Pain and Regional Anesthesia
Differential Spinal Cord Gene Expression in Rodent Models of Radicular and Neuropathic Pain
LaCroix-Fralish, Michael L. B.S.*; Tawfik, Vivianne L. B.Sc.*; Tanga, Flobert Y. M.S.†; Spratt, Kevin F. Ph.D.‡; DeLeo, Joyce A. Ph.D.§
Background: Neuropathic pain and radicular low back pain both have a major impact on human health worldwide. Microarray gene analysis on central nervous system tissues holds great promise for discovering novel targets for persistent pain modulation.
Methods: Rat models of lumbar radiculopathy (L5 nerve root ligation) and neuropathy (L5 spinal nerve transection) were used for these studies. The authors measured mechanical allodynia followed by analysis of global gene expression in the lumbar spinal cord at two time points (7 days and 14 days) after surgery using the Affymetrix RAE230A GeneChip® (Santa Clara, CA). The expression patterns of several genes of interest were subsequently confirmed using real-time reverse transcriptase polymerase chain reaction.
Results: The authors observed similarly robust mechanical allodynia in both models. Second, they observed significant differences in lumbar spinal cord gene expression across chronic pain models. There was little overlap between genes altered in each injury model, suggesting that the site and type of injury produce distinct spinal mechanisms mediating the observed mechanical allodynia. The authors further confirmed a subset of the genes using reverse transcriptase polymerase chain reaction and identified several genes as either neuropathy-associated genes or radiculopathy-associated genes.
Conclusions: These two models of persistent pain produce similar allodynic outcomes but produce differential gene expression. These results suggest that diverging mechanisms lead to a common behavioral outcome in these pain models. Furthermore, these distinct pathophysiologic mechanisms in neuropathic versus radicular pain may implicate unique drug therapies for these types of chronic pain syndromes.
Click on the links below to access all the ArticlePlus for this article.
Please note that ArticlePlus files may launch a viewer application outside of your web browser.
ONE form of persistent pain, chronic low back, affects more than two thirds of the Western population at any given time,1
and a recent study2
suggests that approximately half of these patients experience a neuropathic element to their low back pain. Furthermore, the healthcare cost of painful neuropathic disorders, including diabetic neuropathy, causalgia, and back or neck pain with neuropathic involvement, has been estimated to total threefold more than matched controls.3
Clinically, patients present with pain of multiple etiologies and varying symptoms; differential responses to treatment are therefore common and not unexpected. The development and introduction of novel analgesics guided by a refined knowledge of the pathogenesis of pain is dire.
Pain researchers have developed several animal models mimicking chronic pain-like behaviors to study the cellular and molecular correlates of aberrant pain transmission. To date, most pain research using animal models has focused on injury to a peripheral nerve, usually the sciatic or spinal nerve 4–9
. In addition, specific animal models of nerve root or radicular pain have also been developed.10–13
Although Wall and Devor14
and Kawakami et al.11,13
have postulated the importance of the location of a nerve injury to the severity of clinical symptoms, there have been few studies comparing nerve lesions central to the dorsal root ganglion (DRG) versus
peripheral. Root lesions central to the DRG lead to a different sequence of events as compared with lesions of peripheral nerves14
; therefore, it is imperative to investigate the unique pathophysiologic changes that occur after injury to these distinct sites.
In recent years, the development of high-density microarray technology has allowed investigators to determine the expression levels of several thousand messenger RNA (mRNA) transcripts concurrently.15,16
The utility of these assays in identifying candidate genes involved in the development of chronic pain syndromes has been proposed.17,18
Specifically, gene expression patterns after peripheral nerve injury in rats has been investigated in the DRG19,20
and spinal cord,21–23
as well as in peripheral nerve stumps after sciatic axotomy24
and spinal cord after spinal cord injury–inducing central pain.25
Taken together, these studies have identified several hundred candidate genes, many of which have yet to be confirmed by secondary assays, which may help to describe the complex cellular and molecular cascade triggered by nerve injury.
Here we describe the use of two of these models: L5 nerve root ligation (LR), a central radicular injury with an inflammatory component, and L5 spinal nerve transection (L5tx), a peripheral nerve injury. Previously, we have demonstrated that these models differ in their responses to drug therapy; specifically, radicular pain has been previously shown to be resistant to a cytokine antagonist cocktail (interleukin-1 receptor antagonist and soluble tumor necrosis factor receptor), whereas in a peripheral neuropathic pain model, this cocktail was effective in reducing tactile allodynia.26
These findings led us to question whether peripherally induced neuropathic and centrally induced radicular pain produced differential spinal cord gene expression.
Materials and Methods
Male Sprague-Dawley (Hsd:Sprague-Dawley) rats used in this study were obtained from Harlan Sprague-Dawley (Indianapolis, IN) and were approximately 8 weeks of age at the time of surgery. All animals were housed one per cage under US Department of Agriculture and Association for Assessment and Accreditation of Laboratory Animal Care International–approved conditions with a 12:12-h light–dark cycle and free access to food and tap water. Care was taken to minimize animal discomfort and to limit the number of animals used. All experimental procedures were approved by the Dartmouth College Institutional Animal Care and Use Committee (Lebanon, New Hampshire). All surgical procedures were performed during inhalation anesthesia induced with 4% gaseous halothane in oxygen and maintained at 1.5–2%.
