 min.
The fiber was considered activated by the drug if activity of at least 0.1 impulse/s was elicited if background activity was absent during baseline recording, or if ongoing activity was present, an increase of at least two standard deviations greater than the average baseline ongoing activity. For PMX53 application, some fibers had ongoing activity. If ongoing activity was present we noted if PMX53 decreased this activity. If the average activity decreased by at least two standard deviations from the baseline, it was considered a significant decrease.
After ongoing activity of C-fibers was assessed, the test solution inside the ring was aspirated to minimize heat dissipation and a thermocouple was gently placed to measure the subcutaneous temperature. A radiant heat lamp was placed in the translucent area underneath the organ bath and the light beam was focused onto the epidermal side of the skin. After 10 s baseline recording, a computer-controlled standard heat ramp was delivered starting from 32 to 45°C over 15 s by a customized heat stimulator (Bioengineering, University of Iowa, Iowa City, IA). The peak temperature, 45°C, was used to avoid potential tissue damage of higher temperatures. We previously determined that the temperature of the epidermal side was approximately 1°C higher than the subdermal side. Fibers having a receptive field in a previously heated area were avoided for subsequent recordings. Each fiber was tested with heat only once because previously we noted that repeated heating sensitized the fiber responses. Action potentials were counted for 20 s beginning from the onset of the heat, including the heat ramp application (15 s) and 5 s after the peak temperature when the temperature remained elevated to 41°C, for 'during heat' analysis. Action potentials between 20 s and 60 s after the onset of the heat were also counted for 'after heat' analysis that reflect after discharges following the stimulus. The temperature that elicited the first action potential during heat stimulation was considered as threshold if background activity was absent. If background activity was present, threshold was determined by the temperature during heating that increased background activity at least two standard deviations greater than the average baseline (10 s, 1 s bin). Background activity was subtracted from total action potential numbers during recording period, assuming background activity was sustained during the heat stimulus.
To avoid repeated application of drug for testing of heat and mechanical stimuli, mechanical responses were tested in separate experiments from heat. Servo-controlled mechanical stimulation (Series 300B dual mode servo system, Aurora Scientific, Canada) was used to measure mechanosensitivity of C- and A-fibers. The most sensitive spot of the receptive field of each fiber was isolated with a metal cylinder as described above. A flat and cylindrical metal probe (tip size 0.7 mm) attached to the tip of stimulator arm was placed onto the receptive field so that no force was generated. After a 2 min baseline recording, a computer-controlled ascending series of square force stimuli (5, 10, 20, 40 and 80 mN; 2 s duration; 60 s intervals) was applied to the receptive field. Then, the SIF solution inside the ring was replaced with C5a 1 μg/ml or PBS-vehicle solution with 100 μl volume without any movement of the mechanical probe or ring. After a 2 min drug application, the same series of mechanical stimuli was applied to the receptive field in the presence of applied drug. C-fibers were tested regardless of location of the receptive fields in relation to the incision; A-fibers ≤ 2 mm from the incision were studied. The force that elicited the first action potential during mechanical stimulation was considered threshold if background activity was absent. If background activity was present, threshold was determined by the force that increased activity by at least two standard deviations greater than the average background. Background activity was subtracted from the total number of action potentials during mechanical stimulation.
Parametric and non-parametric analyses were selected based on the Kolmogorov-Smirnov test for normal distribution (SigmaStat software. Jandel Corporation, San Rafael, CA). For electrophysiological data, all data were analyzed based on distances between receptive field and incision site: sham vs. incision ≤ 2 mm vs. incision > 2 mm group based on our previous studies [11, 13]. The heat response threshold, and total action potentials during and after heat stimulation were analyzed using t-test (two groups) and one-way analysis of variance (ANOVA) followed by Holm-Sidak correction (three groups) for parametric data analysis, or Mann-Whitney rank sum test (two groups) and Kruskall-Wallis ANOVA followed by Dunn's test (three groups) for non-parametric data analysis. A chi-square test was used to compare the percentage of fibers that had increased ongoing activity or to evaluate the proportion of afferents responding to heat and the proportion that changed background activity. Analysis of the mechanical stimulus-response relationship before and after drug was performed using two-way repeated measures ANOVA. Electrophysiological data for heat and mechanical data are presented as median value and means ± SEM, respectively. The behavioral and mRNA expression data were analyzed by two-way ANOVA followed by Bonferroni post-hoc test for multiple comparisons. Protein analysis was done by one-way ANOVA followed by Bonferroni post-hoc test for multiple comparisons. Behavior data and the expression of mRNA and protein are presented as means ± SEM. P values less than 0.05 were considered significant (Prism 4, GraphPad Software, La Jolla, CA).
