Jump to ContentJump to Main Navigation
Show Summary Details
More options …

Scandinavian Journal of Pain

Official Journal of the Scandinavian Association for the Study of Pain

Editor-in-Chief: Breivik, Harald

CiteScore 2018: 0.85

SCImago Journal Rank (SJR) 2018: 0.494
Source Normalized Impact per Paper (SNIP) 2018: 0.427

See all formats and pricing
More options …
Volume 10, Issue 1


Stimulation-induced expression of immediate early gene proteins in the dorsal horn is increased in neuropathy

Ognjen Bojovic / Clive R. Bramham / Arne Tjølsen
Published Online: 2016-01-01 | DOI: https://doi.org/10.1016/j.sjpain.2015.09.002


Background and aims

Peripheral neuropathic pain is described as a pain state caused by an injury or dysfunction of the nervous system, and could have clinical manifestations such as hyperalgesia, allodynia and spontaneous pain. The development of neuropathic pain may depend on long-term forms of neuronal plasticity in the spinal cord (SC). Expression of the immediate early gene proteins (IEGPs) Arc, Zif268, and c-Fos are implicated in establishment of long-term potentiation (LTP) induced by conditioning stimulation (CS) of primary afferent fibres. However, the impact of the neuropathic state (Bennett’s model) on CS-induced expression of IEGPs has not been studied. The aim of this study was to compare the levels of Arc, c-Fos and Zif268 immunoreactivity prior to and after conditioning stimulation in animals with developed neuropathic pain, with sham operated, non-ligated controls.


Twenty-four animals were divided equally into the neuropathic and non-neuropathic groups. Neuropathic pain was induced in all animals by conducting a loose ligation of the sciatic nerve with Chromic Catgut 4.0 sutures 7 days prior to conditioning stimulation or sham operation. The loose ligation was performed by placing sutures around the sciatic nerve compressing the nerve slightly just enough to reduce but not completely diminish the perineural circulation. A state of neuropathy was confirmed by a significant decrease in mechanical withdrawal threshold measured by von Frey’s fibres. Immunohisto-chemical analysis was performed on transverse sections obtained from the L3-L5 segments of the SC at 2 and 6 h post-CS and IEGP positive cells were counted in lamina I and II of the dorsal horn. During statistical analyses, the groups were compared by means of analysis of variance (univariate general linear model). If significant differences were found, each set of animals was compared with the sham group with post hoc Tukey’s multiple comparison test.


Strikingly, all IEGPs exhibited a significant increase in immunoreactivity at both time points compared to time-matched, sham operated controls. Maximal IEGP expression was found 2 h after CS in neuropathic rats, and there was a smaller but still significant increase 6h after CS. The unstimulated side of the dorsal horn in stimulated animals did not show any significant change of the number of IEGP positive cells and was approximately at the same level as sham operated animals. The number of IEGP positive cells in sham operated controls (non-neuropathic and non-stimulated animals) showed same immunoreactivity in 2 and 6 h post sham operation.

Conclusion and implications

The neurophysiological process of neuropathic pain development is complex and needs to be studied further in order to clarify its nature and components. This present study is meant to reveal a step towards further understanding the role of Arc, c-Fos and Zif268 in neuropathic pain. Moreover, this study might contribute to the knowledge base for further research on better therapeutic possibilities for neuropathic pain.

Keywords: Sciatic nerve ligation; Neuropathic pain; Immediate early gene proteins; Arc; Fos; Zif268

1 Introduction

Neuropathic pain has been defined as a pain state caused by an injury or dysfunction of the nervous system, and has clinical manifestations such as hyperalgesia, allodynia and spontaneous pain [1,2]. Many etiological factors can lead to neuropathy as nerve compression or damage leading to partial or total nerve ligation. The nerve can be damaged on different locations between the CNS and the peripheral nerve ending [3].

However, there has been limited therapeutic success with drugs such as NSAIDS, opiates [4], anticonvulsants and antidepressants [5] against neuropathic pain. One of the best known animal models of neuropathic pain development is the loose sciatic nerve ligation described by Bennett [6], in which the sciatic nerve gets partially injured by light constriction of the sciatic nerve with a loosely tied thread.

Long-term potentiation (LTP) as a response to conditioning stimulation (CS) of afferent fibres is a common model of synaptic plasticity in the brain and the spinal cord [7]. Many hippocampal studies are used as a source on mechanisms of LTP formation, function and maintenance [8]. LTP has been divided into two phases, early and late, where the late phase has been proven to require de novo protein synthesis [9]. Immediate-early gene proteins (IEGP) such as early growth response protein 1 (Egr-1) (also known as Zif 268 - zinc finger protein 225) and activity regulated cytoskele-tal protein (Arc) have been found to be required for the process of late-phase LTP establishment in the hippocampus [9,10]. In the spinal cord, the most effective type of stimulation to induce LTP has been shown to be a series of high-frequency (e.g. 100 Hz) trains of electric stimulation [11]. Previous studies have shown that peripheral stimulation of afferent fibres leads to an increase of expression of c-Fos mRNA in spinal cord neurons and synaptic Arc protein [12,13].

Nociceptive information in the spinal cord is acquired, processed and transmitted mainly by nociceptive specific neurons (NS) and wide dynamic range neurons (WDR). The NS neurons are most abundant in Lamina I and II and respond to intense stimuli [14,15] while in deeper in laminae V and VI, WDR neurons are most abundant. Our research focused on Lamina I and II whose borders were previously defined in the research of Molander et al. [16]. Furthermore, it was shown that WDR neurons react in a graded manner to gentle touch, stronger mechanical and noxious stimulations [17].

Previous studies have shown elevated c-Fos, Zif268 and Arc immunoreactivity in neuropathic rats where neuropathy was induced by means of various methods such as the Bennett protocol [18] and Kim and Chung protocol [19]. However, it is not known whether CS-induced expression of IEGPs in the spinal cord dorsal horn differs between neuropathic and non-neuropathic states. Here, we compared CS-induced of IEGPs in the Bennett model of neuropathic pain relative to shame operated, non-ligated controls. The present study contributes to the clarification of the highly complex process of neuropathic pain formation. The protocol of sciatic nerve ligation represents a model of constriction nerve injury, such as a nerve injury present during spinal nerve root constriction caused by disc prolapse, or nerve constriction in the carpal tunnel syndrome.

2 Materials and methods

2.1 Animals and surgery

Female Sprague-Dawley rats, 2-3 months of age, weighing 240-300 g were used (NTac:SD, Taconic Europe, Ejby, Denmark). The animals had free access to food and water and were held on a 12/12-h light/dark cycle.