Animals were divided into two groups according to the site of injury used: (1) a group of rats (n = 2/time point) that received a unilateral mononeuropathy by transection of the L5 spinal nerve (L5tx) distal to the L5 dorsal root ganglion,27–29
or (2) a group of rats (n = 2/timepoint) that received an experimental lumbar radiculopathy (LR) with loose ligation of the dorsal and ventral L5 nerve roots with 5-0 chromic gut suture along with placement of 5 pieces (3–5 mm in length) of 4-0 chromic gut on the nerve roots.10,30
Two sham groups (n = 2/group) were prepared by performing the surgical procedures without either nerve transection or nerve root ligation.
The development of mechanical allodynia was assessed using 2-g (20.02 mN) and 12-g (115.26 mN) calibrated von Frey filaments (Stoelting, Wood Dale, IL) by a single investigator blinded to the surgical status of the rats. In each testing session, the animals were subjected to 30 tactile stimulations to the plantar surface of the ipsilateral (nerve-injured) hind paw in the region of the L5 innervation. Mechanical allodynia was assessed by recording the total number of responses elicited during three successive trials (10 stimulations/trial, 30 stimulations total) separated by at least 10 min. The resulting data were then expressed as the percent responses out of total possible responses. Animals were acclimated to the testing procedure twice before the surgical procedure to record baseline values. Any animals displaying abnormal baseline paw withdrawals were excluded from the study.
Tissue Isolation and RNA Preparation
Rats were quickly killed by carbon dioxide asphyxiation followed by decapitation. The spinal cord was then quickly removed, rinsed in phosphate-buffered saline (PBS), and immediately placed on dry ice. Total RNA was prepared from the lumbar region of the spinal cord of the sample using the TRIzol reagent (Invitrogen, Carlsbad, CA) according to the manufacturer’s recommended protocol. The crude RNA was further purified using RNeasy columns (Qiagen Inc., Valencia, CA) according to manufacturer’s RNA cleanup protocol. Spectrophotometric analysis was used to quantify RNA concentration and to assess sample purity.
Affymetrix GeneChip® Microarray Protocol
Affymetrix RAE230A GeneChip® microarrays (Santa Clara, CA) containing 4,699 known rat sequences, 700 nonexpressed sequence tags and 10,467 expressed sequence tags, were used for these experiments. Approximately 5 μg of starting RNA was used for each sample. The double-stranded complementary DNA (cDNA), created using SuperScript II (Invitrogen) reverse transcriptase, was used as a template for an in vitro transcription reaction using biotin-labeled nucleotides to synthesize the labeled complementary RNA samples to be hybridized to the microarrays (BioArray HighYield RNA Transcript Labeling Kit [T7], Cambridge BioScience, Cambridge, United Kingdom). A second purification procedure was performed and the labeled RNA was fragmented at 94°C for 35 min. For each sample, hybridization cocktails were assembled, including 20 μg of fragmented biotin-labeled RNA and hybridization controls as established by Affymetrix. Two hundred microliters of hybridization cocktail, containing 15 μg of probe, was loaded onto each GeneChip® and placed in a 45°C rotisserie at 60 rpm for 16 h to hybridize (GeneChip® Hybridization Oven 640). After the hybridization step, the Affymetrix Fluidics Station 400 was used to administer streptavidin-phycoerythrin and antibody stains to the microarrays. The individual GeneChips® were then scanned using the Agilent GeneArray Scanner.
GeneChip® Normalization and Expression Level Analysis
The individual raw image.DAT files from each individual microarray were normalized to the group median intensity using DNA-Chip Analyzer software (dChip version 1.3#
) as described previously.31,32
After normalization, the individual expression levels for each gene were calculated using the probe match–mismatch (pm-MM) model–based expression index. The calculated expression levels for each gene were then used in the subsequent statistical analyses to determine which genes from each experimental GeneChip® were differentially expressed as compared with control GeneChips®.
Microarray Data Analysis
In this study, the treatment groups were 7 days postinjury, 14 days postinjury, and 7 days post–sham surgical control, with three gene expression comparisons of interest (7 days–sham, 14 days–sham, and 14 days–7 days). With these three comparisons for each of the two groups defined by the different nerve injury models (L5 nerve root ligation or L5 spinal nerve transection), a total of six separate analyses were performed to identify outliers. Two animals were used for each treatment. The stability of scores between animals in each treatment group was evaluated using the Cronbach α internal consistency reliability index as well as a test–retest reliability estimate. Extremely high reliability estimates supported the decision to average the gene expression scores for each group. For the linear regression model, the target group (e.g., 7 days post–L5 nerve root ligation) was regressed on the reference group (e.g., sham) and a confidence interval around the prediction of Y (7 days post–L5 nerve root ligation) from X (sham) established. The target gene was then defined to be an outlier if the observed score (Y) was outside of the confidence interval. In this study, with 15,866 probe sets being examined, a 99% confidence interval around the regression line was chosen as the basis for defining a discrepancy between the predicted and observed gene expression sufficiently large to suggest differential gene expression. All analyses were performed using SAS version 9.1 (SAS Institute Inc., Cary, NC).