PMX53 suppresses heat hyperalgesia and mechanical allodynia induced by hind paw incision
PMX53 suppresses heat hyperalgesia and mechanical allodynia induced by C5a
C5a and C5aR mRNA
C5a production in Skin
Single fiber recording
In this preparation, 14 of 38 (36.8%) fibers treated with PBS-vehicle had significant spontaneous activity (at least 0.1 impulse/s); activity decreased in 2 of 14 spontaneously active fibers (14.2%) after PBS-vehicle. Of those exposed to PMX53 1.8 μg/ml, 9 of 42 (21.4%) fibers were spontaneously active; only 3 of 9 spontaneously active fibers (33.3%) decreased ongoing activity after PMX53 application (data not shown). For all spontaneously active C-fibers, regardless of proximity to the incision, no differences were observed in the proportion that decreased activity after PMX53 vs. PBS-vehicle. Thus, there was no apparent contribution of C5a to this ongoing activity that is present in vitro based on responses to PMX53.
In the PBS-vehicle treated tissue, a high percentage of C-fibers (49/57, 85.9%) in all groups responded to heat (Figure 7E, I and 7M). There was no difference in the proportion of fibers responding to heat among the sham group and those with receptive fields ≤ 2 mm and > 2 mm from the incision. Almost all C-fibers (85/91, 93.4%) responded to heat after application of C5a (1 or 0.1 μg/ml), however, incision, compared to sham, did not increase the heat responses to C5a or the proportion of C-fibers responding to heat.
In this study, mRNA levels of C5 and C5aR, and C5a protein in the skin were dramatically increased after incision. Blockade of C5aR in vivo using a selective C5aR antagonist, PMX53, decreased exogenous C5a-induced heat and mechanical hypersensitivity. PMX53 alleviated incision-induced heat hypersensitivity at 24 hours and decreased mechanical hypersensitivity later at 48 hours. In vitro PMX53 blocked sensitization of C-fiber afferents to heat by C5a but did not by itself influence ongoing activity or heat sensitivity in afferents innervating control or incised skin. C5a sensitized C-fiber afferent responses to heat; this was less evident in afferents adjacent to the incision. C5a did not elicit a greater prevalence of increased ongoing activity in afferents from incised versus unincised control tissue. The magnitude of mechanical responses was also not affected by C5a in any nociceptive fibers innervating incised or unincised skin. Altogether, high local concentrations of C5a contribute to enhanced behavioral responses to heat 1 day after incision and also to mechanical responses on day 2 and thereafter. High local C5a expression rather than increased responsiveness of nociceptors to C5a contributes to hypersensitivity after incision.
The hind paw incision induced heat and mechanical hypersensitivity, and these hypersensitivities were significantly attenuated by local blockade of C5aR in the hind paw (Figure 1), highlighting the contribution of peripheral C5a to incisional pain. Heat, but not mechanical sensitization was reduced by C5aR blockade early after incision, i.e. within the first 24 hours. PMX53 was also able to suppress behavioral hyperalgesia induced by local injection of C5a (Figure 2). Hyperalgesia caused by the application of other inflammatory mediators, e.g. zymosan, carrageenan and lipopolysaccharide have also been associated with C5aR activation . Our studies here suggest that at least at early time points, C5a alters the heat sensitivity of C-fibers more markedly than mechanical sensitivity. Apparently the contribution of peripheral C5a signaling to mechanical sensitization is a relatively minor contributor to sensitization early as opposed to later times after incision. The contribution of central C5a in neuropathic pain has been suggested [28, 29]; however it remains to be determined whether it also holds true for postoperative pain.
mRNA and protein expression
The mRNA levels of C5 and C5aR after incision were locally plastic, but we did not find evidence for C5 system plasticity within the DRG or central nervous systems (Figure 3). While C5 levels near incisions peak early and remain elevated (Figure 3 and 4), local C5aR changes only become significant at about 24 hours after incision. Though we have shown C5a can act directly on afferent fibers , we observed no increase in C5aR expression in the DRG or spinal cord after incision. Thus, the up-regulation of C5 and C5aR after incision appears to be locally restricted, and perhaps related to the known expression of C5/C5aR by neutrophils and intrinsic cells of the skin.
