- Open Access
Bullatine A stimulates spinal microglial dynorphin A expression to produce anti-hypersensitivity in a variety of rat pain models
Journal of Neuroinflammation volume 13, Article number: 214 (2016)
Aconiti brachypodi Radix (Xue-shang-yi-zhi-hao) has been prescribed to manage chronic pain, arthritis, and traumatic injuries. Bullatine A, a C20-diterpenoid alkaloid, is one of its principle effective compounds. This study aimed to investigate the anti-hypersensitivity of bullatine A in a variety of rat pain models and explore its mechanisms of action.
Rat neuropathic pain, inflammatory pain, diabetic neuropathic pain, and bone cancer pain models were used. Dynorphin A and pro-inflammatory cytokines were measured in the spinal cord and cultured primary microglia. Double immunofluorescence staining of dynorphin A and glial and neuronal cellular markers was also measured in the spinal cord.
Subcutaneous and intrathecal injection of bullatine A dose-dependently attenuated spinal nerve ligation-, complete Freud’s adjuvant-, diabetes-, and bone cancer-induced mechanical allodynia and thermal hyperalgesia, with the efficacies of 45–70 % inhibition, and half-effective doses of 0.9–1.9 mg/kg for subcutaneous injection. However, bullatine A was not effective in blocking acute nociceptive response in the normal condition. Bullatine A specifically stimulated dynorphin A expression in microglia in the spinal cord in vivo and cultured primary microglia in vitro; the stimulatory effects were completely inhibited by the microglial inhibitor minocycline. In contrast, bullatine A did not have an inhibitory effect on peripheral nerve injury- or lipopolysaccharide-induced pro-inflammatory cytokine expression. The spinal anti-allodynic effects of bullatine A were entirely blocked by intrathecal injection of minocycline, the specific dynorphin A antiserum, and the selective k-opioid receptor antagonist.
We, for the first time, demonstrate that bullatine A specifically attenuates pain hypersensitivity, regardless of the pain models employed. The results also suggest that stimulation of spinal microglial dynorphin A expression mediates bullatine A anti-nociception in pain hypersensitivity conditions.
Aconiti brachypodi Radix (Xue-shang-yi-zhi-hao), the dried roots of Aconitum brachypodum Diels and several other morphologically similar species (genus Aconitum, family Ranunculaceae), is listed in the Chinese Pharmacopoeia for its analgesic and anti-rheumatic properties [1–3]. The bioactive extracts of A. brachypodi Radix, in the forms of pills, liniment, patch, and injection, are widely prescribed in China to manage chronic pain, arthritis, and traumatic injuries. As a principal group of compounds present in Aconitum, approximately 170 alkaloids have been identified and fell into four skeletal categories: C18-, C19-, C20- and bis-diterpenoid alkaloids [3–5]. Bullatine A, a C20-diterpenoid alkaloid, is one of the major effective and quality control ingredients identified from A. brachypodi Radix . The chemical structures of C18-, C19-, and C20-diterpenoid alkaloids, as well as bullatine A, are presented in Fig. 1. Unlike the high toxicity of C18- and C19-diterpenoid alkaloids, such as aconitine, bulleyaconitine A, and lappaconitine, bullatine A exhibits significantly lower toxicity (oral half-lethal dose: bullatine A 754 mg/kg vs. aconitine 1.8 mg/kg in mice) [3, 7]. It was reported that systemic administration of bullatine A and the ethanol extract of A. brachypodi Radix including bullatine A effectively attenuated pain responses in the mouse hot-plate, acetic acid, and formalin tests . However, no investigations have been published to date on the anti-nociceptive effects of bullatine A in pain hypersensitivity models.
The crucial role of spinal microglia has been recognized with regard to the initiation and development of chronic pain, including neuropathic pain, inflammatory pain, diabetic neuropathic pain, and bone cancer pain [9–13]. Activated microglia have been implicated in chronic pain states, leading to the production of pro-inflammatory cytokines, such as tumor necrosis factor-α (TNF-α), interleukin (IL)-6, and IL-1β [13, 14]. The cytokines released from activated microglia can consequently induce central sensitization of neurons in the spinal dorsal horn by altering the excitatory or inhibitory synaptic transmission, contributing to pain facilitation . Li et al. showed that bullatine A, by selectively antagonizing P2X7 receptors, inhibited ATP-induced microglial death/apoptosis and P2X receptor-mediated inflammatory response . On the other hand, bulleyaconitine A, a C19-diterpenoid alkaloid of Aconitum, was recently reported to exhibit potent anti-nociception through stimulation of the dynorphin A expression in spinal microglia .
In this paper, we aimed to investigate the anti-hypersensitive effects of bullatine A in a variety of rat models of pain hypersensitivity, including spinal nerve ligation-induced neuropathic pain, streptozotocin-induced diabetic neuropathic pain, complete Freud’s adjuvant (CFA)-induced inflammatory pain, and bone cancer pain. We also explored the mechanisms underlying bullatine A anti-nociception, particularly the involvement of expressions of spinal microglial dynorphin A and pro-inflammatory cytokines. In addition, guan-fu base A is an anti-arrhythmic C20-diterpenoid alkaloid [18–20] and has a similar carbon skeleton structure to bullatine A (Fig. 1). Its effects on nociception in neuropathy and microglial dynorphin A expression were also comparatively studied.
Drugs and reagents
Bullatine A and guan-fu base A were purchased from the National Institute for the Food and Drug Control (Beijing, China) with purity not less than 98 % determined by the manufacturer with high-performance liquid chromatography (HPLC). The molecular weights of both compounds were verified in house by a high-resolution mass spectrum (Waters Corporation, Milford, MA, USA). Dynorphin A(1–17) (sequence: YGGFLRRIRPKLKWDNQ) was synthesized by Dang Gang Peptides Co. (Hangzhou, China) with purity not less than 98 % determined by the manufacturer. Morphine hydrochloride, lidocaine, and minocycline were purchased from the Northeast Pharmaceuticals Group (Shenyang, China), the First Chengdu Pharmaceuticals Group (Chengdu, China), and Yuanye Biotech (Shanghai, China), respectively. 5′-Guanidinonaltrindole (GNTI) and streptozotocin were purchased from Sigma-Aldrich (St. Louis, MO, USA), and CTAP (sequence : FCYWRTXT) and naltrindole were purchased from Abcam (Cambridge, UK) and Tocris (Bristol, UK), respectively. The rabbit polyclonal antibody-neutralizing dynorphin A was purchased from Phoenix Pharmaceuticals (Burlingame, CA, USA). Based on the manufacturer’s information, the antiserum was specific to dynorphin A (100 %), but not to dynorphin B (0 %), β-endorphin (0 %), α-neo-endorphin (0 %), or leu-enkephalin (0 %). Its specificity was also validated by the antigen absorption test from other laboratories [21, 22]. All the drugs and reagents were dissolved or diluted in 0.9 % normal saline except streptozotocin which was freshly dissolved in the citrate buffer (pH 4.3).
Male and female adult (160–250-g body weight) and 1-day-old neonatal Wistar rats were obtained from the Shanghai Experimental Animal Institute for Biological Sciences (Shanghai, China). The adult animals were housed (three to four per cage) in the Shanghai Jiao Tong University Experimental Animal Center (Shanghai, China) at standard room temperature (22 ± 2 °C), under conditions of a 12/12-h reversed light-dark cycle (7:00 a.m.–7:00 p.m.), and received food and water ad libitum. Adult rats were accustomed to the laboratory environment for 3–5 days before the experiments. Experimental study groups (n = 6 in each group) were randomly assigned, and the researcher was blinded to the behavior tests. The research protocols were approved by the Animal Care and Welfare Committee of Shanghai Jiao Tong University and carried out in accordance with the animal care guidelines of the National Institutes of Health.
Primary cell cultures
Glial cells and neurons were isolated from the cortex and spinal cord of 1-day-old neonatal rats. The isolated cortex and spinal cord were minced and then incubated with trypsin. Dissociated cells were suspended in Dulbecco’s modified Eagle’s medium (DMEM) supplemented with 10 % (vol/vol) fetal bovine serum (FBS), penicillin (100 U/mL), and streptomycin (100 μg/mL). For glial cell cultures, cell suspensions were plated in 75-cm2 tissue culture flasks (1 × 107 cells/flask) pre-coated with poly-l-lysine and maintained at 37 °C in a 5 % carbon dioxide incubator. After culture for 8 days, microglial cells were prepared as floating cell suspensions by shaking the flasks at 260 rpm for 2 h. The aliquots were transferred to new plates, and unattached cells were removed by washing with serum-free DMEM. Harvested microglial cells exhibited a purity >95 %, as determined by the CD11b (OX42) or Iba-1 immunoreactivity. After culture for 11 days, astrocytes were prepared by shaking the flasks for 2 h followed by incubation with 10 mL of 0.05 % trypsin-ethylenediamine tetraacetic acid (Invitrogen, Grand Island, NY, USA) in a cell incubator for 15 min to separate the oligodendrocytes from the astrocytes. After trypsin neutralization with 10 mL of the complete DMEM medium, the floating cell suspensions were discarded. A nearly intact layer of astrocytes in the bed layer was then trypsinized and subcultured conventionally. Prepared astrocytes exhibited a purity >90 %, as determined by the glial fibrillary acidic protein (GFAP) immunoreactivity.