Quantitative Real-time RT-PCR
The purified total RNA from the lumbar spinal cords from a replicate surgical experiment (n = 3/group) Sprague-Dawley rats was reverse transcribed to cDNA using the Superscript III First Strand Synthesis kit (Invitrogen). The resulting cDNA was diluted to 10 ng/μl. Primers for rat glyceraldehyde 3-phosphate dehydrogenase (GAPDH), decorin (DCN), aquaporin (AQP4), insulin-like growth factor 1 (IGF1), insulin-like growth factor 2 (IGF2), prostaglandin D2 synthase (PTGDS), insulin-like growth factor binding protein 3 (IGFBP3), CD74 antigen (HLADG), glial fibrillary acidic protein (GFAP), and integrin-αM (ITGAM) were designed according to our previously published protocol33
and are shown in supplementary table 1 (additional information regarding this is available on the Anesthesiology Web site at http://www.anesthesiology.org
). Primers were synthesized by Applied Biosystems (Foster City, CA). The quantitative real-time reverse transcriptase polymerase chain reaction (RT-PCR) reactions were performed in a total reaction volume of 25 μl containing a final volume of 12.5 μl of SYBR® Green PCR Master Mix (Applied Biosystems), 900 nm of forward and reverse primers, and 5 μl of diluted cDNA (10 ng/μl). The reactions were performed in 96-well plates using the iCycler IQ Multicolor Real-Time PCR detection system (Bio-Rad, CA). The CT
values for each quantitative real-time RT-PCR reaction were determined using the iCycler software (Bio-Rad). Relative expression of each of the genes was determined using the 2−ΔΔCT
using the expression of GAPDH as a control housekeeping gene. All samples gave a single peak upon melt curve analysis, indicating there were no contaminating products or primer dimers for the genes assayed.
Statistical significance for the behavioral experiments was determined by mixed factorial analysis of variance followed by Bonferroni multiple comparison post hoc test using GraphPad Prism version 4.02 (GraphPad Software Inc., San Diego, CA). Statistical significance for the RT-PCR experiments was determined by one-way analysis of variance followed by Bonferroni multiple comparison post hoc test. A statistical threshold of α = 0.05 (P < 0.05) was considered significant for all experiments.
Mechanical Allodynia in Rats after L5 Nerve Root Ligation and L5 Spinal Nerve Transection
We have previously demonstrated that both the L5 nerve root ligation model of lumbar radiculopathy (LR) and the L5 spinal nerve transection model (L5tx) of peripheral neuropathy produce reliable, robust, and long-lasting mechanical allodynia.26,29,35–37
In this study, age-matched male Sprague-Dawley rats exhibited robust mechanical allodynia after LR and L5tx beginning at day 1 after surgery and lasting throughout the testing period. During the course of the study, no significant difference in the magnitude of mechanical allodynia was observed between the LR and L5tx groups in response to the 2-g (fig. 1A
) or 12-g (fig. 1B
) von Frey filaments. No significant mechanical allodynia was observed in either sham surgery group (fig. 1
Identification of Differential Gene Expression
In these experiments, gene expression values ranged from 1 to 12,237, with 95% of the scores below 1,000 in most cases. The reliability estimates associated with the gene expression scores within experimental groups (i.e.
, replicates) are summarized in table 1
. We observed high reliability estimates for both the internal consistency (coefficient α) and the test–retest reliability estimates, with all indices exceeding 0.97. From this analysis, we determined that replicate consistency was considered adequate grounds for averaging the results from replicate rats from each group before evaluating differences in gene expression across the experimental groups. Differential gene expression across experimental groups was evaluated by using a linear regression method. We followed this analysis with further classification of the genes identified by the linear regression method based on the relative magnitude change to group the genes into subcategories based on expression magnitudes.