Twenty-four animals were divided in two groups of twelve animals, the neuropathic and non-neuropathic groups. All animals underwent a surgical intervention where the non-neuropathic animals were sham operated while the sciatic nerve of the neuropathic rats was ligated. All animals were operated under brief Isoflurane anaesthesia. Neuropathic pain was induced by means of surgical procedures previously described [6]. During this intervention, the common sciatic nerve was revealed by a blunt dissection through the biceps femoris muscle. Around 10 mm of the nerve was freed of adhering tissue and 4 ligatures with 4/0 chromic catgut (Chromic Catgut 1/2 circle, 4.0 round bodied; from KRUUSE Norge) were tied loosely around it with 1- 2 mm spacing between them and constricted to a degree previously described [6] to reduce the diameter of the nerve by a just noticeable amount [5]. The sutures were placed on the caudal part of the sciatic nerve, leaving the upper, cranial part free from sutures. The cranial part will further on be the location for stimulation electrode placement.

To check the level of allodynia as a clinical indication of neuropathic pain, the mechanical withdrawal thresholds were tested first at baseline before surgery and afterwards from the 4th post-surgery day with von Frey’s filaments of varying thickness. Before testing, the animal was placed in an elevated Plexiglas cage with a wire mesh floor and allowed to adapt for 10 min. The mid-plantar surface of the rats’ hind paws was stimulated with von Frey’s filaments through the wire mesh floor until the filament bent slightly. During allodynia testing we used 14 von Frey filaments, numbers 1-20 (Somedic Sverige) with a calibrated stiffness corresponding to 0.008, 0.02, 0.04, 0.07, 0.16, 0.4, 0.6, 1.0, 1.4, 2, 4, 6, 8, 10, 15, 26, 60,100,180 and 200 g. The filaments are presumed to roughly represent a logarithmic scale of applied force and a linear scale of perceived force (information provided by the manufacturer: North Coast Medical Inc.). As previously described [20] the filaments were applied to each hind paw in an order of increasing stiffness and the withdrawal threshold of each individual hind paw was defined as the force (in grams) of the filament that induced three of five positive responses (brisk withdrawal). The non-lesioned side served as a control, displaying no effect of the contralateral loose nerve ligation [20].

The baseline response thresholds before surgical intervention in the non-affected side were >60-70g pressure [20]. Allodynia was defined as severe if the response was positive to the filaments with a stiffness corresponding to 0.16-1.0 (g) (four filaments 0.16; 0.40, 0.60 and 1.0 g). Allodynia was defined as moderate if the animals responded to filaments with a stiffness corresponding to 1.4-6.0 (g) (four filaments 1.4, 2.0,4.0 and 6.0). Mild allodynia was positive if the animals responded to the filaments with a stiffness corresponding to 8.0-26 (g) (four filaments 8.0,10,15 and 26).

Both the neuropathic and non-neuropathic group was divided in 2 sub-groups, the two and six-hour groups with six animals per subgroup. Every subgroup was divided into 2 smaller groups, one stimulated and one sham operated small group. Each small group consisted of three animals, where the animals of the stimulated small group received CS while the control animals were sham operated without receiving the actual CS.

On the 7th day after nerve ligation or sham operation the animals were first checked for withdrawal threshold as previously described, and then anaesthetized with 1.7-2.2-mg/kg urethane (250mg/ml in sterile water) injected intraperitoneally. Animals were then checked for presence of pedal and corneal reflexes whose absence indicated an appropriate level of anaesthesia. After shaving of the surgery areas, the rats were transferred to a heating pad and during the whole process of stimulation and waiting, the animal body temperature was kept at 37 °C.

The left sciatic nerve was re-dissected from the surrounding muscles on the thigh so that a total length of 1-2 cm of the nerve was exposed. Proximal to the nerve division and proximal to the ligatures, the nerve was placed in a bipolar silver hook electrode (2 mm distance between hooks). The hooks were isolated from the surrounding tissue by means of elastic plastic film (Parafilm, American Can Company, USA).

All animals were perfused, dependent of the group, 2 or 6 h after CS or after the sham operation.

2.2 Sciatic nerve stimulation

A conditioning stimulation (CS) consisting of 10 stimulus trains, with stimulus duration of 0.5 ms, amplitude of 7.2 mA, a frequency of 100 Hz, train duration of 2 s and 8 s intervals between trains was used to stimulate all animals except the sham-operated groups. These characteristics of CS have shown to be approximately four times the threshold for C-fibre evoked neuronal firing [7] and have been shown to induce LTP in the dorsal horn of intact animals [21]. CS was given via a PC with Spike2 software coupled via a Digitimer 1401 interface to a stimulator (Neurolog Systems with Stimulus isolator NL800) connected to the bipolar silver hook. The sham-operated animals underwent surgery and sciatic nerve mounting on the silver hook electrodes without actually CS delivery.

2.3 Immunohistochemistry

After reflex testing that showed abolishment of corneal and pedal reflexes the animals were transcardially perfused with a 4 °C, 4% paraformaldehyde (PFA) in 0.1 M phosphate buffer with pH 7.4. After fixing the animal’s scull in a stereotaxic frame, one cranial-caudal incision was made from the medial occipital region to the top of the inter-ilium bone line on the skin to reveal the processi spinosi and the paravertebral musculature [22].

Six segments of the spinal cord (Th13-L5 segments) were dissected out. Thereafter, the caudal pieces that contained the L3-L5 segments of the spinal cord were cut from the residual trunk frozen in custom made aluminium foil wells (Ø8 mm) in dry ice and kept at -80 °C. A technician at this point marked the spinal cord samples so that the following procedures continued without knowledge of the time post CS or treatment of animal groups. The information of the pretreatment and the time point was sealed, and the seal was broken when all results were obtained.

From this tissue part, the cranial 3.2 mm of the frozen L3-L5 trunk was transverse sectioned in 20 μm thick sections. In this manner, the sections were taken from the region L3/L4 which was in our previous research found to be the area of the spinal cord with maximal cellular IEGP response after sciatic nerve stimulation. The sections were mounted on Superfrost GOLD slides (Braunschweig, Germany) so that each slide contained a number of sections for each time point and control sections.

Spinal cord sections were first washed in PBST (0.1% Triton X in PBS) and blocked in blocking buffer for 1 h (3% horse serum, 0.3% Triton X in PBS). Afterwards they were incubated overnight in primary antibody diluted in PBST (0.1% Triton X), 3% normal horse serum at 4°C. After three 5 min washes in PBST, the section were incubated with biotinylated secondary antibody in PBST for 2 h at room temperature. Sections were then washed 3 times 5 min in PBST and incubated in streptavidin-HRP diluted in PBST for 1 h, washed again in the same way, and 3,3'-diaminobenzidine (DAB) stained for 8 min approximately at room temperature under a microscope to control the colour development. The slides were then washed in Milli-Q water three times and stained for 5 min with 0.1% Cresyl Violet (pre heated to 50°C). The slides were then washed 3 times with Milli-Q water and subsequently immersed 3 min in each of four baths with increasing ethanol concentration (75%, 90%, 96%, and 96%) and 3 min in two 100% xylene baths. The sections were cover-slipped with DPX mounting medium, and were dried in RT 24 h before imaging.