For the neuronal culture, cell suspensions were plated in plates pre-coated with poly-l-lysine (100 μg/mL). After 4 h of incubation in the DMEM with 10 % FBS, the medium was changed to the Neurobasal (Invitrogen, Grand Island, NY, USA) containing B27 supplement and 0.5 mM glutamine for further culture. Experiments were initiated 5–6 days after plating. Harvested neurons exhibited a purity >85 %, as determined by the NeuN immunoreactivity.
RNA extraction, reverse transcription, and real-time quantitative polymerase chain reaction (PCR)
TRIzol reagent (Invitrogen, Grand Island, NY, USA) was used to isolate total RNA from rat ipsilateral spinal lumbar enlargements (L3–L5) and primarily cultured cells . A sample of 1 μg of total RNA was reversely transcribed using a ReverTra Ace qPCR RT-Kit (Toyobo Co., Osaka, Japan). Real-time quantitative PCR was carried out with a Mastercycler ep realplex (Eppendorf, Germany) using the Realmaster Mix (SYBR Green I) (Toyobo Co., Osaka, Japan). The fold change was calculated using the 2−ΔΔCt method after normalization to gapdh. The primers were as follows: 5′-CCA AGG TCA TCC ATG ACA AC-3′ (gapdh forward); 5′-TCA TCC ATG ACA AC-3′ (gapdh reverse) ; 5′-CCT GTC CTT GTG TTC CCT GT-3′ (prodynorphin forward); 5′-AGA GGC AGT CAG GGT GAG AA-3′ (prodynorphin reverse) ; 5′-CCC CGA CTA TGT GCT CCT CAC-3′ (TNF-α forward); 5′-AGG GCT CTT GAT GGC GGA-3′ (TNF-α reverse); 5′-GGA AGG CAG TGT CAC TCA TTG TG-3′ (IL-1β forward); 5′-GGT CCT CAT CCT GGA AGC TCC-3′ (IL-1β reverse); 5′-GGG ACT GAT GTT GTT GAC AGC C-3′ (IL-6 forward); and 5′-CAT ATG TAA TTA AGC CTC CGA CTT GTG-3′ (IL-6 reverse) .
For the ex vivo study, sham and neuropathic rats received two intrathecal treatments: (1) 10 μl saline + 10 μl saline; (2) 100 μg minocycline + 10 μl saline; (3) 10 μl saline + 10 μg bullatine A; and (4) 100 μg minocycline + 10 μg bullatine A. The second treatment was administered 4 h after the first treatment, and the ipsilateral spinal lumbar enlargements were obtained 1 h later. The expressions of prodynorphin A, TNF-α, IL-1β, and IL-6 were measured using the real-time PCR.
For the in vitro study, cultured primary cells were under two treatments in the presence and absence of lipopolysaccharides (LPS, 10 ng): (1) control + control; (2) 60 μM minocycline + control; (3) control + 10 μM bullatine A; and (4) 60 μM minocycline + 10 μM bullatine A. The concentration of minocycline was based on the previous references [26–29]. The second treatment was administered 1 h after the first treatment, and the microglia were collected 6 h later. The expressions of prodynorphin A, TNF-α, IL-1β, and IL-6 were measured using the real-time PCR.
Intrathecal catheterization and injection in rats
An 18-cm polyethylene catheter (PE-10: 0.28-mm inner diameter and 0.61-mm outer diameter; Clay Adams, Parsippany, NJ, USA) with a volume of 13 μL was inserted into the rat lumbar level of the spinal cord under inhaled isoflurane anesthesia (4 % for induction and 1 % for maintenance) run by an anesthesiameter (Ugo Basile Gas Anesthesia System, Comerio, Italy). Two days after recovery from anesthesia, the correct positioning of the catheter in the spinal cord was verified by administering 4 % lidocaine (10 μL followed by 15 μL of saline for flushing) with a 50-μL microinjector (Shanghai Anting Microinjector Factory, Shanghai, China). Only rats that had no motor impairment following insertion of the intrathecal catheter were considered for the study, and only rats that developed immediate bilateral paralysis of the hindlimbs following intrathecal administration of lidocaine were selected for the study.
Rat model of neuropathic pain
To induce neuropathic pain, the adult male rats were subjected to spinal nerve ligation as described previously [23, 30]. Under inhaled isoflurane anesthesia, the left L5 and L6 spinal nerves were isolated and tightly ligated with 6–0 silk thread. Sham rats were under the same procedure except for the spinal nerves were not ligated. After ligation, the wound was sutured and the rats were allowed to recover. Of the spinal nerve-ligated animals, only those with marked unilateral allodynia to mechanical stimulation (hindlimb withdrawal thresholds in the operated side <8 g), and no major impairment were included in the study. When intrathecal injection was needed, the intrathecal catheterization was performed in rats at the same time just before spinal nerve ligation. Drug testing started on 2–4 weeks after the surgery of spinal nerve ligation.
Rat model of complete Freud’s adjuvant (CFA)-induced inflammatory nociception
CFA inflammatory nociception was induced according to Butler et al.  and Fan et al. . Briefly, 100 μL of CFA (Sigma-Aldrich, MO, USA) was injected into the tibiotarsal joint of the left hindpaw of each adult male rat under mild inhaled isoflurane anesthesia. The tibiotarsal joint injection of CFA produced immediate and long-lasting inflammation and pain hypersensitivity. The rats entered into the behavior tests 2 days after CFA injection.
Rat model of diabetic neuropathic pain
The adult male rats were fasted for 16 h before receiving a single intravenous injection of streptozotocin (40 mg/kg) [24, 32]. High blood sugar levels were observed on the third day after injection. Mechanical allodynia was measured by electronic von Frey hairs 4–5 weeks afterward.
Rat model of bone cancer pain
The rat bone cancer pain model was produced as described previously [23, 33]. Adult, female rats were anesthetized with intraperitoneal pentobarbital (50 mg/kg). Incisions were made along the patellar ligament to expose the head of the left tibia with minimal damage. A 23-gauge needle was inserted at the site of intercondylar eminence and pierced 7 mm below the knee joint into the medullary cavity of the tibia. The needle was then removed and attached to a 10-μL microinjection syringe. Walker 256 carcinoma cells (4 × 105) in 10 μL the phosphate buffer solution were slowly injected into the tibia cavity. The syringe remained for an additional 1 min to prevent the carcinoma cells from leaking out. The injection site was then closed with aseptic bone wax, and the wound was then closed and dusted with penicillin powder. After recovery from the inoculation surgery, rats were returned to their home cages. The withdrawal thresholds of contralateral and ipsilateral hindlimbs were measured by the application of electronic von Frey hairs 2 weeks afterward.
Behavioral assessments of mechanical allodynia and thermal hyperalgesia in rats
To evaluate mechanical allodynia, the animals were acclimatized for at least 30 min to the test environment, namely a plexiglass box on a metal grid. The hindpaw withdrawal threshold was measured by a 2391 CE Electronic von Frey hair (IITC Life Science Inc, Woodland Hill, CA, USA). The monofilament (with forces ranging from 0.1 to 90 g) was applied to the foot pad with increasing force until the rats suddenly withdrew their hindlimbs. The lowest force producing a withdrawal response was considered as the threshold. Three repeated measurements were made at intervals of approximately 3 min, and the three threshold values were averaged for each hindpaw at each time point.
To assess heat hyperalgesia, rats were put in a plexiglass box on an elevated glass surface. Following an adaption period of at least 30 min, radiant heat source (at a low density of 45) was applied to the plantar medial surface of each hindpaw. The hindpaw withdrawal latency was measured by a 390G Plantar Test Analgesia Meter (IITC Life Science Inc.). To prevent tissue damage, the cutoff was set at 30 s. The paw withdrawal latency was defined as the time from the onset of radiant heat application to the withdrawal of the hindpaws. Both hindpaws were tested independently three times with a 5-min interval between the trials. The result was calculated as the mean of the three repeated measurements.
For the dose response of systemic bullatine A study, two groups of rats from four different pain models were subcutaneously injected with 1 mL/kg saline or 0.3, 0.7, 2, 7, and 20 mg/kg of bullatine A sequentially in 1-h intervals to yield a cumulative dose of approximately 0.3, 1, 3, 10, and 30 mg/kg. The mechanical or thermal thresholds were measured 1 h after each injection. For the dose response of intrathecal bullatine A study, six groups of neuropathic rats received a single intrathecal injection of saline (10 μL) and four doses of bullatine A (0.3, 1, 3, 10 and 30 μg). The withdrawal thresholds to mechanical and thermal stimuli in both contralateral and ipsilateral hindlimbs were measured prior to and 0.5, 1, 2, and 4 h after injection.