Peripheral Nerve Transection and Nerve Root Ligation Induce Differential Spinal Cord Gene Expression after Injury
Microarray analysis of gene expression in the lumbar spinal cord at two time points (7 days and 14 days) after LR or L5tx was performed. In the 7 days postsurgery groups, we identified 417 genes (2.6% of total probesets) regulated in the L5tx rats (figs. 2A and B
) and 386 genes (2.4% of total probesets) in the LR rats (figs. 2C and D
). Further subsetting of the L5tx outlier genes by fold change from the L5tx sham-operated group showed 49 genes with a greater than 1.5-fold change, 186 genes with a 1- to 1.5-fold change, 179 genes with a −1- to −1.5-fold change, and 3 genes with a greater than −1.5-fold change (fig. 2B
). Similarly, further subsetting of the LR outlier genes by fold change from the LR sham-operated group showed 29 genes with a greater than 1.5-fold change, 176 genes with a 1- to 1.5-fold change, 164 genes with a −1- to −1.5-fold change, and 17 genes with a greater than −1.5-fold change (fig. 2D
Of these specific L5tx and LR genes, we identified 139 genes (17.3% of L5tx/LR outlier genes) that were coordinately regulated in both models (fig. 2E
). These commonly regulated genes were nearly equally distributed between up-regulated genes (7 genes with a greater than 1.5-fold change, 68 genes with a 1- to 1.5-fold change) and down-regulated genes (61 genes with a −1- to −1.5-fold change, 3 genes with a greater than −1.5-fold change). A summary of the outlier genes identified 7 days after surgery can be found in supplementary table 2 (additional information regarding this is available on the Anesthesiology Web site at http://www.anesthesiology.org
In the 14 days postsurgery groups, we identified 367 genes (2.3% of total probesets) regulated in the L5tx rats (figs. 3A and B
) and 362 genes (2.3% of total probesets) in the LR rats (figs. 3C and D
). Further subsetting of the L5tx outlier genes by fold change from the L5tx sham-operated group showed 7 genes with a greater than 1.5-fold change, 161 genes with a 1- to 1.5-fold change, 188 genes with a −1- to −1.5-fold change, and 11 genes with a greater than −1.5-fold change (fig. 3B
). Similarly, further subsetting of the LR outlier genes by fold change from the LR sham-operated group showed 16 genes with a greater than 1.5-fold change, 154 genes with a 1- to 1.5-fold change, 161 genes with a −1- to −1.5-fold change, and 31 genes with a greater than −1.5-fold change (fig. 3D
Of these specific L5tx and LR genes, we identified 132 genes (18.1% of L5tx/LR outlier genes) that were coordinately regulated in both models (fig. 3E
). Commonly regulated genes in the 14 days postinjury group were also nearly equal between up-regulated genes (4 genes with a greater than 1.5-fold change, 67 genes with a 1- to 1.5-fold change) and down-regulated genes (56 genes with a −1- to −1.5-fold change, 5 genes with a greater than −1.5-fold change). A summary of the outlier genes identified 14 days after surgery can be found in supplementary table 3 (additional information regarding this is available on the Anesthesiology Web site at http://www.anesthesiology.org
We observed differences in gene expression across the two time points measured as well. In the LR group, we found 62% of the genes to be differentially regulated between the two time points after L5 nerve root ligation. Similarly, in the L5tx group, we found 64% of the genes to be differentially regulated between the two time points after L5 spinal nerve transection.
We further classified the model-specific, nonexpressed sequence tag, outlier genes into functional categories at days 7 and 14 after surgery (fig. 4
). Genes that were commonly expressed in both models were not included. This analysis suggests that functional groups of genes that were differentially regulated at day 7 between the two nerve injury models occurred in genes involved in enzyme/metabolism (33% L5tx vs.
19% LR). At day 14 after surgery, the functional groups of genes that were differentially regulated were involved in enzyme/metabolism (29% L5tx vs.
20% LR), channels/transporters (7% L5tx vs.
14% LR), and structural proteins (11% L5tx vs.
Confirmation of Microarray Targets via Real-time RT-PCR
To confirm the potential genes identified by the microarray analyses, we performed real-time RT-PCR analysis on lumbar spinal cord homogenates from a second group of male Sprague-Dawley rats 7 days after LR or L5tx. We chose PTGDS, IGF1, IGF2, IGFBP3, DCN, HLADG, and AQP4 that were identified as model-specific outlier genes expressed at 7 days after L5tx or LR (fig. 5
). In addition, we chose two genes previously shown to be regulated in both models,26
GFAP and ITGAM. The relative expression of these genes compared with their corresponding sham-operated controls as measured by both Affymetrix microarray analysis and real-time RT-PCR is summarized in table 2
. We observed paradoxical differences in the expression of DCN in the LR group and HLADG in the L5tx group between the two assays. These differences were not significantly different (P
> 0.05) from each other, suggesting some interassay or interanimal variability or both. It is notable, however, that we were able to confirm by a secondary method eight out of nine genes that we selected from the microarray analysis.
As demonstrated previously,26
the astrocyte marker, GFAP, and the microglial marker, ITGAM, were significantly increased in both models of nerve injury (figs. 5A and B
). Similarly, PTGDS, which converts PGH2
and is thought to play a role in PGE2
-induced allodynia, was up-regulated approximately 2-fold after both L5tx and LR (fig. 5C
). In this study, we have identified several novel genes uniquely regulated after L5tx, including DCN, IGF1, IGF2, and IGFBP3. Several genes in the insulin-like growth factor family (IGF1, IGF2, and IGFBP3) were increased 5- to 10-fold in the L5tx group but not in the LR group (figs. 5D–F
). Also notable was DCN, a member of the small, leucine-rich proteoglycan family known to interact with the epidermal growth factor receptor,38
was significantly increased approximately 6-fold after L5 nerve transection but was unchanged after LR surgery (fig. 5G
). In contrast, we found that HLADG (aka CD74), the major histocompatability class II (MHC-II)–associated invariant chain, is increased (approximately 1.4-fold) only after LR surgery and showed no increase in the L5tx animals (fig. 5H
). We observed no significant difference in AQP4 expression between any of the treatment groups (fig. 5I
is defined as pain caused by a lesion of the peripheral or central nervous system manifesting with sensory signs and symptoms.39
The DRG is the boundary dividing the central and peripheral nervous systems, and this nomenclature implies that lesions distal to the DRG are peripheral, whereas injuries proximal to the DRG are central. Clinically, a peripheral nerve injury (such as our L5 nerve transection model) presents with a “burning” pain with occasional lancinating pain that is sometimes controlled with opioid analgesics, gabapentin, and tricyclic antidepressants. Radicular pain, however, has a neuropathic (i.e.