Mouse anti-Arc monoclonal antibody (1:300 dilution) was purchased from Santa Cruz Biotechnology (cat. #sc-17839), rabbit anti-c-Fos (1:1000 dilution) polyclonal antibody was from Cal-biochem (cat. #PC38T) and rabbit anti-zif 268 (Egr-1) (1:300 dilution) was from Santa Cruz Biotechnology (cat. # sc-110). Secondary antibodies were biotin-conjugated anti-mouse IgG (cat. #PK-4002 VECTASTAIN® ABC Kit, Vector laboratories) or biotin-conjugated anti-rabbit IgG (cat. #PK-6101 VECTASTAIN® ABC Kit, Vector Laboratories).

The same person (OB) analyzed all sections. For each stimulated animal, time point and treatment, 32 sections were analyzed for every antibody used. For all three IEGPs the analyzed sections were distributed evenly over the entire area of interest explained previously. As controls, sham operated animals were used and every stimulated animal had as its own control a sham operated animal, that had received exactly the same treatment except the conditioning stimulus. IEGP positive cells were counted in lamina I and II using lamina border differentiation previously defined in the research of Molander et al. [16]. Cells were identified as positive if they showed clear staining of the nucleus with or without staining of the cytoplasm or cellular extensions as defined by Haugan et al. [7].

The stimulated and non-stimulated sides from all dorsal horn sections were imaged (Nikon Eclipse E-600; NIS elements software; resolution 2560 × 1920; colour depth 24-bit RGB) with 400× magnification. All neurons were manually counted in digital pictures and during counting the neurons were labelled to avoid double-counting.

We performed negative controls for all three antibodies (Arc, c-Fos and Zif268) by incubating the sections as previously described but without the primary antibody. These procedures led to elimination of all specific staining.

2.4 Ethical considerations

The experiments were approved by the Norwegian Committee on Research in Animals, and were carried out in accordance with the European Communities Council directive of 24 November 1986 (86/609/EEC). Efforts were made to minimize the number of animals used, and experiments were designed to minimize suffering.

2.5 Statistics

Graphpad Prism 6.0 and SPSS 22.0 were used for graphical representation and statistical evaluation of our results.

The effect of Bennett’s loose sciatic nerve ligation was evaluated by the means ± S.E.M. of unpaired Student’s t-test used to compare mean mechanical response thresholds (in grams) between subjects before and after the operation calculated with use of von Frey’s fibres (Fig. 1A and B).

(A and B) Change in foot withdrawal to von Frey fibres in sham operated and neuropathic animals. (A) Changes in foot withdrawal threshold to von Frey hair stimulation measured daily, 3 days before surgery and 7th day after surgery (N = 12) on operated side of animal, after unilateral sciatic nerve sham operation. Data given as mean withdrawal threshold in grams (g). (B) Changes in foot withdrawal threshold to von Frey hair stimulation measured daily, 3 days before surgery and 7th day after surgery (N = 12) on operated side of animal, after unilateral sciatic nerve loose ligation. Data given as mean withdrawal threshold in grams (g).
Fig. 1

(A and B) Change in foot withdrawal to von Frey fibres in sham operated and neuropathic animals. (A) Changes in foot withdrawal threshold to von Frey hair stimulation measured daily, 3 days before surgery and 7th day after surgery (N = 12) on operated side of animal, after unilateral sciatic nerve sham operation. Data given as mean withdrawal threshold in grams (g). (B) Changes in foot withdrawal threshold to von Frey hair stimulation measured daily, 3 days before surgery and 7th day after surgery (N = 12) on operated side of animal, after unilateral sciatic nerve loose ligation. Data given as mean withdrawal threshold in grams (g).

To compare the quantitative difference for all IEGPs, a uni-variate general linear model of statistical analyzes was applied. Here we conducted comparisons between the 2 and 6h post-stimulation groups and the control (sham-operated) groups. The stimulation/non-stimulation, neuropathic/non-neuropathic and time point were used as independent variables while the number of positive cells was used as the dependent variable. Statistical significance was accepted at the 1% level (Fig. 2A-C). If a significant effect of stimulation was found, each set of animals was compared with the sham group with post hoc Tukey’s multiple comparison test. Separate controls (for non-neuropathic and neuropathic) were used for each treatment group, but data for different time points within the same treatment group were merged since the number of positive cells within same treatment groups, as expected, did not show significant variation with time.

(A-C) Number of IEGP positive cells in the dorsal spinal cord in stimulated and sham operated animals 2 and 6h after conditioning stimulation. A (Arc), B (c-Fos), C (Zif268). For each time point, for each IEGP, the mean number of positive cells of the 6 sections with highest numbers of cells (N = 3 animals) was calculated, and the graphs show the means ± S.E.M. of these values. (‘NoNS’ - non-neuropathic stimulated animals; ‘NS’ – neuropathic stimulated; ‘NoNN’ – non-neuropathic non-stimulated; ‘N’ – neuropathic animals.) During statistical analyzes, the univariate general linear model was used and significance accepted at the 1% level (**p < 0.01). The control bars consist of one control bar for NoNN (2 h and 6 h post sham operation) and one for N animals.
Fig. 2

(A-C) Number of IEGP positive cells in the dorsal spinal cord in stimulated and sham operated animals 2 and 6h after conditioning stimulation. A (Arc), B (c-Fos), C (Zif268). For each time point, for each IEGP, the mean number of positive cells of the 6 sections with highest numbers of cells (N = 3 animals) was calculated, and the graphs show the means ± S.E.M. of these values. (‘NoNS’ - non-neuropathic stimulated animals; ‘NS’ – neuropathic stimulated; ‘NoNN’ – non-neuropathic non-stimulated; ‘N’ – neuropathic animals.) During statistical analyzes, the univariate general linear model was used and significance accepted at the 1% level (**p < 0.01). The control bars consist of one control bar for NoNN (2 h and 6 h post sham operation) and one for N animals.

The statistical results (Fig. 2A-C) were represented with bar graphs, where the height of graphs was calculated as mean values ±S.E.M. (N = 18 sections, the six sections with the highest numbers of positive cells per animal SC (three animals in each group)).

2.6 Inclusion criteria

We used modified criteria for inclusion of animals, previously defined by Smits et al. [20]. The criteria were modified so that animals with a pre-nerve lesion baseline of repeated von Frey withdrawal thresholds below 10 g should not be included. The withdrawal threshold exclusion point was decreased from 60 g to 10g due to a significant percentage of animals that responded to von-Frey fibres calibrated to 10g pressure. In addition, it was decided that animals without any decrease in von Frey withdrawal threshold below pre-ligation threshold should be defined as non-responders (N = 0) to the stimulation protocol and therefore should be excluded from the analysis. In our study, all animals were included as the inclusion criteria were met in all subjects.