For the antagonist intervention study, groups of neuropathic rats in each study received two intrathecal injections of the vehicle (10 μL) + bullatine A (10 μg)/dynorphin A (1 μg) and the antagonist + bullatine A (10 μg)/dynorphin A (1 μg). All of the second treatments were administered 0.5 h after the first treatment except minocycline which was given 4 h after the first injection. The withdrawal thresholds to mechanical stimuli in both contralateral and ipsilateral hindlimbs were measured prior to and 0.5, 1, 2 and 4 h after the second injection. The time and dose regimens of the antagonists in the studies were based on the following references: (1) the microglial inhibitor minocycline (100 μg) [34, 35]; (2) the specific dynorphin A antiserum (1:10 dilution) ; and (3) the selective μ-opioid antagonist CTAP (10 μg), k-opioid antagonist GNTI (50 μg), and σ-opioid antagonist naltrindole (5 μg) .
Double immunofluorescence labeling of dynorphin A and microglia, astrocytes, or neurons on spinal cord sections was undertaken and observed using a TCS SP8 confocal microscope (Leica Microsystems, Wetzlar, Germany) by modified protocols . Rats were anesthetized by pentobarbital injection (40 mg/kg) and intracardially perfused with 100 mL normal saline, followed by 60 mL of 4 % paraformaldehyde (w/v) in PBS. Spinal lumbar enlargements (L3–L5) were collected and fixed in 4 % buffered paraformaldehyde for 12 h and placed in 30 % sucrose solution for 48 h at 4 °C. Tissues were entrapped in the OCT embedding agent (Leica Microsystems) and cut into 30-μm-thick frozen sections, which were incubated in 10 % goat serum (v/v) and 0.5 % Triton X-100 (v/v) in PBS for 1 h, then incubated with the rat dynorphin A antibody (1:100; rabbit polyclonal, Phoenix Pharmaceuticals) and other primary antibodies at 4 °C for 24 h. Spinal neuronal and glial cells were identified by the following cellular markers: Iba-1 (1:100; mouse monoclonal; Millipore, Darmstadt, Germany) for microglia, GFAP (1:100; mouse polyclonal; Millipore) for astrocytes, and NeuN (1:60; mouse polyclonal; Millipore) for neurons. The dynorphin A was visualized with the Alexa-555-conjugated goat anti-rabbit secondary antibody (1:200, Invitrogen). Other antibodies were detected with the Alexa-488-conjugated goat anti-mouse secondary antibody (1:200, Invitrogen).
For quantity measurement of dynorphin A and/or Iba-1/GFAP/NeuN-immunopositive cell intensity in the spinal cord, photomicrographs of the medial three fourths of the superficial dorsal horn (laminas I–V) were captured under a 10× or 40× magnification. The positively stained surface area was measured by a researcher blinded to the experimental conditions using a computer-assisted image analysis program (ImageJ Software, National Institutes of Health) after low and high thresholds were set to exclude background fluorescence and include immunofluorescent intensity measurements only from positively stained areas. A co-localization analysis was performed using ImageJ software with a co-localization finder to generate images in which co-localized pixels appeared as white. The same configuration setup was used to measure all surface areas in each experimental group at the same time. The averaged percentage immunolabeled surface area was the fraction of the positive immunofluorescent surface area of the total measured picture area from three nonadjacent sections of each spinal cord. Data were then calculated from six rats of each group.
Data evaluation and statistical analysis
The percentage of the maximal possible effect (% MPE) was calculated using the following formula: (post-drug threshold in ipsilateral hindlimb − baseline threshold in ipsilateral hindlimb)/(baseline threshold in contralateral hindlimb − baseline threshold in ipsilateral hindlimb) × 100 . The % MPE values near 100 indicate normal mechanical thresholds (i.e., near contralateral thresholds) while values near 0 indicate allodynia. For the dose–response curve analysis, the parameters, i.e., minimum effect, maximum effect (E max), half-effective dose (ED50) or half-effective concentration (EC50), and Hill coefficient (n), were calculated by fitting non-linear least-square curves to the relation Y = a + bx, where x = [D]n/(ED50 n + [D]n) or [C]n/(EC50 n + [C]n). The value of ED50 or EC50 and b (E max) were projected by yielding a minimum residual sum of squares of deviations from the theoretical curve . The data were expressed as means ± SEM or with 95 % confidence limits, and there were no missing data. The statistical significance was evaluated by unpaired and two-tailed Student t tests and one-way or two-way repeated-measure analysis of variance (ANOVA) in Prism (version 5.01, GraphPad Software, Inc., San Diego, CA, USA). The post hoc Student–Newman–Keuls test was conducted when the effect of the drug (dose) (for the one-way ANOVA, the factor was drug [dose]; for the two-way ANOVA, the factors were drug [dose], time, and their interaction) was observed to be statistically significant. The probability values were two-tailed, and the statistical significance criterion P value was 0.05.
Systemic bullatine A specifically attenuated pain hypersensitivity in a variety of pain models
The anti-nociceptive effect of bullatine A was first examined in the rat model of neuropathic pain. Tight ligation of peripheral L5/L6 spinal nerves induced marked ipsilateral mechanical allodynia and thermal hyperalgesia. Two groups of neuropathic rats received subcutaneously injections of the vehicle (0.9 % saline, 1 mL/kg) and bullatine A (3 mg/kg). The paw withdrawal responses to mechanical and thermal stimuli were measured before and 0.5, 1, 2, and 4 h after injection. Subcutaneous bullatine A time-dependently alleviated mechanical allodynia (Fig. 2a) and thermal hyperalgesia (Fig. 2b) in ipsilateral paws, with the peaks at 1 h and durations of nearly 4 h (P < 0.05, by two-way ANOVA followed by the post hoc Student–Newman–Keuls tests). Subcutaneous bullatine A did not significantly alter normal withdrawal response to mechanical and heat stimuli in contralateral paws. No apparent sedation or motor side effects of bullatine A were observed during the study period. In addition, cumulative dose–response of bullatine A was conducted in two groups of neuropathic rats. Animals received repetitive subcutaneous injection of saline or bullatine A at 1-h intervals. The mechanical or thermal thresholds were measured before and 1 h after each dose injection. Subcutaneous bullatine A dose-dependently alleviated mechanical allodynia (Fig. 2c) and thermal hyperalgesia (Fig. 2d) in ipsilateral paws. The dose–response analyses were projected from the % MPE values from each dose for the blockade of mechanical allodynia and heat hyperalgesia. The ED50 values calculated were 1.9 and 0.7 mg/kg, and the E max values were 56.6 and 66.1 % MPE, respectively (Fig. 2e).
Intravenous injection of streptozotocin (40 mg/kg) in rats produced immediate and permanent high blood sugar (>16.7 mmol/L) and resulted in stable painful neuropathy 4–5 weeks later, represented by bilateral mechanical allodynia . Subcutaneous injection of bullatine A (3 mg/kg) was effective in attenuation of mechanical allodynia in a time-dependent manner, with the peak effect at 1 h after injection (P < 0.05, by two-way ANOVA followed by the post hoc Student–Newman–Keuls tests) (Fig. 2f). Cumulative doses (0.3–30 mg/kg) of subcutaneous bullatine A attenuated mechanical allodynia in a dose-dependent manner (Fig. 2g), with the ED50 value of 1.2 mg/kg and E max value of 65.5 % MPE, which were projected from the dose–response analyses using % MPE at 1 h after injection calculating from the pre-streptozotocin paw withdrawal thresholds of 37.9 ± 1.9 g (Fig. 2h).
We further determined the anti-nociceptive effect of bullatine A in CFA-induced acute inflammatory nociception. Two groups of CFA-treated rats received subcutaneous injection of the vehicle (0.9 % saline, 1 mL/kg) and bullatine A (3 mg/kg). Subcutaneous injection of bullatine A did not significantly alter the paw withdrawal responses in contralateral paws during the 4-h observation period. However, bullatine A significantly blocked mechanical allodynia (Fig. 3a) and thermal hyperalgesia (Fig. 3b) in ipsilateral paws in a time-dependent manner, with the peak of 1 h after injection (P < 0.05, by two-way ANOVA followed by the post hoc Student–Newman–Keuls tests). In a cumulative dose range of 0.3 to 30 mg/kg, subcutaneous injection of bullatine A dose-dependently alleviated mechanical allodynia (Fig. 3c) and thermal hyperalgesia (Fig. 3d) in ipsilateral paws. The calculated ED50 values for the blockade of mechanical allodynia and thermal hyperalgesia were 1.4 and 0.6 mg/kg, and the E max values were 50.2 % MPE and 60.2 % MPE, respectively (Fig. 3e).
Tibia implantation of cancer cells produced progressive mechanical allodynia in rats 14 days after surgery. As shown in Fig. 3f, subcutaneous injection of bullatine A (3 mg/kg) blocked bone cancer-induced mechanical allodynia in ipsilateral paws with the peak effect at 1 h and the duration of almost 4 h (P < 0.05, by two-way ANOVA followed by the post hoc Student–Newman–Keuls tests). It did not significantly affect withdrawal thresholds in contralateral paws. Subcutaneous injection of bullatine A (0.3 to 30 mg/kg, cumulative doses) dose-dependently increased withdrawal thresholds in ipsilateral paws (Fig. 3g), with the ED50 value of 0.9 mg/kg and E max value of 45.6 % MPE calculated from the % MPE values at 1 h after injection (Fig. 3h).
