On the possible role of ERK, p38 and CaMKII in the regulation of CGRP expression in morphine-tolerant rats
© Wang et al; licensee BioMed Central Ltd. 2011
Received: 1 April 2011
Accepted: 21 September 2011
Published: 21 September 2011
The neuropeptide, calcitonin gene-related peptide (CGRP) has been proposed to be a regulator of the development of morphine analgesic tolerance and thereby could be a target to reduce the induction of this phenomenon under clinical conditions. However, the mechanisms of CGRP regulation are unclear. We investigated here the possible role of the extracellular signal-regulated protein kinase (ERK), p38 and calcium/calmodulin-dependent protein kinase II (CaMKII) in CGRP regulation following chronic morphine treatment.
A 7-day treatment with morphine (15 μg/day) led to an increase in CGRP contents in the spinal cord dorsal horn (SCDH) and dorsal root ganglion (DRG) and this effect was prevented by the inhibition of the ERK, p38 or CaMKII pathway. The phosphorylation/activation of ERK, p38 and CaMKII was enhanced in the SCDH following chronic morphine while in DRG only the phosphorylation of CaMKII was increased. Moreover, our chronic morphine treatment up-regulated neuronal nitric oxide synthase (nNOS) levels in the SCDH, an effect blocked by the inhibition of the ERK, p38 or CaMKII pathway. The blockade of nNOS activity also suppressed chronic morphine-induced CGRP increases in the DRG and SCDH. Double immunofluorescence studies revealed that nNOS and CaMKII are co-localized in the SCDH and that CaMKII is activated in CGRP-expressing DRG neurons.
The activation of spinal ERK, p38 and CaMKII, alongside nNOS, is involved in chronic morphine-induced CGRP up-regulation in both the DRG and SCDH. Moreover, the stimulation of CaMKII in the DRG likely directly regulates the expression of CGRP associated with morphine analgesic tolerance.
KeywordsCGRP ERK p38 CaMKII morphine
Opiates such as morphine are the most commonly used drugs in the clinical management of moderate to severe pain, including cancer pain. However, their clinical usefulness is largely hindered by the development of analgesic tolerance, which often requires escalating doses to achieve equivalent pain relief . The mechanisms underlying this phenomenon have been extensively investigated and several hypotheses have been proposed, including the altered activity of excitatory substances and their intracellular signaling pathways, the desensitization of mu-opioid receptor and its possible linkage with arrestin as well as interaction between mu- and delta-opioid receptors . In accordance with these data, a neuropeptide, calcitonin gene-related peptide (CGRP), has been suggested to play a major role in the development of tolerance to morphine-induced analgesia [3–7] and thus could be a promising target to reduce the occurrence of tolerance. Indeed, chronic morphine treatment results in an increase in CGRP expression and/or release in the spinal cord [3, 5, 6, 8, 9]. Moreover, treatment with a CGRP receptor antagonist was shown to prevent the development of tolerance to morphine-induced analgesia [3, 4]. Furthermore, the role of CGRP in morphine tolerance may be attributable to its differential regulation of cell-type specific kinase-transcription factor cascades [5, 6]. Accordingly, it is of interest to investigate how the expression of CGRP is regulated following chronic morphine treatment.
CGRP, a 37-amino acid neuropeptide is broadly distributed in the peripheral and central nervous systems, including the dorsal root ganglion (DRG) and its nerve terminals, which are the predominant source of CGRP in the spinal cord dorsal horn (SCDH) . Mounting evidence has suggested that various factors influence CGRP expression under certain conditions. For example, CGRP levels can be increased in vivo or in vitro by growth factors such as nerve growth factor (NGF) or the cytokine activin A in sensory neurons [11–16]. In particular, peripheral stimulation such as inflammation can induce an increase in CGRP mRNA levels in the DRG, possibly through the synergistic effect of NGF and activin A . Our previous results have also shown that chronic morphine-induced increases in CGRP levels may result from the activation of ERK and the downstream cAMP response element-binding protein (CREB) in cultured DRG sensory neurons . In the present study, we investigated factors involved in the regulation of the expression of CGRP and associated with the development of tolerance to morphine-induced analgesia both at the level of the DRG and SCDH.