3 Results

3.1 Response thresholds were markedly decreased after loose ligation of the sciatic nerve

As previously described, animals were divided into groups, consisting of 12 sham operated animals and 12 animals with sciatic loose ligation. Before sham operation the withdrawal thresholds (Fig. 1A) were 12.021 ±0.391 g (mean ± standard error of mean, S.E.M.). At day 7 post sham operation, the mean withdrawal thresholds did not change significantly (t-test p>0.05; N = 12; unpaired Student’s t-tests) and stayed approximately the same, as expected. Hence, sham operated rats are referred to as non-neuropathic rats.

Prior to ligation withdrawal thresholds (Fig. 1B) were 13.47 ± 0.455 g (mean ± standard error of mean, S.E.M.). At day 7 post nerve ligation, the mean withdrawal thresholds decreased significantly (t-test **p < 0.0001; N = 12; unpaired Student’s t-tests) to 2.95 ± 0.306 g.

3.2 Neuropathy increases stimulus-induces expression of Arc, Zifl68 and c-Fos in the dorsal horn

According to the allodynia classification proposed by Smits et al. [20], all animals in our study that were subjected to sciatic loose ligation showed moderate allodynia (withdrawal threshold <6.0 g) 7 days after surgery. Neuropathy significantly increased the number of IEGP positive cells at both 2 h and 6 h post CS. Both neuropathic and sham operated animals showed a higher number of positive cells 2 h after CS than after 6 h (Fig. 2A-C).

Statistical analysis (univariate general linear model) was performed comparing the 2 and 6 h post-stimulation groups with the control (sham-operated) groups. Stimulation vs. non-stimulation, neuropathy vs. non-neuropathy and time point were used as independent variables while the number of IEGP positive cells was used as the dependent variable (Fig. 2A-C).

Bennett’s procedure led to a maximal IEGP expression 2 h after CS in neuropathic animals. The increase in the number of IEGP positive cells compared to non-neuropathic stimulated animals was 83.0% for Arc, 42.4% for c-Fos and 37.2% for Zif268 (Fig. 2A-C). After 6 h the increase compared to non-neuropathic animals was 80.4% for Arc, 52.2% for c-Fos and 48.3% for Zif268 (Fig. 2A-C).

The unstimulated side of the dorsal horn in stimulated animals did not show any significant change of the number of IEGP positive cells and was approximately at the same level as sham operated animals. The control (non-neuropathic and non-stimulated animals, no stimulation) values in non-neuropathic and neuropathic groups separately showed same immunoreactivity in 2 and 6 h post sham operation and therefore were considered with their data combined as one group (separately for non-neuropathic and neuropathic animals) (Fig. 3).

(A-E) DAB staining photomicrographs of dorsal spinal cord 2 h post stimulation and photomicrograph of staining controls. Photomicrographs of a transverse sectioned SC, immunohistochemical DAB staining of cells expressing Arc (A), c-Fos (B) and Zif268 (C) in superficial SC dorsal horn laminar neurons (10×; 2h post-CS, 7d morphine treated animals). Arrows indicate positive cells. The number of positive cells is greatest indorsal horn ipsilateral to stimulation (marked with triangle). The contralateral side shows little or no expression of Arc (A), c-Fos (B) and Zif268 (C). Section D and E are controls of staining without the primary antibody with different secondary antibodies marked on pictures. Scale bars= 100μm.
Fig. 3

(A-E) DAB staining photomicrographs of dorsal spinal cord 2 h post stimulation and photomicrograph of staining controls. Photomicrographs of a transverse sectioned SC, immunohistochemical DAB staining of cells expressing Arc (A), c-Fos (B) and Zif268 (C) in superficial SC dorsal horn laminar neurons (10×; 2h post-CS, 7d morphine treated animals). Arrows indicate positive cells. The number of positive cells is greatest indorsal horn ipsilateral to stimulation (marked with triangle). The contralateral side shows little or no expression of Arc (A), c-Fos (B) and Zif268 (C). Section D and E are controls of staining without the primary antibody with different secondary antibodies marked on pictures. Scale bars= 100μm.

4 Discussion

In this study we have evaluated the difference of stimulus-induced immunoreactivity of Arc, c-Fos and Zif268 in the dorsal horn between neuropathic rats and sham-operated rats after sciatic nerve CS. We used a series of 100 Hz stimulation trains on primary afferent fibres of the sciatic nerve. Our focus of interest was the L3-L5 segment of lumbar spinal cord that probably receives the highest density of afferent nerve fibre input from the sciatic nerve [22,23] and shows the highest immunoreactivity of IEGPs as a response to CS. Sham-operated animals without CS were used as controls. We used the Bennett’s sciatic nerve loose ligation model as the most commonly used model of neuropathic pain. However Bennett’s nerve ligation involves a slight variability in the degree of damaged fibres leading to some variability in the number of responders and their behaviour [3]. Our SC sections showed a slight variability of positive cells between animals receiving same CS at same levels of the SC that could be explained by the previous fact mentioned.

The loose sciatic nerve ligation in Bennett’s model of neuropathy features a ‘co-mingling’ of axons and Schwann cells that become denervated distal to the ligation. Damaged Schwann cells could influence intact axons with a variety of neuroactive cytokines [24] and factors as tumour necrosis factor alpha (TNFa) contributing to the pain state. Properly conducted Bennett’s loose ligation results in neuropathic development that can be found the first day after ligation [25] and might last for many weeks after the procedure [26]. A recovery and decrease in neuropathy was reported 8-10 weeks after the ligation [27]. Since our experiments were conducted with a 7-day post operation time period, we cannot comment on the previous report. A variety of neurobiological mechanisms are responsible for the development of the neuropathic state. Some of the factors are collateral spreading of non-damaged fibres into denervated skin regions, increased excitability of damaged axons, leading to central sensitization. Loss of inhibitory mechanisms and inhibitory neurons in the spinal cord could also be responsible for neuropathy [3]. Electrophysiological studies in the spinal cord of neuropathic rats led to a finding that C-fibre evoked responses increased while the threshold for C-fibre activation decreased compared to naïve animals. Studies reported that more neurons were spontaneously active with an increased firing frequency in neuropathic rats. The previous implies that the spinal cord increased excitability in neuropathic rats, compensating for the decrease of peripheral input formed as a consequence of nerve ligation [28].

Development of peripheral neuropathy after loose sciatic nerve ligation is validated in a series of Von Frey fibre pain threshold tests. Similar to our experiments, Decosterd et al., reported a significant decrease of withdrawal threshold after ligation surgery and maintained a stable level afterwards [3,4]. Withdrawal thresholds to von Frey filament stimulation decreased significantly in our data 7 days after loose ligation, from 11.91 ± 0.746 g (mean±S.E.M.; before Bennett’s procedure) to 2.95 ± 0.306 g.