Intrathecal bullatine A specifically attenuated neuropathic pain
In order to test the anti-nociceptive efficacy of bullatine A in the spinal cord, six groups of neuropathic rats received a single intrathecal injection of saline (10 μL) or bullatine A at different doses (0.3, 1, 3, 10, and 30 μg). As shown in Fig. 4a, intrathecal bullatine A markedly suppressed mechanical allodynia in ipsilateral paws in a dose-dependent manner but did not significantly alter withdrawal thresholds in contralateral paws. No apparent sedation or motor side effects of bullatine A were observed during the study period. The anti-allodynic effect was time-dependent, with a peak effect at 1 h after injection and a duration of 4 h. Dose–response analysis showed that the ED50 value was 1.1 μg and E max value was 55.5 % MPE, as calculated from the 1 h data after injection (Fig. 4b). On the contrary, intrathecal injection of the bullatine A analog guan-fu base A, at the most tolerable dose of 100 μg, did not show any significant anti-allodynic effects (Fig. 4c).
Bullatine A upregulated the spinal microglial prodynorphin expression
To test whether bullatine A affected the spinal gene expressions of dynorphin A and pro-inflammatory cytokines, four groups of neuropathic rats received intrathecal injection of saline (10 μL) or minocycline (100 μg) followed by a single dose of saline (10 μL) or bullatine A (10 μg) 4 h afterward. The rats were sacrificed 1 h after the second treatment, and ipsilateral lumbar enlargements (L3–L5) of the spinal cord were obtained. The cellular prodynorphin gene expression relative to gapdh was measured by real-time quantitative PCR in spinal homogenates. Since we recently reported that the C19-diterpenoid alkaloid bulleyaconitine-increased dynorphin A level measured by enzyme-linked immunosorbent assay was in parallel with the prodynorphin gene expression , the prodynorphin gene expression was only measured in this study. As shown in Fig. 5a, peripheral nerve injury approximately 20 days after surgery did not significantly change the basal prodynorphin gene expression, which was consistent with our previous results in which spinal nerve injury did not alter the basal spinal dynorphin A level . Intrathecal bullatine A significantly increased the prodynorphin expression by 1.9- and 2.1-fold in the sham and neuropathic rats, respectively. Intrathecal injection of the microglial inhibitor minocycline [40, 41] completely inhibited bullatine A-increased prodynorphin expression (P < 0.05, by one-way ANOVA followed by the post hoc Student–Newman–Keuls tests), although it did not significantly alter the baseline prodynorphin expression.
The expression of pro-inflammatory cytokines was also measured in the same rats. Compared to the sham rats, spinal nerve ligation dramatically increased the spinal expression of TNF-α, IL-1β, and IL-6 by approximately 8-, 6- and 14-fold, respectively (P < 0.05, by one-way ANOVA followed by post hoc Student–Newman–Keuls tests). Pretreatment with minocycline completely blocked nerve injury-increased TNF-α (Fig. 5b), IL-1β (Fig. 5c), and IL-6 (Fig. 5d) expression (P < 0.05, by one-way ANOVA followed by post hoc Student–Newman–Keuls tests). In contrast, intrathecal administration of bullatine A did not significantly affect the gene expression of cytokines, including TNF-α (Fig. 5b), IL-1β (Fig. 5c), and IL-6 (Fig. 5d), in either sham or neuropathic rats.
We further determined the effects of bullatine A on the expression of prodynorphin and pro-inflammatory cytokines in microglial cells in the presence and absence of LPS. Cultured primary microglial cells (1 × 106 cells per well) from the cortex of neonatal rats were treated with minocycline (60 μM) 1 h prior to LPS (10 ng/mL) or bullatine A (10 μM) treatment, and microglial cells were collected 6 h later. Treatment with minocycline at 60 μM for 24 h did not affect microglial viability measured by the MTT assay (100 % ± 9.5 % vs. 103.8 % ± 6.0 %, n = 5), consistent with the previous report. As shown in Fig. 6a, LPS (10 ng/mL) did not significantly change the baseline expression of the prodynorphin gene , whereas bullatine A (10 μM) markedly increased the prodynorphin expression by 2.0- and 2.5-fold in the absence and presence of LPS, respectively. In agreement with the in vivo findings in the spinal cord, minocycline completely inhibited bullatine A-induced increase in the prodynorphin expression (P < 0.05, by one-way ANOVA followed by post hoc Student–Newman–Keuls tests), without affecting the baseline level in the absence and presence of LPS. However, bullatine A at 10 μM did not significantly affect the prodynorphin gene expression in cultured primary astrocytes originated from the cortex (Fig. 6b) or neurons either from the cortex (Fig. 6b) or from the spinal cord (relative expression value 1.0 ± 0.1 vs. 0.9 ± 0.3).
In order to compare the stimulatory effect of bullatine A and guan-fu base A on the prodynorphin gene expression, cultured primary microglial cells were treated with different concentrations of bullatine A (1 × 10−6, 3 × 10−5, 1 × 10−5, 3 × 10−5, and 1 × 10−4 M) or of guan-fu base A (1 × 10−6, 3 × 10−5, 1 × 10−5, 3 × 10−5, 1 × 10−4 and 3 × 10−4 M) for 6 h and the cellular prodynorphin gene was measured by real-time PCR. Cell viability was not affected under the tested bullatine A or guan-fu base A. As shown in Fig. 6c, bullatine A increased the prodynorphin gene expression in a concentration-dependent manner, with an EC50 value of 3.2 μM. In contrast, guan-fu base A up to 300 μM did not significantly affect the expression of prodynorphin.
Treatment with LPS produced an extraordinary increases (26-, 30-, and 35-fold) in the expressions of TNF-α, IL-1β, and IL-6 mRNA, respectively (P < 0.05, by one-way ANOVA followed by post hoc Student–Newman–Keuls tests). As shown in Fig. 6d–f, minocycline completely blocked LPS-induced overexpression of TNF-α, IL-1β, and IL-6 (P < 0.05, by one-way ANOVA followed by the post hoc Student–Newman–Keuls tests), although it did not affect their baseline expressions. In contrast, the treatment with bullatine A did not significantly inhibit the gene expression of those pro-inflammatory cytokines in the presence or absence of LPS stimulation.
Bullatine A induced dynorphin A upregulation in spinal microglia in neuropathic rats
We examined the differential distribution of dynorphin A in the spinal cord of neuropathic rats treated with intrathecal saline (10 μL) or bullatine A (10 μg). In control rats, the dynorphin A immunofluorescence staining was widely expressed throughout the white and gray matter of the spinal cord, particularly in laminae I–V of the dorsal horn and dorsolateral to the central canal (Fig. 7a), in agreement with previous immunohistochemical staining in naïve and polyarthritic rats . After 1 h treatment of bullatine A, dynorphin A staining was much more intense in the ipsilateral dorsal horn (Fig. 7b). Upregulation of dynorphin A expression in the ipsilateral dorsal horn I–V laminae was quantified using the computer-assisted image quantification program. Compared to saline-treated rats, bullatine A significantly increased the averaged percentage immunolabeled surface area by 104 % (P < 0.05, unpaired and two-tailed Student t test) (Fig. 7c). Immunofluorescence was also stained with the microglial marker Iba-1, astrocytic marker GFAP, and neuronal marker NeuN. After treating with bullatine A, ipsilateral (laminae I–V) expressions of microglial (Fig. 7d–f), astrocytic (Fig. 7g–i), and neuronal (Fig. 7j–l) markers were not significantly changed, compared to the saline-treated rats.
Dynorphin A has been reported to be localized and secreted in neurons, astrocytes, and microglia [17, 43, 44]. To identify cell types that specifically promote expression of dynorphin A in the spinal dorsal horn after bullatine A treatment, we performed double immunofluorescence labeling of dynorphin A with microglial, astrocytic, and neuronal cellular markers. As shown in Fig. 8a–d, dynorphin A immunofluorescence was co-labeled with Iba-1 on microglia in the I–V laminae of the dorsal horn in saline-treated rats. Double immunofluorescence of dynorphin A with Iba-1 was significantly upregulated after treatment of bullatine A by 3.4-fold, as measured using the computer-assisted image analysis program (P < 0.05, unpaired and two-tailed Student t test) (Fig. 8e). Dynorphin A was also co-labeled with GFAP on astrocytes and NeuN on neurons in the spinal dorsal horn. However, there was no significant difference in co-immunofluorescence staining of dynorphin A and GFAP (Fig. 8f–j) or NeuN (Fig. 8k–o) between saline- and bullatine A-treated rats.