, nerve root injury) component, although there are no accepted diagnostic criteria for defining it.40
Acute low back pain is often managed with nonsteroidal antiinflammatory drugs and muscle relaxants,41
whereas chronic radicular pain with obvious disc involvement is often managed surgically with varying degrees of success. For example, the number of spine surgeries with fusion has increased dramatically within recent years without an adequate evidence base to justify its use.42
In a different study, surgical discectomy demonstrated a significantly higher success rate compared with nonsurgical treatment.43
Clearly, there is significant disconnect in the clinical approaches to treating neuropathic pain and chronic radicular pain. Therefore, in the current study, we sought to determine whether radiculopathy and neuropathy differed in their abilities to alter spinal gene transcription in an effort to identify novel candidate genes that may be pain etiology subtype specific. We observed that these two models display similar magnitudes of mechanical allodynia. Furthermore, gene expression patterns diverged significantly. Many genes were found to be coregulated in the two models and likely represent a basic set of genes transcriptionally altered by any type of injury to the nervous system, whereas other genes diverged significantly between the two models.
A similar magnitude of mechanical allodynia to tactile stimulus was observed after both the L5tx (peripheral) and LR (central) models of chronic pain, in agreement with a previously published study.26
This finding, in light of the differences in the site and type of nerve injury used in these two models, suggests that allodynia as a symptom or phenomenon is a behavioral outcome mediated by several different pathophysiologic pathways. This concept has been explored in a previous study in which allodynia from the L5tx and LR models was shown to correlate significantly across six strains of mice.30
These data also suggest that treating neuropathies originating from disparate sites of injury (e.g.
, central vs.
peripheral) with pharmacotherapies developed for their ability to treat specific symptoms (e.g.
, antiallodynic drugs) without regard to the unique pathophysiologic mechanisms that underlie each type injury may not be globally effective.
Our laboratory, among others, has extensively investigated the role of central nervous system neuroimmune activation (glial activation and immune mediator expression) in the development and maintenance of chronic pain states.28,44,45
As in the current study, previous results have shown that markers for astrocytic and microglial activation (GFAP and OX-42, respectively) were found to be similarly increased in both injury models.26
These findings suggest that because of their central spinal placement, glial cells may participate in the genesis and maintenance of pain, regardless of the site of the precipitating injury.
A group of genes belonging to the insulin-like growth factor family were confirmed to be up-regulated after injury exclusively in the L5tx group. Insulin-like growth factor-I (IGF-I, somatomedin C) and insulin-like growth factor-II (IGF-2, somatomedin A) are small, mitogenic polypeptides that act as general growth and/or trophic factors for all central nervous system cell types.46
Previous studies have demonstrated up-regulation of IGF-I after peripheral nerve freeze injury47
or peripheral nerve crush.48
Together, these findings suggest that the insulin-like growth factors may be a peripheral nerve injury–specific response that may be involved in axonal regeneration, a function not required after LR injury.
Previously, we have observed spinal MHC class II expression after both peripheral and nerve root injury with a qualitatively greater expression after nerve root injury. Interestingly, peripheral inflammation from either zymosan49
did not lead to MHC class II expression in the spinal cord. Furthermore, decreased MHC class II expression after administration of the immunosuppressant agents methotrexate or leflunomide was associated with a decrease in existing mechanical allodynia after injury.51,52
In the current study, we observed an increase in the mRNA for the HLADG gene, which encodes the invariant polypeptide chain of MHC class II, after LR but not L5tx. This suggests a transcriptional regulation of the HLADG gene after root injury proximal to the DRG.
Two previous studies by Wang et al.22
and Yang et al.21
have examined, using microarray technology, gene expression in the spinal cord after spinal nerve ligation or sciatic nerve transection, respectively. Both studies examined gene expression at 14 days after injury and, thus, are comparable to our 14 days post-L5tx group. The experiments by Yang et al.21
show few correlative genes as compared with the current study, most likely because of differences in the microarray platform (cDNA spotted arrays vs.
Affymetrix GeneChip®). In contrast, comparing the study by Wang et al.22
with the current study demonstrates several genes that are positively identified in both studies (e.g.
, MHC class II genes, complement protein genes, CD37 leukocyte antigen).