Similar to other studies mentioned later in the discussion, we found a difference in IEGP expression after CS between neuropathic and naïve rats. The stimulated SC side showed the significant increase in IEGP expression in both 2 h and 6 h post CS compared to controls. The control sides and sham operated control animals did not show significant IEGP expression change due to CS. Interestingly, Lee et al. [19] reported an elevation in IEGP expression on the contralateral, unstimulated side of the SC. Our sections contained IEGP positive cells in lamina I and II of the lumbar spinal cord as previously shown in other studies [7]. However, in contrary to Lee et al. [19] and Williams et al. [29], we did not manage to confirm increased IEGP expression in deeper laminas of the SC. Previous studies reported elevation of the number of c-Fos positive cells was found predominantly in the lamina I and II of the dorsal horn [19,27] while Zif268 was reported to be increased in all the laminas I–IV [2]. Experimental work from Hossaini et al. from 2010 showed that Arc protein was elevated in neuropathic rats at 2 h post ligation [30]. Moreover, stimulation of afferent fibres was shown to lead to enhanced expression of c-Fos mRNA in spinal cord neurons and synaptic Arc protein [12,13].

Strikingly, our study showed an increase in the number of Arc positive cells in neuropathic, non-stimulated rats, observed 7 days after ligation. The expression of c-Fos and Zif268 was not altered significantly in neuropathic rats prior to CS. The influence of neuropathy was reported previously to induce increased immunoreactivity of IEGP positive cells in the dorsal horn [19,29] without CS. Moreover, Arc protein was defined as an important factor for consolidation of memory and it is necessary for the late phase LTP in the hippocampus [10,31]. Arc enables expansion of the cytoskeletal network, which underlies stable morphological changes in dendritic spines during in vivo LTP [10,32,33]. In the SC, Arc dependent long-term synaptic changes in spinal transmission were defined as a feature of anti-nociceptive neurons [30]. Hossaini et al. reported the presence of increased immunoreactivity in Arc protein predominantly located in lamina II of the spinal dorsal horn. He reported elevated Arc expression 2 h after nerve ligature. However, contrary to our results, Arc expression was reported as diminished one and two weeks after the ligature in non-stimulated animals which simultaneously had developed thermal hyperalgesia and allodynia [30]. The elevation of Arc after loose sciatic nerve ligation can be a sign that Arc might have a role in neuropathic pain development. Studies have yet not determined the effects of selective Arc inhibition on neuropathic pain development. Others have found that Arc/Arg3.1 mRNA was only increased 2 h after ligation but not 1 week nor 2 weeks after the operation when the neuropathic pain symptoms, i.e. mechanical and thermal hyperalgesia and allodynia, had developed [30]. Moreover, in the spinal cord, the central projections of nociceptors synapse with second order neurons. These neurons may enter a state of elevated responsiveness [30] after nociceptive stimulation due a responsible mechanism similar to the mechanism of LTP development in the hippocampus [34]. Arc IEGP plays a role in the processes of LTP establishment, long term depression (LTD), homeostatic scaling of AMPA receptors [31], spinal processing [35] and may ‘underlie chronic pain disorders’ [30]. Moreover, immunohistochemical studies revealed that about 10% of Arc positive cells in the spinal cord expressed PKC-γ receptors. PKC-γ receptors have an important role in the formation of chronic pain [36].

C-fos is known as a neuronal activity marker [5] and found to be increased after spinal [37] and peripheral CS [29] in neuropathic rat models. Similarly, with immunohistochemical staining we found a significant increase of the number of c-Fos positive cells in neuropathic animals compared to non-neuropathic sham operated animals after CS. Here we reported a significant c-Fos expression increase 7 days after loose ligation in animal subjects 2 and 6 h after CS. However, other studies reported that higher expression of c-Fos could be found 3 weeks after the neuropathic intervention. Interestingly, c-Fos was reported to have a bi-phasic expression elevation in deep dorsal SC layers, 2h and 24 h after loose ligation [38] and that contralateral expression can be found 8 h to 24 h after ligation. Williams et al. reported c-Fos expression elevation in superficial layers 2 h after ligation that was reported normalized 24 h after the ligation [29]. Further on, the expression of c-Fos was reported to be blocked in deep but not superficial layers after morphine and MK-801 (antagonist of NMDA receptors) block. Conditioning stimulation of afferent C-fibres results in the formation of fast synaptic potentials by activation of NMDA receptors, AMPA receptors and kainic acid (KA) [39]. Activation of NMDA and voltage gated Ca2+ channels results in Ca2+ influx activating many protein kinases and nitrous oxide (NO) activating the expression of IEG c-Fos [40]. FOS protein, the product of c-Fos gene activation, together with JUN (protein product of c-Jun gene) inhibits c-Fos transcription [41,42].

FOS and JUN are part of the AP1 (activation protein-1 transcription factor) heterodimer, that binds to a DNA site located in genes coding for preprodynorphin, among many other genes [43]. The product of predynorphin is dynorphin that as an endogenous opioid binds to kappa opioid receptors [44] located on neurons synapsing with local excitatory circuit neurons [45]. Furthermore, studies have shown that dynorphin injected intrathecally produces prolonged allodynia [46,47]. NMDA antagonists have the characteristic of preventing allodynia. It has therefore been concluded that dynorphin and its activity on NMDA receptors, represents one of the main factors of allodynia establishment [48]. Therefore, the previous suggests that dynorphin might be responsible for chronic allodynia and hyperalgesia development [49]. Since c-Fos was found to be expressed in the same areas of the superficial layers of spinal cord after CS asZif268, it was suggested that those two IEGP together might have a role in ‘converting extracellular events such as noxious stimulation into long-term intracellular changes’ [50,51]. However, the detailed role of c-Fos in pain regulation has to be further investigated [52].

Zif268 (aka Egr1) is a zink finger transcription factor, a functional marker of neuroplasticity [53], that becomes expressed after noxious stimulation. Studies showed that LTP formation [54] and the development of persistent pain states [55] in the spinal cord as well and memory consolidation [56] investigated in the hippocampus are dependent on Zif268 IEGP expression. Further on, Zif268 has a function as a functional marker of neuroplasticity [53]. The formation of Zif268 can be decreased or stopped by the application of NMDA antagonists. Therefore it has been suggested that NMDA receptors might be responsible for the up-regulation of Zif268 after tissue injury [57]. To conclude, it has therefore been proposed that Zif268 ‘may contribute to signalling pathways involved in synaptic potentiation’ [58].