Possible role of ERK, p38 and CaMKII in the development of morphine antinociceptive tolerance
Involvement of ERK, p38 and CaMKII in CGRP regulation related to morphine antinociceptive tolerance
Possible role of nNOS in the regulation of CGRP by ERK, p38 and CaMKII during the development of morphine tolerance
In the present study, we investigated intracellular signaling molecule(s) involved in the regulation of CGRP known to participate in the development of tolerance to morphine's analgesia. Our data suggest a role of ERK, p38 and CaMKII, as shown by enhanced activation/phosphorylation of these kinases in the SCDH while their inhibitions prevented chronic morphine-induced CGRP increases as well as the development of tolerance to morphine-induced analgesia. The CGRP-related regulatory processes may involve retrograde signaling via the NO signal transduction system because the level of nNOS, a major NO-synthesizing enzyme, is increased in the SCDH following chronic morphine treatment and can be modulated by the inhibition of either ERK or p38 or CaMKII pathway. Moreover, the blockade of nNOS also inhibited chronic morphine-induced increases in CGRP level. The morphological data showed that CaMKII and nNOS are co-localized in neurons of the SCDH. In the DRG, increased CaMKII activation/phosphorylation was observed in CGRP-expressing neurons in morphine-tolerant animals. Taken together, chronic morphine-induced CGRP up-regulation in both the DRG and SCDH likely involves the activation of spinal ERK, p38 and CaMKII as signaling molecules, a process also requiring nNOS. Additionally, the activation of CaMKII in the DRG may directly influence the expression of CGRP required for the development of tolerance to morphine-induced analgesia.
The neuropeptide CGRP has been proposed to play an important role in spinal nociceptive processing [20, 21]. Once released, CGRP can act both pre- and post-synaptically on functional CLR/RAMP1 family 3 GPCR receptors , leading to the activation of various downstream signaling molecules including protein kinase A (PKA), PKC, CaMKII and MAP kinase involved in the multiple and complex pathophysiological effects induced by CGRP [22–24]. We have previously demonstrated a major role of CGRP and its receptors in the pathogenesis of morphine antinociceptive tolerance [3–6]. Specifically, blockade of CGRP receptors using peptide (CGRP8-37) as well as non-peptide (BIBN4096BS) CGRP receptor antagonists prevented the development of tolerance to morphine-induced analgesia as well as chronic morphine-induced CGRP up-regulation in the DRG and SCDH [3–6]. Several kinases including ERK, p38 and CaMKII have also been suggested to be involved in the development of tolerance to morphine-induced analgesia [5, 6, 25, 26] and their activation can be regulated by the blockade of CGRP receptor signaling [5, 6]. Therefore it was deemed to be of major interest to investigate the link between CGRP expression/regulation and kinase activities in the development of tolerance to morphine-induced analgesia. Accordingly, we examined the activity of the aforementioned kinases in both DRG and SCDH in tolerant animals. In agreement with earlier studies [5, 6, 25, 26], ERK, p38 and CaMKII showed increased levels in their phosphorylation/activation in the SCDH. We then used specific inhibitors to block each of the three kinase pathways. These various inhibitors blocked chronic morphine-induced CGRP increases in both DRG and SCDH. These data strongly suggest an existence of a key relationship between CGRP expression/regulation and these kinases in the development of tolerance to morphine-induced analgesia.
It is well established that CGRP is predominantly derived from nerve terminals of the DRG primary afferent fibers in the SCDH . Available data have also shown that activated/phosphorylated ERK and p38 kinases are expressed in glial cells in the SCDH [5–7, 26] while activated CaMKII is mostly present in neurons . Hence, how is it that messengers expressed in both neurons and glia can have similar effects on the modulation of CGRP observed in morphine tolerant animals? It is known that as a diffusible molecule, NO plays a crucial role in the development of morphine analgesic tolerance [27, 28]. Once released, NO can exert its effects either via the activation of the soluble guanylate cyclase (sGC)-cyclic GMP (cGMP) pathway [29, 30] or directly by modulating gene expression through its S-nitrosylation of target proteins . Therefore, we hypothesize that NO can act as an intermediate linking the activation of kinases to CGRP expression during the development of tolerance to morphine-induced analgesia. In support of this hypothesis, our data have demonstrated significant increases in nNOS levels in the SCDH in morphine-tolerant animals. These increases can be prevented by the inhibition of the ERK, p38 and CaMKII pathways. In addition, both CaMKII and nNOS are co-localized, suggesting the existence of a CaMKII-nNOS cascade regulating CGRP expression following chronic morphine treatment. As mentioned earlier, both ERK and p38 are mostly expressed in glial cells, suggesting an indirect effect by the modulation of these kinases. Interestingly, the inhibition of nNOS activity largely blocks chronic morphine-induced CGRP up-regulation in the DRG and SCDH, indicating that NO may act as a retrograde signaling molecule to regulate presynaptic CGRP expression levels. Taken together, these data suggest that chronic morphine-induced CGRP up-regulation involves the activation of a neuronal CaMKII-nNOS pathway, a process that can be regulated by the activation of ERK and p38 via a glial-neuronal cell interaction.