Overall, our results suggest that the characteristic patterns of spinal gene transcription observed after peripheral or nerve root injury may implicate differential responses in neuropathic and radicular pain. We found unique gene expression patterns after LR and L5tx surgery, with surprisingly little overlap between the groups (only 8.7% and 10.9% at days 7 and 14, respectively). We also observed a significant time effect on the gene expression after nerve injury, which suggests different phases of gene expression at different time points after spinal nerve and nerve root injury. All of these differential gene expression profiles may explain divergent behavioral outcomes as well as distinct analgesic responsiveness in peripheral nerve and root injury models26
and in human pain conditions. This suggests that the site of injury makes a seminal contribution to the ensuing spinal plasticity, which has key implications for therapy. Specifically, although similar pain responses may be observed (patients often exhibit allodynia, dysesthesias, and hyperesthesias) the underlying mechanisms may differ, suggesting that radicular and neuropathic syndromes may respond to unique drug therapies. These findings further suggest that chronic pain may be responsive to specific pharmacotherapy depending on the site of injury and that the current trend toward treating radicular pain principally with surgery may need to be reexamined. Finally, our findings highlight the importance of elucidating basic pain mechanisms to allow for the development of etiology-specific treatments with increased efficacy over currently available therapies.
The authors thank Ausra Milano, Ph.D. (Research Associate, Department of Genetics, Dartmouth College, Hanover, New Hampshire), for her expert analysis of the microarray experiments and Nancy Nutile-McMenemy, M.S. (Research Assistant, Department of Anesthesiology, Dartmouth College), for her editorial assistance.
1. Andersson GB: Epidemiological features of chronic low-back pain. Lancet 1999; 354:581–5
2. Kaki AM, El-Yaski AZ, Youseif E: Identifying neuropathic pain among patients with chronic low-back pain: Use of the Leeds Assessment of Neuropathic Symptoms and Signs pain scale. Reg Anesth Pain Med 2005; 30:422–8
3. Berger A, Dukes EM, Oster G: Clinical characteristics and economic costs of patients with painful neuropathic disorders. J Pain 2004; 5:143–9
4. Bennett GJ, Xie YK: A peripheral mononeuropathy in rat that produces disorders of pain sensation like those seen in man. Pain 1988; 33:87–107
5. DeLeo JA, Coombs DW: Autotomy and decreased spinal substance P following peripheral cryogenic nerve lesion. Cryobiology 1991; 28:460–6
6. DeLeo JA, Coombs DW, Willenbring S, Colburn RW, Fromm C, Wagner R, Twitchell BB: Characterization of a neuropathic pain model: sciatic cryoneurolysis in the rat. Pain 1994; 56:9–16
7. Kim SH, Chung JM: An experimental model for peripheral neuropathy produced by segmental spinal nerve ligation in the rat. Pain 1992; 50:355–63
8. Seltzer Z, Dubner R, Shir Y: A novel behavioral model of neuropathic pain disorders produced in rats by partial sciatic nerve injury. Pain 1990; 43:205–18
9. Wall PD, Scadding JW, Tomkiewicz MM: The production and prevention of experimental anesthesia dolorosa. Pain 1979; 6:175–82
10. Hashizume H, DeLeo JA, Colburn RW, Weinstein JN: Spinal glial activation and cytokine expression after lumbar root injury in the rat. Spine 2000; 25:1206–17
11. Kawakami M, Weinstein JN, Chatani K, Spratt KF, Meller ST, Gebhart GF: Experimental lumbar radiculopathy. Behavioral and histologic changes in a model of radicular pain after spinal nerve root irritation with chromic gut ligatures in the rat. Spine 1994; 19:1795–802
12. Olmarker K, Larsson K: Tumor necrosis factor alpha and nucleus-pulposus-induced nerve root injury. Spine 1998; 23:2538–44
13. Kawakami M, Weinstein JN, Spratt KF, Chatani K, Traub RJ, Meller ST, Gebhart GF: Experimental lumbar radiculopathy: Immunohistochemical and quantitative demonstrations of pain induced by lumbar nerve root irritation of the rat. Spine 1994; 19:1780–94
14. Wall PD, Devor M: Sensory afferent impulses originate from dorsal root ganglia as well as from the periphery in normal and nerve injured rats. Pain 1983; 17:321–39
15. Schena M, Shalon D, Davis RW, Brown PO: Quantitative monitoring of gene expression patterns with a complementary DNA microarray. Science 1995; 270:467–70
16. Lipshutz RJ, Fodor SP, Gingeras TR, Lockhart DJ: High density synthetic oligonucleotide arrays. Nat Genet 1999; 21:20–4
17. Mirnics K, Pevsner J: Progress in the use of microarray technology to study the neurobiology of disease. Nat Neurosci 2004; 7:434–9