Intrathecal the microglial inhibitor, dynorphin A antiserum, and k-opioid receptor antagonist suppressed bullatine A-induced anti-nociception
In order to test whether the spinal microglial dynorphin A expression was causally associated with bullatine A anti-nociception, the microglial inhibitor minocycline, the specific dynorphin A antiserum , and antagonists of the opioid receptor subtypes were applied. Two groups of neuropathic rats were first given an intrathecal injection of 10 μL of saline or 100 μg of minocycline, followed by a second intrathecal injection of 10 μg of bullatine A 4 h later. Hindpaw withdrawal thresholds to the mechanical stimulus were measured before and 0.5, 1, 2, and 4 h after the second administration. The effects of minocycline in neuropathic pain are complex when different treatment regimens are applied. It is generally accepted that treatment with minocycline may not be anti-nociceptive in established neuropathy, although its preemptive treatment prevented the induction and/or early development of neuropathic pain [17, 24, 26, 27, 40, 45–48]. As shown in Fig. 9a, intrathecal injection of bullatine A produced time-dependent anti-allodynic effects. Minocycline did not significantly alter the basal withdrawal response in either paws but entirely inhibited the anti-allodynic effects exerted by bullatine A in ipsilateral paws (P < 0.05, by two-way ANOVA followed by the post hoc Student–Newman–Keuls tests).
Similarly, two groups of neuropathic rats received intrathecal injection of 10 μL of blank rabbit serum or 10 μL of the dynorphin A antiserum (1:10 dilution). Each rat received a second intrathecal injection of 10 μg of bullatine A 0.5 h later. The paw withdrawal responses to the mechanical stimulus were measured. The time and dose regimen of the dynorphin A antiserum was based on the previous publications . Intrathecal injection of bullatine A produced time-dependent anti-allodynia in the ipsilateral paws. The dynorphin A antiserum entirely prevented bullatine A from suppressing mechanical allodynia (P < 0.05, by two-way ANOVA followed by the post hoc Student–Newman–Keuls tests), although it did not significantly alter the basal withdrawal response in either paws (Fig. 9b).
As dynorphin A has variously been reported to inhibit [49, 50] or facilitate pain [51, 52], the effect of dynorphin A on nociception was tested in our conditions. Three groups of neuropathic rats received intrathecal injection of saline (10 μL) and two non-paralytic doses (1 and 10 μg) of the synthetic dynorphin A. Intrathecal administration of dynorphin A(1–17) dose-dependently suppressed mechanical allodynia in ipsilateral paws, with the peak effect (48.8 and 60.5 % MPE) at 1 h and a duration of 4 h (P < 0.05, by two-way ANOVA followed by the post hoc Student–Newman–Keuls tests) (Fig. 9c).
In physiological conditions, dynorphin A modulates anti-nociceptive response primarily through the activation of the k-opioid receptor located on neurons in the descending inhibitory system, although it has some affinity for μ- and δ-opioid receptors [53, 54]. To confirm which subtype of opioid receptors was responsible for dynorphin A anti-nociception, we tested the possible blockade effects of the selective μ-opioid receptor antagonist CTAP , k-opioid receptor antagonist 5′-guanidinonaltrindole (GNTI) , and δ-opioid receptor antagonist naltrindole  on dynorphin A-exerted anti-allodynia. It is noted that we selected GNTI instead of the traditionally used nor-binaltorphimine as the latter was recently reported to be an inverse agonist of the k-opioid receptor [58, 59]. Four groups of neuropathic rats received the following pairs of intrathecal injections: saline (10 μL) + dynorphin A(1–17) (1 μg), GNTI (50 μg) + dynorphin A(1–17) (1 μg), CTAP (10 μg) + dynorphin A(1–17) (1 μg), and naltrindole (5 μg) + dynorphin A(1–17) (1 μg). The second treatment occurred 0.5 h after the first injection, and the paw withdrawal responses to the mechanical stimulus were measured before and 0.5, 1, 2, and 4 h thereafter. As shown in Fig. 9d, intrathecal injection of GNTI, but not CTAP or naltrindole, totally prevented the anti-allodynic effect of dynorphin A (P < 0.05, by two-way ANOVA followed by the post hoc Student–Newman–Keuls tests), although it was ineffective in altering the basal withdrawal thresholds in both paws.
Lastly, the above selective opioid receptor antagonist was employed to determine which subtype of opioid receptors participated in bullatine A anti-nociception. Four groups of neuropathic rats received intrathecal injections of saline (10 μL), GNTI (50 μg), CTAP (10 μg), and naltrindole (5 μg) before being intrathecally given bullatine A (10 μg). The second administration occurred 0.5 h after the first injection, and the paw withdrawal responses to mechanical stimulus were measured. As shown in Fig. 9e, intrathecal injection of bullatine A induced time-dependent anti-allodynia in ipsilateral paws. In contrast to the negative effects of intrathecal CTAP and naltrindole on bullatine A anti-allodynia, intrathecal injection of GNTI completely inhibited the anti-allodynic effects of bullatine A (P < 0.05, by two-way ANOVA followed by the post hoc Student–Newman–Keuls tests), without affecting the baseline withdrawal response in both paws.
Our study, for the first time, demonstrated that bullatine A was effective in blocking spinal nerve ligation- and CFA-induced mechanical allodynia and thermal hyperalgesia and diabetic- and bone cancer-induced mechanical allodynia with efficacies of 45–70 % MPE and ED50 values of 0.9–1.9 mg/kg by subcutaneous injection. It is worth noting that bullatine A does not show any inhibitory effects of nociceptive responses stimulated by mechanical or thermal stimuli in normal physiological conditions, suggesting that bullatine A was rather anti-hypersensitive than anti-noxious. Our results indicate that bullatine A is effective in the blockade of pain hypersensitivity, independent of pain models employed, and provide the pharmacological evidence to support its potential use for the treatment of chronic pain.
Emerging evidence indicates that spinal microglia activation and microglia-derived pro-inflammatory cytokines, such as IL-1β, IL-6, and TNF-α, play a crucial role in the pathogenesis of neuropathic pain and other pathological conditions [60, 61]. As expected, we observed that LPS and spinal nerve injury dramatically increased expressions of TNF-α, IL-1β, and IL-6 in cultured primary microglial cells by 26- to 35-fold and in the spinal cord by 6- to 14-fold, which were completely blocked by the microglial inhibitor minocycline. Minocycline is a broad-spectrum antimicrobial tetracycline derivative and is generally considered to be a specific inhibitor of microglia (but not astrocytes [62, 63] or oligodendroglial progenitors ), although it was reported to have some direct biological effects in neurons [65, 66]. Minocycline has been extensively used to study the role of microglia in experimental models of brain ischemia , traumatic brain injury , and peripheral nerve injury-induced neuropathy [17, 24, 26, 27, 34, 40, 45]. In contrast, bullatine A (1–50 μM) was recently reported to decrease ATP-induced overexpression of IL-1β, IL-6, and inducible nitric oxide synthase in mouse BV-2 microglial cells . However, our data do not support the observation either in vitro or in vivo, as bullatine A at 10 μM or 10 μg did not inhibit LPS- or spinal nerve injury-induced overexpression of the pro-inflammatory cytokines in either cultured microglial cells or the spinal cord.
Instead, we revealed that the anti-hypersensitivity of bullatine A was produced by the stimulation of dynorphin A expression in spinal microglia. Dynorphin A is an endogenous opioid neurotransmitter produced in various regions of the brain, including the hypothalamus, the striatum, the hippocampus, and the spinal cord [69–71]. The localization and secretion of dynorphin A have been observed in neurons [72, 73], astrocytes , and microglia . The effects of dynorphin A on nociception are bimodal depending on physiological vs. pathological conditions, low vs. high concentrations, and time courses during the development of pain hypersensitivity . At low doses, dynorphin A produces analgesia primarily through activation of k-opioid receptors located on the neurons in the descending inhibitory system [50, 53, 54, 74], while at high concentrations it may induce allodynia and paralysis through the activation of neuronal and microglial N-methyl-d-aspartic acid (NMDA) receptors [50, 75–77]. The involvement of spinal microglial-expressed dynorphin A in bullatine A anti-hypersensitivity is supported by the following findings. First, bullatine A stimulated prodynorphin expression in the primary culture of microglia (but not of neurons or astrocytes) and the spinal cord and produced anti-nociception, which were completely blocked by the microglial inhibitor minocycline. In addition, double immunofluorescence staining technology revealed that intrathecal bullatine A-stimulated dynorphin A protein in the ipsilateral spinal dorsal horn was specifically co-localized with microglia (but not neurons or astrocytes). Moreover, the specific anti-dynorphin A serum, which has been found to block the anti-allodynic effects of bulleyaconitine A in neuropathic pain , entirely eliminated bullatine A anti-hypersensitivity. Furthermore, the highly selective k-opioid receptor antagonist GNTI at the dose to block the anti-nociceptive effect of the synthetic dynorphin A completely inhibited the anti-hypersensitive effects of bullatine A in neuropathy. In contrast, the μ-opioid receptor antagonist CTAP or δ-opioid receptor antagonist naltrindole was not effective in blocking bullatine A anti-nociception. These results indicate that bullatine A exerts anti-hypersensitivity by specifically stimulating spinal microglia to express and secrete dynorphin A, which then acts on the k-opioid receptors located on the post-microglial synaptic neurons.