It should be noted that the western blot analyses did not reveal any increases in the phosphorylation of ERK and p38 in DRG extracts. In contrast, a chronic morphine treatment increased ERK phosphorylation in cultured DRG  as well as the phosphorylation of ERK and p38 in vivo . However, CaMKII showed a significant increase in its phosphorylation in the DRG, suggesting different molecular responsiveness of these kinases to morphine exposure and the development of tolerance. The different molecular responses could be attributable to the differential cell localization of kinases in the two regions, i.e. glia-localized in spinal cord and neuron-localized in DRG. In addition, activated CaMKII was found to be expressed in CGRP-enriched DRG neurons with the inhibition of CaMKII activity decreasing CGRP expression, suggesting that the chronic morphine-induced CGRP up-regulation may also involve the direct activation of CaMKII in DRG neurons.
All animal experiments were approved by the Animal Care and Use Committee of McGill University as well as Canadian Council on Animal Care and performed according to the guidelines of the International Association for the Study of Pain concerning the use of laboratory animals.
Operative procedures and drug delivery
Intrathecal catheterization was performed on male Sprague-Dawley rats weighing 230-250 g as previously described [5–7]. Specifically, under isoflurane anesthesia, a polyethylene (PE)-10 tubing was implanted into the subarachnoid space through the gap between the vertebrae L5 and L6 and extended to the caudal part of the lumbar enlargement. The remaining portion of the tubing was partly sutured to the neighboring musculature and exited through a small hole at the back of the neck. Animals were allowed to recover for 7-9 days before behavioral experiments and were acclimated to the testing environment. Drugs were injected through the exterior end of the tubing in a total volume of 10 μl followed by a flush of 15 μl of saline. Drug doses were chosen in accordance with previous studies [3, 5, 6, 26, 33]. The following drugs were purchased from Sigma-Aldrich (St. Louis, MO, USA): morphine sulfate (1.5 μg/μl in saline), 4-(4-fluorophenyl)-2-(4-methylsulfinylphenyl)-5-(4-pyridyl)1H-imidazole (SB203580; 1 μg/μl in 20% DMSO) and 2'-amino-3'-methoxyflavone (PD98059; 1 μg/μl in 20% DMSO) while 2-[N-(2-hydroxyethyl)]-N-(4-methoxybenzenesulfonyl)]amino-N-(4-chlorocinnamyl)-N-methylbenzylamine)phosphate (KN93; 1.5 mM in 20% DMSO), 7-Nitroindazole (7-NI; 2.5 μg/μl in 20% DMSO) and (4S)-N-(4-amino-5[aminoethyl]aminopentyl)-N'-nitroguanidine, TFA (NG; 7.5 μg/μl in 20% DMSO) were purchased from Calbiochem (San Diego, CA, USA).
The standard regimen of daily intrathecal injection of morphine (15 μg/day for 7 days) was used to induce analgesic tolerance to morphine as previously described [3, 5, 34]. Analgesic effects of morphine were evaluated by paw-withdrawal latency. Specifically, a radiant heat beam was focused on the plantar surface of the hindpaw . The thermal stimulation intensity was adjusted to produce a baseline latency of 10-12 sec and a cut-off time of 25 sec was used to prevent any potential tissue injury. Paw-withdrawal response latency was defined as the time from the onset of radiant heat to paw withdrawal and measured automatically by a digital meter. We conducted behavioral testing before and 30 min after drug injection on days 1 and 7. Data were standardized by conversion to percentage of maximal possible effect (%MPE) according to the following formula: [(response latency-baseline latency)/(cut-off time-baseline latency)]×100.
On day 8 ascending doses of morphine were acutely injected to animals previously receiving various chronic treatments through the intrathecal catheter every 30 min until a maximal analgesic effect was achieved in the tail-flick test, as previously reported [3, 6]. The cumulative dose-response curve of the antinociceptive effect of acute morphine was constructed accordingly. A non-linear regression analysis was used to determine the ED50 values while their statistical significance was computed using one-way ANOVA followed by a student-Newman-Keuls (SNK) post-hoc test for comparisons between groups. The standardized behavioral data were expressed as mean ± SEM and analyzed by two-way repeated ANOVA with a SNK post hoc test.
Animals were perfused via the ascending aorta with 300 ml of 4% paraformaldehyde following a flush of 100-150 ml saline. The lumbar spinal cords (L4 and 5) and corresponding DRGs were harvested, post-fixed in the same fixative for 4 h at 4°C and then transferred to 30% sucrose overnight for cryoprotection. DRG (16 μm) and transverse spinal cord sections (35 μm) were cut on a cryostat and collected for immunohistochemical studies.