18. Griffin RS, Mills CD, Costigan M, Woolf CJ: Exploiting microarrays to reveal differential gene expression in the nervous system. Genome Biol 2003; 4:105
19. Costigan M, Befort K, Karchewski L, Griffin RS, D’Urso D, Allchorne A, Sitarski J, Mannion JW, Pratt RE, Woolf CJ: Replicate high-density rat genome oligonucleotide microarrays reveal hundreds of regulated genes in the dorsal root ganglion after peripheral nerve injury. BMC Neurosci 2002; 3:16
20. Xiao HS, Huang QH, Zhang FX, Bao L, Lu YJ, Guo C, Yang L, Huang WJ, Fu G, Xu SH, Cheng XP, Yan Q, Zhu ZD, Zhang X, Chen Z, Han ZG, Zhang X: Identification of gene expression profile of dorsal root ganglion in the rat peripheral axotomy model of neuropathic pain. Proc Natl Acad Sci U S A 2002; 99:8360–5
21. Yang L, Zhang FX, Huang F, Lu YJ, Li GD, Bao L, Xiao HS, Zhang X: Peripheral nerve injury induces trans-synaptic modification of channels, receptors and signal pathways in rat dorsal spinal cord. Eur J Neurosci 2004; 19:871–83
22. Wang H, Sun H, Della Penna K, Benz RJ, Xu J, Gerhold DL, Holder DJ, Koblan KS: Chronic neuropathic pain is accompanied by global changes in gene expression and shares pathobiology with neurodegenerative diseases. Neuroscience 2002; 114:529–46
23. Islamov RR, Hendricks WA, Katwa LC, McMurray RJ, Pak ES, Spanier NS, Murashov AK: Effect of 17 beta-estradiol on gene expression in lumbar spinal cord following sciatic nerve crush injury in ovariectomized mice. Brain Res 2003; 966:65–75
24. Kubo T, Yamashita T, Yamaguchi A, Hosokawa K, Tohyama M: Analysis of genes induced in peripheral nerve after axotomy using cDNA microarrays. J Neurochem 2002; 82:1129–36
25. Nesic O, Lee J, Johnson KM, Ye Z, Xu GY, Unabia GC, Wood TG, McAdoo DJ, Westlund KN, Hulsebosch CE, Regino Perez-Polo J: Transcriptional profiling of spinal cord injury-induced central neuropathic pain. J Neurochem 2005; 95:998–1014
26. Winkelstein BA, Rutkowski MD, Sweitzer SM, Pahl JL, DeLeo JA: Nerve injury proximal or distal to the DRG induces similar spinal glial activation and selective cytokine expression but differential behavioral responses to pharmacologic treatment. J Comp Neurol 2001; 439:127–39
27. Colburn RW, DeLeo JA, Rickman AJ, Yeager MP, Kwon P, Hickey WF: Dissociation of microglial activation and neuropathic pain behaviors following peripheral nerve injury in the rat. J Neuroimmunol 1997; 79:163–75
28. Colburn RW, Rickman AJ, DeLeo JA: The effect of site and type of nerve injury on spinal glial activation and neuropathic pain behavior. Exp Neurol 1999; 157:289–304
29. Tawfik VL, LaCroix-Fralish ML, Nutile-McMenemy N, DeLeo JA: Transcriptional and translational regulation of glial activation by morphine in neuropathic pain. J Pharmacol Exp Ther 2005; 313:1239–47
30. LaCroix-Fralish ML, Rutkowski MD, Weinstein JN, Mogil JS, DeLeo JA: The magnitude of mechanical allodynia in a rodent model of lumbar radiculopathy is dependent on strain and sex. Spine 2005; 30:1821–27
31. Li C, Hung Wong W: Model-based analysis of oligonucleotide arrays: Model validation, design issues and standard error application. Genome Biol 2001; 2:1–11
32. Li C, Wong WH: Model-based analysis of oligonucleotide arrays: Expression index computation and outlier detection. Proc Natl Acad Sci U S A 2001; 98:31–6
33. Tanga FY, Raghavendra V, DeLeo JA: Quantitative real-time RT-PCR assessment of spinal microglial and astrocytic activation markers in a rat model of neuropathic pain. Neurochem Int 2004; 45:397–407
34. Livak KJ, Schmittgen TD: Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) method. Methods (Duluth) 2001; 25:402–8
35. Winkelstein BA, DeLeo JA: Nerve root injury severity differentially modulates spinal glial activation in a rat lumbar radiculopathy model: Considerations for persistent pain. Brain Res 2002; 956:294–301
36. Sweitzer SM, Colburn RW, Rutkowski M, DeLeo JA: Acute peripheral inflammation induces moderate glial activation and spinal IL-1beta expression that correlates with pain behavior in the rat. Brain Res 1999; 829:209–21
37. Sweitzer SM, Schubert P, DeLeo JA: Propentofylline, a glial modulating agent, exhibits antiallodynic properties in a rat model of neuropathic pain. J Pharmacol Exp Ther 2001; 297:1210–7
38. Santra M, Reed CC, Iozzo RV: Decorin binds to a narrow region of the epidermal growth factor (EGF) receptor, partially overlapping but distinct from the EGF-binding epitope. J Biol Chem 2002; 277:35671–81
39. Backonja MM: Defining neuropathic pain. Anesth Analg 2003; 97:785–90
40. Dworkin RH, Backonja M, Rowbotham MC, Allen RR, Argoff CR, Bennett GJ, Bushnell MC, Farrar JT, Galer BS, Haythornthwaite JA, Hewitt DJ, Loeser JD, Max MB, Saltarelli M, Schmader KE, Stein C, Thompson D, Turk DC, Wallace MS, Watkins LR, Weinstein SM: Advances in neuropathic pain: Diagnosis, mechanisms, and treatment recommendations. Arch Neurol 2003; 60:1524–34