We have also recently reported that the C19-diterpenoid alkaloids aconitine and bulleyaconitine A produced anti-hypersensitivity entirely via stimulation of spinal microglial dynorphin A expression and secretion which were not dependent on the interaction with neuronal sodium channels, and their anti-hypersensitivity was separated from the neurotoxicity . Taken together, our results indicate that both C19- and C20-diterpenoid alkaloids exhibit dynorphin A expression properties, regardless of their different carbon skeletal structures. However, although the anti-nociceptive efficacy was nearly the same for both bulleyaconitine A and aconitine, the anti-allodynic potency of bullatine A is nearly 10–32-fold less that of bulleyaconitine A in spinal nerve ligation-induced neuropathic rats (ED50: 59.5 μg/kg vs. 1.9 mg/kg for subcutaneous injection and 111.3 ng vs. 1.1 μg for intrathecal injection) . In addition, the potency of bullatine A (EC50 3.2 μM) to stimulate dynorphin A expression in microglia is around 76-fold less than that of bulleyaconitine A (EC50 41.9 nM) . The potencies of anti-hypersensitivity and dynorphin A expression stimulation between bullatine A and bulleyaconitine A are well positively correlated, which further supports our note that stimulation of dynorphin A expression in spinal microglia entirely mediates the anti-hypersensitivity of Aconitum and its diterpenoid alkaloids. The findings have made a conceptual advancement, as it was generally accepted that the interaction of Aconitum and its alkaloids with neuronal sodium channels were responsible for their analgesia and toxicity [4, 5]. Furthermore, it has been reported that glucagon-like peptide 1 receptor (GLP-1) receptor agonism-induced anti-nociception in pain hypersensitivity through spinal microglial expression of β-endorphin [24, 26]. Our findings of bullatine A and bulleyaconitine A further highlight that spinal microglia exert an anti-nociceptive role, in addition to their known pro-nociceptive functions [9–13]. However, it is worthy to note that activation of microglia may not be required for bullatine A and bulleyaconitine A to induce dynorphin A expression, as both of them stimulated dynorphin A expression by similar degrees in the ipsilateral spinal cord from both sham rats and established neuropathic rats  and as bullatine A induced dynorphin A expression in the primary culture of microglia with and without LPS challenge.
Mitogen-activated protein kinases (MAPKs) are a family of evolutionally conserved molecules. After being activated by phosphorylation, they play a critical role in cell signaling, particularly in relation to microglial activation [13, 45, 78]. MAPKs include p38, extracellular signal-regulated kinase (ERK1/2) and c-Jun N-terminal kinase (JNK) [79–81]. Minocycline is likely a non-selective inhibitor of MAPKs, as it has been found to inhibit activation of all of three MAPK subtypes [34, 35, 82–86]. We recently discovered that bulleyaconitine A significantly induced cyclic AMP production and activation of cAMP-dependent protein kinase A (PKA); subsequently, PKA specifically regulated the activity of p38 (but not ERK1/2 or JNK) MAPK and its translocation to the nucleus and then phosphorylated the transcription factor cyclic AMP-response element binding protein (CREB), leading to increased prodynorphin expression and anti-nociception (Li et al., unpublished data, 2016). Given that minocycline completely blocked bulleyaconitine A- and bullatine A-induced spinal microglial dynorphin A expression and anti-nociception, and that both bullatine A and bulleyaconitine A are diterpenoid alkaloids and originated from the genus Aconitum, we speculate that bullatine A shares the same mechanism with bulleyaconitine A, by which bullatine A stimulates dynorphin A expression by activation of the microglial cyclic AMP/PKA/p38 MAPK/CREB signaling pathway.
The structure-activity relationships of C18- and C19-diterpenoid alkaloids of Aconitum have been extensively studied . The C8-acetyl and C14-benzoyl groups were found to be essential for aconitines to stimulate spinal microglial dynorphin A expression and subsequent anti-hypersensitivity, while hydroxylation at C3 and C15 was also helpful for the actions . In contrast, little information has been reported about the structure-activity relationship for C20-diterpenoid alkaloids to produce anti-nociception. There are seven types of C20-diterpenoid alkaloids in nature and five types exist in the Aconitum species. Bullatine A belongs to the denudatine-type (six-membered ring and a chemical bond between C-20 and C-7), and guan-fu base A belongs to the hetisine-type (the most complicated structure in C20-diterpenoid alkaloids with a seven-membered ring and a link between N and C-6), with the significant difference in which the hydroxyl group exists in C15 only in bullatine A [3, 88]. The biogenetic relationship studies between C20- and C19-diterpenoid alkaloids revealed that the bio-transformation of denudatine-type (but not hetisine-type) diterpenoid alkaloids is one of the major pathways to form aconitines, which was specifically regulated by the C15-hydroxyl group . Our study demonstrated that the treatment with guan-fu base A up to 300 μM did not stimulate dynorphin A gene expression in cultured microglia and intrathecal guan-fu base A up to 100 μg did produce anti-nociception in neuropathy, whereas bullatine A was markedly positive in the parameters with high EC50 of 3.2 μM and ED50 of 1.1 μg. The differential activities suggest that the C15-hydroxyl group may be required for C20-diterpenoid alkaloids to express dynorphin A and subsequently anti-nociception.
Systemic and intrathecal injection of bullatine A specifically and dose-dependently inhibits pain hypersensitivity in a variety of rat models of pain, including neuropathic pain, bone cancer pain, inflammatory pain, and diabetic neuropathic pain. Bullatine A stimulates dynorphin A expression in the spinal cord and cultured primary microglia in a minocycline-sensitive manner. The spinal anti-allodynic effects of bullatine A are entirely blocked by minocycline, the specific dynorphin A antiserum, and the selective k-opioid receptor antagonist, indicating that bullatine A anti-nociception is entirely mediated by the stimulation of spinal microglial dynorphin A expression. Our results suggest that both C19- and C20-diterpenoid alkaloids stimulate dynorphin A expression, regardless of their different carbon skeletal structures and further highlight that spinal microglia exert an anti-nociceptive role in addition to their known pro-nociception.
Analysis of variance
Complete Freund’s adjuvant
- EC50 :
- ED50 :
- E max :
Glucagon-like peptide 1 receptor
High-performance liquid chromatography
N-methyl-d-aspartic acid receptor
Tumor necrosis factor-α
- % MPE:
% maximal possible effect
China Pharmacopoeia Committee. Pharmacopoeia of People’s Republic of China. Beijing: People’s Medical Publishing House; 1977. p. 580.
Li GN. Yunnan Zhiwu Zhi [Chinese Medicine Record of Yunnan]. Yunnan: Yunnan Science and Technology Press; 1990. p. 472–3.
Xiao PG, Wang FP, Gao F, Yan LP, Chen DL, Liu Y. A pharmacophylogenetic study of Aconitum L. (Ranunculaceae) from China. Acta Phytotaxon Sin. 2006;44:1–46.
Ameri A. The effects of Aconitum alkaloids on the central nervous system. Prog Neurobiol. 1998;56:211–35.
Chodoeva A, Bosc JJ, Robert J. Aconitum alkaloids and biological activities. In: Ramawat KG, Mérillon JM, editors. Nature products. Berlin-Heidelberg: Springer; 2013. p. 1503–23.
Teng SY, Zhang SX, Niu K, Zhai LJ, Wang SJ. Development and validation of an LC-MS/MS method for the determination of bullatine A in rat plasma: application to a pharmacokinetic study. Biomed Chromatogr. 2015;29:1798–804.
Singhuber J, Zhu M, Prinz S, Kopp B. Aconitum in traditional Chinese medicine—a valuable drug or an unpredictable risk? J Ethnopharmacol. 2009;126:18–30.
Ren W, Yuan L, Li J, Huang XJ, Chen S, Zou DJ, Liu XM, Yang XZ. Ethanolic extract of Aconiti brachypodi Radix attenuates nociceptive pain probably via inhibition of voltage-dependent Na(+) channel. Afr J Tradit Complement Altern Med. 2012;9:574–83.
Jin SX, Zhuang ZY, Woolf CJ, Ji RR. p38 mitogen-activated protein kinase is activated after a spinal nerve ligation in spinal cord microglia and dorsal root ganglion neurons and contributes to the generation of neuropathic pain. J Neurosci. 2003;23:4017–22.
Wang XW, Li TT, Zhao J, Mao-Ying QL, Zhang H, Hu S, Li Q, Mi WL, Wu GC, Zhang YQ, Wang YQ. Extracellular signal-regulated kinase activation in spinal astrocytes and microglia contributes to cancer-induced bone pain in rats. Neuroscience. 2012;217:172–81.
Wang D, Couture R, Hong Y. Activated microglia in the spinal cord underlies diabetic neuropathic pain. Eur J Pharmacol. 2014;728:59–66.
Raghavendra V, Tanga FY, DeLeo JA. Complete Freunds adjuvant-induced peripheral inflammation evokes glial activation and proinflammatory cytokine expression in the CNS. Eur J Neurosci. 2004;20:467–73.
Taves S, Berta T, Chen G, Ji RR. Microglia and spinal cord synaptic plasticity in persistent pain. Neural Plast. 2013;2013:753656.