Zif268 was shown to have an important role in LTP maintenance [59] and it is induced in neurons in response to conditioning stimulation [60]. Similarly to our findings, the results of Ruiz-Torner et al. [61] showed that CS induces an increase of immunoreactivity of Zif268, described as a characteristic of neuronal activation. This increase was found in the superficial laminae, defined as the location of primary terminal nerve endings of A-delta and C noxious fibres [61]. Strikingly, Vadakkan et al. [62] reported bilateral SC dorsal horn Zif268 expression and proposed supraspinal structures of the nervous system as possible mechanisms of this change. Opposite to Vadakkan et al., we found only ipsilateral Zif268 immunoreactivity increase similar to Williams et al. and Lee et al. [19,29]. Moreover, Ko et al. suggested that Zif268 plays a selective role in nociceptive behavioural responses to persistent inflammatory pain but not to acute noxious stimuli [58]. Our results showed a similar trend of Zif268 expression as for Arc and c-Fos. Contrary to the expression of Arc, Zif268 did not show elevated expression after neuropathic pain prior to CS.

All IEGPs showed a significant increase in expression 6 h post-CS. Our results showed a higher increase in expression (compared to controls) at 6h than at 2h post-CS while at the same time the expression levels were higher at the 2 h post-CS time point. Unfortunately, we cannot propose a reason for this specific expression pattern that followed all studied IEGPs. As previously mentioned for Arc and c-Fos, before studies include selective IEGP knock-out animals and determine the dependence of neuropathy on specific IEGPs we can argue for that the previous mentioned IEGPs have a potential role in neuropathic formation. However, the specific function has not been yet described.

To conclude, the results of this study showed that conditioning stimulation led to an increased expression of all studied IEGPs. Hence the fact that all studied IEGPs showed significant increase after induction of neuropathic pain, we might suggest a potential cooperative or individual role of Arc, c-Fos and Zif268 in the establishment and/or sustainability of neuropathic pain in rats.

The process of chronic pain development is a complex neu-robiological phenomenon. This study adds to the knowledge of the mechanisms of neuropathic pain and improves the basis for further studies of neuropathic pain development and treatment. This study however only involves animal research and neuropathic pain as a consequence of sciatic nerve ligation. The findings of this experiment are similar to neurobiological alterations formed as a consequence of nerve compression during carpal tunnel syndrome or spinal root compression due to a vertebral disc prolapse but have clear limitations since it was conducted on animals. Future investigations should focus on revealing details of IEGP functions, potentially by selective knock out of specific IEGPs.


  • We studied the immunoreactivity of Arc, c-Fos and Zif268 after nerve ligation.

  • Expression of Arc, Zif and Fos was not elevated in neuropathic animals before stimulation.

  • Stimulus-induced immunoreactivity was clearly increased in neuropathy.

  • Contralateral dorsal horn showed unchanged immunoreactivity after neuropathic treatment.

  • The studied IEGP’s may have a role in sensitization in neuropathic conditions.


This work was supported by grants from the University of Bergen. The authors thank Torhild F. Sunde for her technical support and advice. No conflict of interest declared.


  • [1]

    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. PubMedCrossrefGoogle Scholar

  • [2]

    Toniolo EF, Maique ET, Ferreira Jr WA, Heimann AS, Ferro ES, Ramos-Ortolaza DL, Miller L, Devi LA, Dale CS. Hemopressin, an inverse agonist of cannabinoid receptors, inhibits neuropathic pain in rats. Peptides 2014;56:125–31. PubMedCrossrefGoogle Scholar

  • [3]

    Decosterd I, Woolf CJ. Spared nerve injury: an animal model of persistent peripheral neuropathic pain. Pain 2000;87:149–58. CrossrefPubMedGoogle Scholar

  • [4]

    Dowdall T, Robinson I, Meert TF. Comparison of five different rat models of peripheral nerve injury. Pharmacol Biochem Behav 2005;80:93–108. CrossrefPubMedGoogle Scholar

  • [5]

    Kayser V, Viguier F, Ioannidi M, Bernard JF, Latremoliere A, Michot B, Vela JM, Buschmann H, Hamon M, Bourgoin S. Differential anti-neuropathic pain effects of tetrodotoxin in sciatic nerve-versus infraorbital nerve-ligated rats - behavioral, pharmacological and immunohistochemical investigations. Neu-ropharmacology 2010;58:474–87. Google Scholar

  • [6]

    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. CrossrefPubMedGoogle Scholar

  • [7]

    Haugan F, Wibrand K, Fiska A, Bramham CR, Tjolsen A. Stability of long term facilitation and expression of zif268 and Arc in the spinal cord dorsal horn is modulated by conditioning stimulation within the physiological frequency range of primary afferent fibers. Neuroscience 2008;154:1568–75. PubMedCrossrefGoogle Scholar

  • [8]

    Abraham WC, Williams JM. LTP maintenance and its protein synthesis-dependence. Neurobiol Learn Mem 2008;89:260–8. CrossrefPubMedGoogle Scholar

  • [9]

    Bramham CR, Messaoudi E. BDNF function in adult synaptic plasticity: the synaptic consolidation hypothesis. Prog Neurobiol 2005;76:99–125. PubMedCrossrefGoogle Scholar

  • [10]

    Messaoudi E, Kanhema T, Soule J, Tiron A, Dagyte G, da Silva B, Bramham CR. Sustained Arc/Arg3.1 synthesis controls long-term potentiation consolidation through regulation of local actin polymerization in the dentate gyrus in vivo. J Neurosci 2007;27:10445–55. CrossrefPubMedGoogle Scholar

  • [11]

    Sandkühler J. Long-term potentiation and long-term depression in the spinal cord; 2007. p. 1058–60. Google Scholar

  • [12]

    Liu YP, Liu S. Electrical nerve stimulation and the relief of chronic pain through regulation of the accumulation of synaptic Arc protein. Med Hypotheses 2013;81:192–4. CrossrefPubMedGoogle Scholar

  • [13]

    Wisden W, Errington ML, Williams S, Dunnett SB, Waters C, Hitchcock D, Evan G, Bliss TV, Hunt SP. Differential expression of immediate early genes in the hippocampus and spinal cord. Neuron 1990;4:603–14. PubMedCrossrefGoogle Scholar

  • [14]

    Rexed B. The cytoarchitectonic organization of the spinal cord in the cat. J Comp Neurol 1952;96:414–95. Google Scholar

  • [15]

    Hughes DI, Boyle KA, Kinnon CM, Bilsland C, Quayle JA, Callister RJ, Graham BA. HCN4 subunit expression in fast-spiking interneurons of the rat spinal cord and hippocampus. Neuroscience 2013;237:7–18. CrossrefPubMedGoogle Scholar

  • [16]

    Molander C, Xu Q, Grant G. The cytoarchitectonic organization of the spinal cord in the rat. I. The lower thoracic and lumbosacral cord. J Comp Neurol 1984;230:133–41. Google Scholar

  • [17]

    Coghill RC, Mayer DJ, Price DD. Wide dynamic range but not nociceptive-specific neurons encode multidimensional features of prolonged repetitive heat pain. J Neurophysiol 1993;69:703–16. CrossrefPubMedGoogle Scholar

  • [18]