Single labeling of CGRP
To remove endogenous peroxidase activity, floating spinal cord sections were treated with 0.03% H2O2 for 15 min. Next, to block any non-specific binding and enhance membrane permeability, sections were processed with 10% normal donkey serum and 0.03% TrionX-100 in 0.01 M PBS at room temperature (RT) for 30 min. Sections were incubated at 4°C with the primary guinea pig anti-CGRP antibody (1:3000, Peninsula Labs, San Carlos, CA, USA) for 48 hr. After rinsing in 0.01 M PBS, sections were incubated at RT in biotinylated donkey anti-guinea pig IgG for 1 h followed by reaction with avidin-biotin-peroxidase complex (ABC) for 30 min using Vectastain ABC kit (Vector, Burlingame, CA, USA). The immunoprecipitates were developed in 0.05% diaminobenzidine with 0.01% hydrogen peroxide and intensified by the addition of 0.02% nickel ammonium sulfate. In addition, CGRP fluorescent staining (1:500) was performed with the same primary antibody and visualized using Alexa488-conjugated donkey anti-guinea pig secondary antibody.
To reveal if CaM kinase II (CaMKII) can be activated in CGRP-expressing neurons, DRG sections were incubated with a mixture of rabbit anti-p-CaMKII (1:400) and guinea pig anti-CGRP (1:500). To identify the cell type(s) expressing nNOS or CaMKII, spinal sections were incubated with a mixture of rabbit anti-nNOS (or rabbit anti-CaMKII) and mouse anti-glial fibrillary acidic protein (GFAP, an astroglial marker, 1:1000, Millipore, Billerica, MA, USA), or mouse anti-OX-42 (a microglial marker, 1:100, AbD Serotech, Raleigh, NC, USA) or mouse anti-NeuN (a neuronal marker, 1:1000, Millipore) antibodies. Spinal sections were also incubated with a mixture of goat anti-nNOS and rabbit anti-CaMKII to determine if these two molecules are co-localized.
Animals were rapidly perfused through the ascending aorta with 100-150 ml of saline under anesthesia and the L4-L6 spinal cords and corresponding DRGs were collected on dry ice and stored at -80°C. Tissues were homogenized in modified RIPA buffer (50 mM Tris-HCl, 150 mM NaCl, 1 mM EDTA, 1% Igepal CA-630, 0.1% SDS, 50 mM NaF, and 1 mM NaVO3) containing a mixture of protein inhibitors (Sigma) including PMSF (2 mM), leupeptin (10 μg/ml) as well as aprotinin (10 μg/ml) and protein concentrations were determined by using a BCA protein assay kit (Pierce Biotechnology, Rockford, IL, USA). Equal amounts of protein samples (20 μg/lane) were loaded and separated on SDS-PAGE gels (4-20% tris-glycine gels, Invitrogen, Carlsbad, CA, USA; for CGRP, 18% tris-glycine gels were also included) and electroblotted onto Hybond-C nitrocellulose membranes (Amersham Biosciences, Piscataway, NJ, USA). The membranes were then processed for 1 h at RT with 5% skim milk to block non-specific binding sites and incubated overnight at 4°C with various indicated primary antibodies. After rinsing in 1xTBST, membranes were further incubated with HRP-conjugated secondary antibodies for 1 h at RT, developed in ECL solution for 1-5 min and exposed onto X-films for 1-5 min. Antibodies including p-ERK, p-p38 and p-CaMKII were purchased from Cell Signaling Technology and used at a dilution of 1:1000 while CGRP (1:1000) was obtained from Peninsula Labs and nNOS (1:800) from Santa Cruz Biotechnology. For loading controls, membranes were incubated with a stripping buffer and reprobed with antibodies against ERK, p38 and CaMKII at a dilution of 1:1000 (Cell Signaling Technology) as well as beta-actin at a dilution of 1:5000 (Santa Cruz Biotechnology). Specific bands were captured using a Sierra Scientific MS-4030 video camera (Sierra Scientific, Sunnyvale, CA, USA)and quantified by densitometric analysis using MCID version 6 Elite imaging software (Imaging Research, St. Catharines, ON, Canada). The density of each target band was normalized with its corresponding internal loading control bands. The fold change was defined as the ratio of the normalized data of the treatment group relative to its control group. Data are expressed as mean ± SEM. Statistical significance was analyzed using one-way or two-way ANOVA, wherever appropriate followed by a SNK post hoc test for comparisons between groups.
List of abbreviations used
calmodulin-dependent protein kinase II
calcitonin gene-related peptide
cAMP response element-binding protein
dorsal root ganglion
extracellular signal-regulated protein kinase
neuronal nitric oxide synthase
protein kinase A
spinal cord dorsal horn
soluble guanylate cyclase.
This study was supported by a grant from the Canadian Institutes of Health Research to R.Q. The authors appreciate the critiques and comments by Ms. Mira Thakur and thank Dr. Weiya Ma and Mr. Bruno St-Jacques for their technical support.
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