Chauvet N, Palin K, Verrier D, Poole S, Dantzer R, Lestage J. Rat microglial cells secrete predominantly the precursor of interleukin-1beta in response to lipopolysaccharide. Eur J Neurosci. 2001;14:609–17.
Kawasaki Y, Zhang L, Cheng JK, Ji RR. Cytokine mechanisms of central sensitization: distinct and overlapping role of interleukin-1beta, interleukin-6, and tumor necrosis factor-alpha in regulating synaptic and neuronal activity in the superficial spinal cord. J Neurosci. 2008;28:5189–94.
Li J, Ren W, Huang XJ, Zou DJ, Hu X. Bullatine A, a diterpenoid alkaloid of the genus Aconitum, could attenuate ATP-induced BV-2 microglia death/apoptosis via P2X receptor pathways. Brain Res Bull. 2013;97:81–5.
Li TF, Fan H, Wang YX. Aconitum-derived bulleyaconitine A exhibits antihypersensitivity through direct stimulating dynorphin A expression in spinal microglia. J Pain. 2016;17:530–48.
Chen WZ, Dong YL, Zhang YF, Ding GS. Anti-arrhythmia effects of guan-fu base A. Zhongguo Yao Li Xue Bao. 1983;4:247–50.
Wang YQ, Su L, Gong GQ, Liu JH. Guanfu base A inhibit the post-infarction ventricular arrhythmias in dogs. Yao Xue Xue Bao. 1994;29:141–4.
Dong YL, Chen WZ. Effects of guan-fu base a on experimental cardiac arrhythmias and myocardial contractility. Yao Xue Xue Bao. 1995;30:577–82.
Yamada K, Ono Y, Kubo KY, Yamamoto T, Onozuka M. Occlusal disharmony transiently impairs learning and memory in the mouse by increasing dynorphin A levels in the amygdala. Tohoku J Exp Med. 2013;230:49–57.
Wakabayashi Y, Nakada T, Murata K, Ohkura S, Mogi K, Navarro VM, Clifton DK, Mori Y, Tsukamura H, Maeda K, et al. Neurokinin B and dynorphin A in kisspeptin neurons of the arcuate nucleus participate in generation of periodic oscillation of neural activity driving pulsatile gonadotropin-releasing hormone secretion in the goat. J Neurosci. 2010;30:3124–32.
Zhang JY, Gong N, Huang JL, Guo LC, Wang YX. Gelsemine, a principal alkaloid from Gelsemium sempervirens Ait., exhibits potent and specific antinociception in chronic pain by acting at spinal alpha 3 glycine receptors. Pain. 2013;154:2452–62.
Gong N, Xiao Q, Zhu B, Zhang CY, Wang YC, Fan H, Ma AN, Wang YX. Activation of spinal glucagon-like peptide-1 receptors specifically suppresses pain hypersensitivity. J Neurosci. 2014;34:5322–34.
Leitl MD, Onvani S, Bowers MS, Cheng KJ, Rice KC, Carlezon WA, Banks ML, Negus S. Pain-related depression of the mesolimbic dopamine system in rats: expression, blockade by analgesics, and role of endogenous kappa-opioids. Neuropsychopharmacology. 2014;39:614–24.
Fan H, Gong N, Li TF, Ma AN, Wu XY, Wang MW, Wang YX. The non-peptide GLP-1 receptor agonist WB4-24 blocks inflammatory nociception by stimulating beta-endorphin release from spinal microglia. Br J Pharmacol. 2015;172:64–79.
Fan H, Li TF, Gong N, Wang YX. Shanzhiside methylester, the principle effective iridoid glycoside from the analgesic herb Lamiophlomis rotata, reduces neuropathic pain by stimulatine spinal microglia beta-endorphin expression. Neuropharmacology. 2016;101:98–109.
Nutile-McMenemy N, Elfenbein A, Deleo JA. Minocycline decreases in vitro microglial motility, beta1-integrin, and Kv1.3 channel expression. J Neurochem. 2007;103:2035–46.
Wang AL, Yu AC, Lau LT, Lee C, le Wu M, Zhu X, Tso MO. Minocycline inhibits LPS-induced retinal microglia activation. Neurochem Int. 2005;47:152–8.
Kim SH, Chung JM. An experimental model for peripheral neuropathy produced by segmental spinal nerve ligation in the rat. Pain. 1992;50:355–63.
Butler SH, Godefroy F, Besson JM, Weil-Fugazza J. A limited arthritic model for chronic pain studies in the rat. Pain. 1992;48:73–81.
Courteix C, Eschalier A, Lavarenne J. Streptozocin-induced diabetic rats: behavioural evidence for a model of chronic pain. Pain. 1993;53:81–8.
Huang JL, Chen XL, Guo C, Wang YX. Contributions of spinal D-amino acid oxidase to bone cancer pain. Amino Acids. 2012;43:1905–18.
Mei XP, Xu H, Xie C, Ren J, Zhou Y, Zhang H, Xu LX. Post-injury administration of minocycline: an effective treatment for nerve-injury induced neuropathic pain. Neurosci Res. 2011;70:305–12.
Hua XY, Svensson CI, Matsui T, Fitzsimmons B, Yaksh TL, Webb M. Intrathecal minocycline attenuates peripheral inflammation-induced hyperalgesia by inhibiting p38 MAPK in spinal microglia. Eur J Neurosci. 2005;22:2431–40.
Ju J, Shin DJ, Na YC, Yoon MH. Role of spinal opioid receptor on the antiallodynic effect of intrathecal nociceptin in neuropathic rat. Neurosci Lett. 2013;542:118–22.
Bowersox SS, Gadbois T, Singh T, Pettus M, Wang YX, Luther RR. Selective N-type neuronal voltage-sensitive calcium channel blocker, SNX-111, produces spinal antinociception in rat models of acute, persistent and neuropathic pain. J Pharmacol Exp Ther. 1996;279:1243–9.
Wang YX, Gao D, Pettus M, Phillips C, Bowersox SS. Interactions of intrathecally administered ziconotide, a selective blocker of neuronal N-type voltage-sensitive calcium channels, with morphine on nociception in rats. Pain. 2000;84:271–81.
Huang Q, Chen Y, Gong N, Wang YX. Methylglyoxal mediates streptozocin-induced diabetic neuropathic pain via activation of the peripheral TRPA1 and Nav1.8 channels. Metabolism. 2016;65:463–74.
Raghavendra V, Tanga F, DeLeo JA. Inhibition of microglial activation attenuates the development but not existing hypersensitivity in a rat model of neuropathy. J Pharmacol Exp Ther. 2003;306:624–30.
Tikka T, Fiebich BL, Goldsteins G, Keinanen R, Koistinaho J. Minocycline, a tetracycline derivative, is neuroprotective against excitotoxicity by inhibiting activation and proliferation of microglia. J Neurosci. 2001;21:2580–8.
Weihe E, Millan MJ, Hollt V, Nohr D, Herz A. Induction of the gene encoding pro-dynorphin by experimentally induced arthritis enhances staining for dynorphin in the spinal cord of rats. Neuroscience. 1989;31:77–95.
Wahlert A, Funkelstein L, Fitzsimmons B, Yaksh T, Hook V. Spinal astrocytes produce and secrete dynorphin neuropeptides. Neuropeptides. 2013;47:109–15.
Marvizon JC, Chen W, Murphy N. Enkephalins, dynorphins, and beta-endorphin in the rat dorsal horn: an immunofluorescence colocalization study. J Comp Neurol. 2009;517:51–68.
Ledeboer A, Sloane EM, Milligan ED, Frank MG, Mahony JH, Maier SF, Watkins LR. Minocycline attenuates mechanical allodynia and proinflammatory cytokine expression in rat models of pain facilitation. Pain. 2005;115:71–83.
Lin CS, Tsaur ML, Chen CC, Wang TY, Lin CF, Lai YL, Hsu TC, Pan YY, Yang CH, Cheng JK. Chronic intrathecal infusion of minocycline prevents the development of spinal-nerve ligation-induced pain in rats. Reg Anesth Pain Med. 2007;32:209–16.
Padi SS, Kulkarni SK. Minocycline prevents the development of neuropathic pain, but not acute pain: possible anti-inflammatory and antioxidant mechanisms. Eur J Pharmacol. 2008;601:79–87.
Zhang X, Xu Y, Wang J, Zhou Q, Pu S, Jiang W, Du D. The effect of intrathecal administration of glial activation inhibitors on dorsal horn BDNF overexpression and hind paw mechanical allodynia in spinal nerve ligated rats. J Neural Transm (Vienna). 2012;119:329–36.
Liu NJ, Schnell S, Wessendorf MW, Gintzler AR. Sex, pain, and opioids: interdependent influences of sex and pain modality on dynorphin-mediated antinociception in rats. J Pharmacol Exp Ther. 2013;344:522–30.
Rojewska E, Makuch W, Przewlocka B, Mika J. Minocycline prevents dynorphin-induced neurotoxicity during neuropathic pain in rats. Neuropharmacology. 2014;86:301–10.
Obara I, Mika J, Schafer MKH, Przewlocka B. Antagonists of the kappa-opioid receptor enhance allodynia in rats and mice after sciatic nerve ligation. Br J Pharmacol. 2003;140:538–46.