Application of C5a to nociceptive terminals directly activated few C-fibers in both sham and incised tissue (Figure 5); therefore enhanced activation by C5a on incision is not evident. Based on the lack of effect of PMX53 applied to the receptive field of spontaneously active fibers (Figure 6), no significant contribution of C5a to the ongoing activity in the incised skin nerve preparation was observed.
In previous studies, incision sensitized nociceptors to heat and lactic acid in skin [11, 30]. Afferents in muscle were also sensitized by incision; heat, mechanical and acid responsiveness were enhanced compared to unincised muscle . It was surprising that incision did not enhance the ability of C5a to sensitize C-fiber afferents to heat or produced spontaneous activity. In fact responses to C5a were not significantly different than vehicle in afferents ≤ 2 mm from the incision. The lack of significance may be due to the fact that some fibers were already sensitized to heat by incision , and the effects of additionally applied C5a on heat responses on afferents adjacent to the incision may be saturated. Because the heat responses (e.g. threshold and total number of action potentials during and after heat) tend to be sensitized in afferents adjacent to the incision (Figure 7F-H), the study may be underpowered to detect a further significant change by C5a. It is possible that mechanically insensitive fibers contribute to heat hyperalgesia in incised and control tissue as well. Some mechanically insensitive fibers could become mechanosensitive after incision, and contribute to heat responses; however, this can not be determined in this protocol. Based on the heat responses after PMX53 application alone (Figure 8), the C5aR does not contribute to heat responses of C-fibers in the incised in vitro preparation.
C5a-induced mechanical hyperalgesia occurs in vivo in naïve animals (Figure 2B). In the present study and in a previous study, neither C-fibers (Figure 9C) nor A-fibers sensitized to mechanical stimuli in sham control tissue , and C5a did not affect mechanical responsiveness of C- or A-fibers in skin from mice that had undergone incision 24 h earlier (Figure 9). Mechanical hypersensitivity may be secondary to other in vivo elements activated by complement which are removed in the skin nerve preparation. Also, the brief treatment period in vitro may not be sufficient to cause mechanical sensitization that occurs as early as 30 min after complement injection in vivo. Finally, because mechanical sensitization of nociceptors has been less apparent than heat sensitization in several studies, many propose that mechanical hypersensitivity is in part due to sensitization in the central nervous system .
The possible role of C5a in incisional pain
Based on observations that C5aR mRNA is expressed in primary sensory neurons and the intracellular calcium level is elevated by C5a treatment in cultured DRG neurons in vitro , behavioral sensitization after incision could be caused by a direct binding of C5a to its peripheral receptors. At the same time, it is also possible that C5a plays a role in incisional pain by indirect mechanisms. C5a is one of the most potent inflammatory molecules known to induce proinflammatory functions such as upregulation of cytokine and chemokine production, and it is also a strong chemoattractant for neutrophils, monocytes and macrophages that can release a mixture of algogenic substances, e.g. histamine, interleukins, TNF-α and others [1–4, 33, 34] which produce heat and mechanical hyperalgesia when injected into hind paw [35–41]. In support, mRNA levels of peripheral C5 and C5aR were markedly increased in the incised skin but not DRG or spinal cord after incision (Figure 3), implying the recruitment of inflammatory cells to the incision site. Our previous study showed several locally produced cytokines from incisions were dependent on C5aR . Thus, these indirect effects of C5a on nociceptive sensitization may be as important as the effects of C5a itself on sensory neurons.
Additionally, activation of small diameter nociceptors by C5a may contribute to behavioral sensitization by releasing various algesic substances e.g. glutamate, neuropeptides and ATP in the peripheral and central terminals to sensitize dorsal horn neurons [42–45] and nociceptors [46–50]. However, this does not occur immediately after application to skin in vitro. It is possible that application of C5a for several hours in vitro could induce mechanical sensitization; however, this can not be tested.
In summary, treatment with a selective C5aR antagonist, PMX-53, decreased heat and mechanical hypersensitivity induced by incision or by local administration of C5a in vivo. The increase of C5a protein level in the incised skin was observed. The mRNA levels of C5 and C5aR in the skin were increased after incision, but not in the DRG and spinal cord. The sensitivity of nociceptors to C5a was not significantly enhanced by incision in vitro. Therefore, the reduced hypersensitivity resulting from PMX53 administration in vivo is caused by blockade of receptor activation produced by high local concentrations of C5a. In the future, the effect of drugs like PMX53 on clinical postoperative pain could be considered.
This research was supported by the Department of Anesthesia at the University of Iowa and National Institutes of Health, Bethesda, Maryland Grant GM079126-02S1 to Drs. Clark and Brennan.
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