    Yamazaki Y, Maeda T, Someya G, Wakisaka S. Temporal and spatial distribution of Fos protein in the lumbar spinal dorsal horn neurons in the rat with chronic constriction injury to the sciatic nerve. Brain Res 2001;914:106–14. PubMedCrossrefGoogle Scholar

  • [19]

    Lee WT, Sohn MK, Park SH, Ahn SK, Lee JE, Park KA. Studies on the changes of c-fos protein in spinal cord and neurotransmitter in dorsal root ganglion of the rat with an experimental peripheral neuropathy. Yonsei MedJ 2001;42:30–40. CrossrefGoogle Scholar

  • [20]

    Smits H, Ultenius C, Deumens R, Koopmans GC, Honig WM, van Kleef M, Linderoth B, Joosten EA. Effect of spinal cord stimulation in an animal model of neuropathic pain relates to degree of tactile allodynia. Neuroscience 2006;143:541–6. CrossrefGoogle Scholar

  • [21]

    Liu X, Sandkuhler J. Characterization of long-term potentiation of C-fiber-evoked potentials in spinal dorsal horn of adult rat: essential role of NK1 and NK2 receptors. J Neurophysiol 1997;78:1973–82. PubMedCrossrefGoogle Scholar

  • [22]

    Waibl H. Advances in anatomy embryology and cell biology, vol. 47 - Fasc. 6. Germany: Springer; 1973. Google Scholar

  • [23]

    Mentis GZ, Alvarez FJ, Bonnot A, Richards DS, Gonzalez-Forero D, Zerda R, O’Donovan MJ. Noncholinergic excitatory actions of motoneurons in the neonatal mammalian spinal cord. Proc Natl Acad Sci U S A 2005;102: 7344–9. CrossrefPubMedGoogle Scholar

  • [24]

    Sorkin LS, Xiao WH, Wagner R, Myers RR. Tumour necrosis factor-alpha induces ectopic activity in nociceptive primary afferent fibres. Neuroscience 1997;81:255–62. PubMedCrossrefGoogle Scholar

  • [25]

    Kajander KC, Madsen AM, Iadarola MJ, Draisci G, Wakisaka S. Fos-like immunoreactivity increases in the lumbar spinal cord following a chronic constriction injury tothe sciatic nerve of rat. Neurosci Lett 1996;206:9–12. CrossrefGoogle Scholar

  • [26]

    Kim SH, Chung JM. An experimental model for peripheral neuropathy produced by segmental spinal nerve ligation in the rat. Pain 1992;50:355–63. CrossrefPubMedGoogle Scholar

  • [27]

    Catheline G, Le Guen S, Honore P, Besson JM. Are there long-term changes in the basal or evoked Fos expression in the dorsal horn of the spinal cord of the mononeuropathic rat? Pain 1999;80:347–57. CrossrefPubMedGoogle Scholar

  • [28]

    Rygh LJ, Kontinen VK, Suzuki R, Dickenson AH. Different increase in C-fibre evoked responses after nociceptive conditioning stimulation in sham-operated and neuropathic rats. Neurosci Lett 2000;288:99–102. PubMedCrossrefGoogle Scholar

  • [29]

    Williams S, Evan G, Hunt SP. Spinal c-fos induction by sensory stimulation in neonatal rats. Neurosci Lett 1990;109:309–14. CrossrefPubMedGoogle Scholar

  • [30]

    Hossaini M, Jongen JL, Biesheuvel K, Kuhl D, Holstege JC. Nociceptive stimulation induces expression of Arc/Arg3.1 in the spinal cord with a preference for neurons containing enkephalin. Mol Pain 2010;6:43. PubMedGoogle Scholar

  • [31]

    Plath N, Ohana O, Dammermann B, Errington ML, Schmitz D, Gross C, Mao X, Engelsberg A, Mahlke C, Welzl H, Kobalz U, Stawrakakis A, Fernandez E, Waltereit R, Bick-Sander A, Therstappen E, Cooke SF, Blanquet V, Wurst W, Salmen B, Bosl MR, Lipp HP, Grant SG, Bliss TV, Wolfer DP, Kuhl D. Arc/Arg3.1 is essential for the consolidation of synaptic plasticity and memories. Neuron 2006;52:437–44. CrossrefPubMedGoogle Scholar

  • [32]

    Fukazawa Y, Saitoh Y, Ozawa F, Ohta Y, Mizuno K, Inokuchi K. HippocampalLTP is accompanied by enhanced F-actin content within the dendritic spine that is essential for late LTP maintenance in vivo. Neuron 2003;38:447–60. PubMedCrossrefGoogle Scholar

  • [33]

    Matsuzaki M, Honkura N, Ellis-Davies GC, Kasai H. Structural basis of long-term potentiation in single dendritic spines. Nature 2004;429:761–6. CrossrefPubMedGoogle Scholar

  • [34]

    Kullmann DM, Lamsa KP. Long-term synaptic plasticity in hippocampal interneurons. Nat Rev Neurosci 2007;8:687–99. CrossrefPubMedGoogle Scholar

  • [35]

    Rygh LJ, Svendsen F, Fiska A, Haugan F, Hole K, Tjolsen A. Long-term potentiation in spinal nociceptive systems – how acute pain may become chronic. Psychoneuroendocrinology 2005;30:959–64. CrossrefPubMedGoogle Scholar

  • [36]

    Malmberg AB, Chen C, Tonegawa S, Basbaum AI. Preserved acute pain and reduced neuropathic pain in mice lacking PKCgamma. Science 1997;278:279–83. PubMedCrossrefGoogle Scholar

  • [37]

    Smits H, Kleef MV, Honig W, Gerver J, Gobrecht P, Joosten EA. Spinal cord stimulation induces c-Fos expression in the dorsal horn in rats with neuropathic pain after partial sciatic nerve injury. Neurosci Lett 2009;450:70–3. CrossrefPubMedGoogle Scholar

  • [38]

    Lee YW, Park KA, Lee WT. Effects of MK-801 and morphine on spinal C-Fos expression during the development of neuropathic pain. Yonsei Med J 2002;43:370–6. CrossrefPubMedGoogle Scholar

  • [39]

    Smullin DH, Skilling SR, Larson AA. Interactions between substance P: calcitonin gene-relatedpeptide, taurine and excitatory amino acids in the spinal cord. Pain 1990;42:93–101. CrossrefPubMedGoogle Scholar

  • [40]

    Meller ST, Gebhart GF. Nitric oxide (NO) and nociceptive processing in the spinal cord. Pain 1993;52:127–36. PubMedCrossrefGoogle Scholar

  • [41]

    Halazonetis TD, Georgopoulos K, Greenberg ME, Leder P. c-Jun dimerizes with itself and with c-Fos, forming complexes of different DNA binding affinities. Cell 1988;55:917–24. PubMedCrossrefGoogle Scholar

  • [42]