Wang ZJ, Gardell LR, Ossipov MH, Vanderah TW, Brennan MB, Hochgeschwender U, Hruby VJ, Malan TP, Lai J, Porreca F. Pronociceptive actions of dynorphin maintain chronic neuropathic pain. J Neurosci. 2001;21:1779–86.
Schwei MJ, Honore P, Rogers SD, Salak-Johnson JL, Finke MP, Ramnaraine ML, Clohisy DR, Mantyh PW. Neurochemical and cellular reorganization of the spinal cord in a murine model of bone cancer pain. J Neurosci. 1999;19:10886–97.
Nahin RL, Hylden JL, Iadarola MJ, Dubner R. Peripheral inflammation is associated with increased dynorphin immunoreactivity in both projection and local circuit neurons in the superficial dorsal horn of the rat lumbar spinal cord. Neurosci Lett. 1989;96:247–52.
Abbruscato TJ, Thomas SA, Hruby VJ, Davis TP. Blood-brain barrier permeability and bioavailability of a highly potent and mu-selective opioid receptor antagonist, CTAP: comparison with morphine. J Pharmacol Exp Ther. 1997;280:402–9.
Jones RM, Portoghese PS. 5′-Guanidinonaltrindole, a highly selective and potent kappa-opioid receptor antagonist. Eur J Pharmacol. 2000;396:49–52.
Ossipov MH, Kovelowski CJ, Vanderah T, Porreca F. Naltrindole, an opioid delta antagonist, blocks the enhancement of morphine-antinociception induced by a CCKB antagonist in the rat. Neurosci Lett. 1994;181:9–12.
Liu RY, Huang XP, Yeliseev A, Xi J, Roth BL. Novel molecular targets of dezocine and their clinical implications. Anesthesiology. 2014;120:714–23.
Zhang H, Shi YG, Woods JH, Watson SJ, Ko MC. Central kappa-opioid receptor-mediated antidepressant-like effects of nor-Binaltorphimine: behavioral and BDNF mRNA expression studies. Eur J Pharmacol. 2007;570:89–96.
Jha MK, Jeon S, Suk K. Glia as a link between neuroinflammation and neuropathic pain. Immune Netw. 2012;12:41–7.
Watkins LR, Milligan ED, Maier SF. Glial activation: a driving force for pathological pain. Trends Neurosci. 2001;24:450–5.
Yoon SY, Patel D, Dougherty PM. Minocycline blocks lipopolysaccharide induced hyperalgesia by suppression of microglia but not astrocytes. Neuroscience. 2012;221:214–24.
Wu DC, Jackson-Lewis V, Vila M, Tieu K, Teismann P, Vadseth C, Choi DK, Ischiropoulos H, Przedborski S. Blockade of microglial activation is neuroprotective in the 1-methyl-4-phenyl-1,2,3,6-tetrahydropyridine mouse model of Parkinson disease. J Neurosci. 2002;22:1763–71.
Zhang SC, Goetz BD, Duncan ID. Suppression of activated microglia promotes survival and function of transplanted oligodendroglial progenitors. Glia. 2003;41:191–8.
Huang WC, Qiao Y, Xu L, Kacimi R, Sun X, Giffard RG, Yenari MA. Direct protection of cultured neurons from ischemia-like injury by minocycline. Anat Cell Biol. 2010;43:325–31.
Wilkins A, Nikodemova M, Compston A, Duncan I. Minocycline attenuates nitric oxide-mediated neuronal and axonal destruction in vitro. Neuron Glia Biol. 2004;1:297–305.
Yrjanheikki J, Tikka T, Keinanen R, Goldsteins G, Chan PH, Koistinaho J. A tetracycline derivative, minocycline, reduces inflammation and protects against focal cerebral ischemia with a wide therapeutic window. Proc Natl Acad Sci U S A. 1999;96:13496–500.
Sanchez Mejia RO, Ona VO, Li M, Friedlander RM. Minocycline reduces traumatic brain injury-mediated caspase-1 activation, tissue damage, and neurological dysfunction. Neurosurgery. 2001;48:1393–9. discussion 9-401.
Khachaturian H, Watson SJ, Lewis ME, Coy D, Goldstein A, Akil H. Dynorphin immunocytochemistry in the rat central nervous system. Peptides. 1982;3:941–54.
Smith AP, Lee NM. Pharmacology of dynorphin. Annu Rev Pharmacol Toxicol. 1988;28:123–40.
Mollereau C, Mouledous L, Lapalu S, Cambois G, Moisand C, Butour JL, Meunier JC. Distinct mechanisms for activation of the opioid receptor-like 1 and kappa-opioid receptors by nociceptin and dynorphin A. Mol Pharmacol. 1999;55:324–31.
Noguchi K, Kowalski K, Traub R, Solodkin A, Iadarola MJ, Ruda MA. Dynorphin expression and Fos-like immunoreactivity following inflammation induced hyperalgesia are colocalized in spinal cord neurons. Brain Res Mol Brain Res. 1991;10:227–33.
Minokadeh A, Funkelstein L, Toneff T, Hwang SR, Beinfeld M, Reinheckel T, Peters C, Zadina J, Hook V. Cathepsin L participates in dynorphin production in brain cortex, illustrated by protease gene knockout and expression. Mol Cell Neurosci. 2010;43:98–107.
Stevens CW, Yaksh TL. Dynorphin A and related peptides administered intrathecally in the rat: a search for putative kappa opiate receptor activity. J Pharmacol Exp Ther. 1986;238:833–8.
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.
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.
Bakshi R, Faden AI. Competitive and non-competitive NMDA antagonists limit dynorphin A-induced rat hindlimb paralysis. Brain Res. 1990;507:1–5.
Tsuda M, Mizokoshi A, Shigemoto-Mogami Y, Koizumi S, Inoue K. Activation of p38 mitogen-activated protein kinase in spinal hyperactive microglia contributes to pain hypersensitivity following peripheral nerve injury. Glia. 2004;45:89–95.
Ji RR, Suter MR. p38 MAPK, microglial signaling, and neuropathic pain. Mol Pain. 2007;3:33.
Pyo H, Joe E, Jung S, Lee SH, Jou I. Gangliosides activate cultured rat brain microglia. J Biol Chem. 1999;274:34584–9.
Pyo H, Jou I, Jung S, Hong S, Joe EH. Mitogen-activated protein kinases activated by lipopolysaccharide and beta-amyloid in cultured rat microglia. Neuroreport. 1998;9:871–4.
Won KA, Kang YM, Lee MK, Park MK, Ju JS, Bae YC, Ahn DK. Participation of microglial p38 MAPK in formalin-induced temporomandibular joint nociception in rats. J Orofac Pain. 2012;26:132–41.
Cho IH, Lee MJ, Jang M, Gwak NG, Lee KY, Jung HS. Minocycline markedly reduces acute visceral nociception via inhibiting neuronal ERK phosphorylation. Mol Pain. 2012;8:13.
Song X, Xu A, Pan W, Wallin B, Kivlin R, Lu S, Cao C, Bi Z, Wan Y. Minocycline protects melanocytes against H2O2-induced cell death via JNK and p38 MAPK pathways. Int J Mol Med. 2008;22:9–16.
Nikodemova M, Duncan ID, Watters JJ. Minocycline exerts inhibitory effects on multiple mitogen-activated protein kinases and IkappaBalpha degradation in a stimulus-specific manner in microglia. J Neurochem. 2006;96:314–23.
Tikka TM, Koistinaho JE. Minocycline provides neuroprotection against N-methyl-D-aspartate neurotoxicity by inhibiting microglia. J Immunol. 2001;166:7527–33.
Cai CQ, Yang CH, Liang JY, Liu JH. Advance in studies on structure-activity relationships of diterpenoid alkaloids in genus Aconitum. Strait Pharma J. 2013;25:1–5.
Wu ZJ, Yang CH, Ye WC, Liu JH. Advances in the studies on the pharmacological activities of C20 diterpenoid alkaloids. Prog Pharma Sci. 2011;35:241–9.
The authors would like to thank Dr. Lei-Ming Ren at Herbei Medical University for his constructive discussion initiating the project.
This study was supported by the National Natural Science Foundation of China (No. 81673403).
Availability of data and materials
Data supporting the conclusions of this article are presented in the manuscript.
YXW and QH conceived and designed the experiments; QH, XFM, HYW, TFL, MLS, and HL performed the experiments; QH, XFM, and YXW analyzed the data; and YXW and QH wrote the paper. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
Consent for publication
All animal procedures performed in this study were reviewed and approved by the Animal Care and Welfare Committee of Shanghai Jiao Tong University and carried out in accordance with the animal care guidelines of the National Institutes of Health.
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Huang, Q., Mao, X., Wu, H. et al. Bullatine A stimulates spinal microglial dynorphin A expression to produce anti-hypersensitivity in a variety of rat pain models. J Neuroinflammation 13, 214 (2016) doi:10.1186/s12974-016-0696-2
- Bullatine A
- Spinal cord
- Dynorphin A
- Pro-inflammatory cytokines