41. Carragee EJ: Clinical practice: Persistent low back pain. N Engl J Med 2005; 352:1891–8
42. Weinstein JN, Bronner KK, Morgan TS, Wennberg JE: Trends and geographic variations in major surgery for degenerative diseases of the hip, knee, and spine. Health Aff (Millwood) 2004; Suppl Web Exclusive: VAR81-9
43. Atlas SJ, Deyo RA, Keller RB, Chapin AM, Patrick DL, Long JM, Singer DE: The Maine Lumbar Spine Study: II. 1-year outcomes of surgical and nonsurgical management of sciatica. Spine 1996; 21:1777–86
44. DeLeo JA, Tanga FY, Tawfik VL: Neuroimmune activation and neuroinflammation in chronic pain and opioid tolerance/hyperalgesia. Neuroscientist 2004; 10:40–52
45. DeLeo JA, Yezierski RP: The role of neuroinflammation and neuroimmune activation in persistent pain. Pain 2001; 90:1–6
46. D’Ercole AJ, Ye P, Calikoglu AS, Gutierrez-Ospina G: The role of the insulin-like growth factors in the central nervous system. Mol Neurobiol 1996; 13:227–55
47. Sjoberg J, Kanje M: Insulin-like growth factor (IGF-1) as a stimulator of regeneration in the freeze-injured rat sciatic nerve. Brain Res 1989; 485:102–8
48. Kanje M, Skottner A, Sjoberg J, Lundborg G: Insulin-like growth factor I (IGF-I) stimulates regeneration of the rat sciatic nerve. Brain Res 1989; 486:396–8
49. Sweitzer SM, White KA, Dutta C, DeLeo JA: The differential role of spinal MHC class II and cellular adhesion molecules in peripheral inflammatory versus
neuropathic pain in rodents. J Neuroimmunol 2002; 125:82–93
50. Fu KY, Light AR, Matsushima GK, Maixner W: Microglial reactions after subcutaneous formalin injection into the rat hind paw. Brain Res 1999; 825:59–67
51. Hashizume H, Rutkowski MD, Weinstein JN, DeLeo JA: Central administration of methotrexate reduces mechanical allodynia in an animal model of radiculopathy/sciatica. Pain 2000; 87:159–69
52. Sweitzer SM, DeLeo JA: The active metabolite of leflunomide, an immunosuppressive agent, reduces mechanical sensitivity in a rat mononeuropathy model. J Pain 2002; 3:360–8
# Available at: http://www.dchip.org/
. Accessed August 20, 2005. Cited Here...
This article has been cited 16 time(s).
Nature Reviews NeuroscienceNuclear calcium signalling in the regulation of brain functionNature Reviews Neuroscience
Neuroscience LettersNovel candidate genes identified in the brain during nociception in common carp (Cyprinus carpio) and rainbow trout (Oncorhynchus mykiss)Neuroscience Letters
PainComplement activation in the peripheral nervous system following the spinal nerve ligation model of neuropathic painPain
European Journal of PainComparison of dorsal root ganglion gene expression in rat models of traumatic and HIV-associated neuropathic painEuropean Journal of Pain
PainProfiling of dynamically changed gene expression in dorsal root ganglia post peripheral nerve injury and a critical role of injury-induced glial fibrillary acetic protein in maintenance of pain behaviorsPain
Journal of NeurochemistryMinocycline decreases in vitro microglial motility, beta(1)-integrin, and Kv1.3 channel expressionJournal of Neurochemistry
Bmc NeuroscienceDifferential expression of Cathepsin S and X in the spinal cord of a rat neuropathic pain modelBmc Neuroscience
Gene Expression Profile of Dorsal Root Ganglion in a Lumbar Radiculopathy Model
PainMorphine, nortriptyline and their combination vs. placebo in patients with chronic lumbar root painPain
Molecular PainOrigins, actions and dynamic expression patterns of the neuropeptide VGF in rat peripheral and central sensory neurones following peripheral nerve injuryMolecular Pain
Journal of NeuroscienceT-Cell Infiltration and Signaling in the Adult Dorsal Spinal Cord Is a Major Contributor to Neuropathic Pain-Like HypersensitivityJournal of Neuroscience
Aquaporins in Sensory and Pain Transmission
Current Neuropharmacology, 8(2):
NeuroscienceSpinal cord transcriptional profile analysis reveals protein trafficking and RNA processing as prominent processes regulated by tactile allodyniaNeuroscience
Journal of NeuroscienceComplement induction in spinal cord microglia results in anaphylatoxin C5a-mediated pain hypersensitivityJournal of Neuroscience
PainHDAC inhibitors attenuate the development of hypersensitivity in models of neuropathic painPain
Neurobiology of Learning and MemoryCellular, molecular, and epigenetic mechanisms in non-associative conditioning: Implications for pain and memoryNeurobiology of Learning and Memory
Supplemental Digital Content
© 2006 American Society of Anesthesiologists, Inc.
Publication of an advertisement in Anesthesiology Online does not constitute endorsement by the American Society of Anesthesiologists, Inc. or Lippincott Williams & Wilkins, Inc. of the product or service being advertised.