    Kubik S, Miyashita T, Guzowski JF. Using immediate-early genes to map hippocampal subregional functions. Learn Mem 2007;14:758–70. CrossrefPubMedGoogle Scholar

  • [43]

    Munglani R, Hunt SP. Molecular biology of pain. Br J Anaesth 1995;75:186–92. PubMedCrossrefGoogle Scholar

  • [44]

    Corvello CM, Metz R, Bravo R, Armelin MC. Expression and characterization of mouse cFos protein using the baculovirus expression system: ability to form functional AP1 complex with coexpressed cJun protein. Cell Mol Biol Res 1995;41:527–35. Google Scholar

  • [45]

    Dubner R, Ruda MA. Activity-dependent neuronal plasticity following tissue injury and inflammation. Trends Neurosci 1992;15:96–103. CrossrefPubMedGoogle Scholar

  • [46]

    Vanderah TW, Laughlin T, Lashbrook JM, Nichols ML, Wilcox GL, Ossipov MH, Malan Jr TP, Porreca F. Single intrathecal injections of dynorphin A or des-Tyr-dynorphins produce long-lasting allodynia in rats: blockade by MK-801 but not naloxone. Pain 1996;68:275–81. PubMedCrossrefGoogle Scholar

  • [47]

    Laughlin TM, Vanderah TW, Lashbrook J, Nichols ML, Ossipov M, Porreca F, Wilcox GL. Spinally administered dynorphin A produces long-lasting allodynia: involvement of NMDA but not opioid receptors. Pain 1997;72:253–60. CrossrefPubMedGoogle Scholar

  • [48]

    Ahmad AH, Ismail Z. c-fos and its consequences in pain. Malays J Med Sci 2002;9:3–8. PubMedGoogle Scholar

  • [49]

    Caudle RM, Mannes AJ. Dynorphin: friend or foe? Pain 2000;87:235–9. PubMedCrossrefGoogle Scholar

  • [50]

    Otahara N, Ikeda T, Sakoda S, Shiba R, Nishimori T. Involvement of NMDA receptors in Zif/268 expression in the trigeminal nucleus caudalis following formal in injection into the rat whisker pad. Brain Res Bull 2003;62:63–70. CrossrefGoogle Scholar

  • [51]

    Morgan JI, Curran T. Stimulus-transcription coupling in the nervous system: involvement of the inducible proto-oncogenes fos and jun. Annu Rev Neurosci 1991;14:421–51. CrossrefPubMedGoogle Scholar

  • [52]

    Gao YJ, Ji RR. c-Fos and p ERK, which is a better marker for neuronal activation and central sensitization after noxious stimulation and tissue injury? Open Pain J 2009;2:11–7. CrossrefGoogle Scholar

  • [53]

    Densmore VS, Kalous A, Keast JR, Osborne PB. Above-level mechanical hyper-algesia in rats develops after incomplete spinal cord injury but not after cord transection: and is reversed by amitriptyline, morphine and gabapentin. Pain 2010;151:184–93. CrossrefGoogle Scholar

  • [54]

    Rygh LJ, Suzuki R, Rahman W, Wong Y, Vonsy JL, Sandhu H, Webber M, Hunt S, Dickenson AH. Local and descending circuits regulate long-term potentiation and zif268 expression in spinal neurons. Eur J Neurosci 2006;24:761–72. CrossrefGoogle Scholar

  • [55]

    Liang F, Jones EG. Developmental and stimulus-specific expression of the immediate-early gene zif268 in rat spinal cord. Brain Res 1996;729:246–52. PubMedGoogle Scholar

  • [56]

    Sarantis K, Antoniou K, Matsokis N, Angelatou F. Exposure to novel environment is characterized by an interaction of D1/NMDA receptors underlined by phosphorylation of the NMDA and AMPA receptor subunits and activation of ERK1/2 signaling: leading to epigenetic changes and gene expression in rat hippocampus. Neurochem Int 2012;60:55–67. PubMedGoogle Scholar

  • [57]

    Wang JQ, Daunais JB, McGinty JF. NMDA receptors mediate amphetamine-induced upregulation of zif/268 and preprodynorphin mRNA expression in rat striatum. Synapse 1994;18:343–53. PubMedCrossrefGoogle Scholar

  • [58]

    Ko SW, Vadakkan KI, Ao H, Gallitano-Mendel A, Wei F, Milbrandt J, Zhuo M. Selective contribution of Egr1 (zif/268) to persistent inflammatory pain. J Pain 2005;6:12–20. CrossrefPubMedGoogle Scholar

  • [59]

    Jones MW, Errington ML, French PJ, Fine A, Bliss TV, Garel S, Charnay P, Bozon B, Laroche S, Davis S. A requirement for the immediate early gene Zif268 in the expression of late LTP and long-term memories. Nat Neurosci 2001;4: 289–96. CrossrefPubMedGoogle Scholar

  • [60]

    Knapska E, Kaczmarek L. A gene for neuronal plasticity in the mammalian brain:Zif268/Egr-1/NGFI-A/Krox-24/TIS8/ZENK? Prog Neurobiol 2004;74:183–211. CrossrefPubMedGoogle Scholar

  • [61]

    Ruiz-Torner A, Olucha-Bordonau F, Valverde-Navarro AA, Martinez-Soriano F. The chemical architecture of the rat’s periaqueductal gray based on acetyl-cholinesterase histochemistry: a quantitative and qualitative study. J Chem Neuroanat 2001;21:295–312. CrossrefGoogle Scholar

  • [62]

    Vadakkan KI, Jia YH, Zhuo M. A behavioral model of neuropathic pain induced by ligation of the common peroneal nerve in mice. J Pain 2005;6:747–56. CrossrefPubMedGoogle Scholar



nociceptive specific neurons


wide dynamic range neurons



About the article

Tel.: +47 46356421; fax: +47 55586360.

Received: 2015-06-17

Revised: 2015-09-05

Accepted: 2015-09-08

Published Online: 2016-01-01

Published in Print: 2016-01-01

Conflict of interest: The authors have no affiliations with or involvement in any organization or entity with any financial interest (such as honoraria; educational grants; participation in speakers’ bureaus; membership, employment, consultancies, stock ownership, or other equity interest; and expert testimony or patent-licensing arrangements), or non-financial interest (such as personal or professional relationships, affiliations, knowledge or beliefs) in the subject matter or materials discussed in this manuscript.

Citation Information: Scandinavian Journal of Pain, Volume 10, Issue 1, Pages 43–51, ISSN (Online) 1877-8879, ISSN (Print) 1877-8860, DOI: https://doi.org/10.1016/j.sjpain.2015.09.002.

Export Citation

© 2015 Scandinavian Association for the Study of Pain. This work is licensed under the Creative Commons Attribution-NonCommercial-NoDerivatives 4.0 License. BY-NC-ND 4.0

Comments (0)

Please log in or register to comment.
Log in