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Pain Medicine  |   June 2011
A Peripheral Adrenoceptor-mediated Sympathetic Mechanism Can Transform Stress-induced Analgesia into Hyperalgesia
Author Affiliations & Notes
  • John E. Donello, Ph.D.
    *
  • Yun Guan, M.D., Ph.D.
  • Mingting Tian, M.S.
  • Cynthia V. Cheevers, B.S.
  • Miguel Alcantara, B.S.
  • Sara Cabrera, M.S.
  • Srinivasa N. Raja, M.D.
    §
  • Daniel W. Gil, Ph.D.
  • * Senior Research Investigator, Department of Biological Sciences, Allergan, Inc., Irvine, California. † Assistant Professor, Department of Anesthesiology/CCM, Johns Hopkins University, Baltimore, Maryland. ‡ Scientist, Department of Biological Sciences, Allergan, Inc. § Professor, Department of Anesthesiology/CCM, Johns Hopkins University. ∥ Vice President, BioScience, Department of Biological Sciences, Allergan, Inc.
Article Information
Pain Medicine / Central and Peripheral Nervous Systems / Pain Medicine
Pain Medicine   |   June 2011
A Peripheral Adrenoceptor-mediated Sympathetic Mechanism Can Transform Stress-induced Analgesia into Hyperalgesia
Anesthesiology 6 2011, Vol.114, 1403-1416. doi:10.1097/ALN.0b013e31821c3878
Anesthesiology 6 2011, Vol.114, 1403-1416. doi:10.1097/ALN.0b013e31821c3878
What We Already Know about This Topic
  • Stress exacerbates chronic pain in patients; however, the mechanisms for exacerbation of pain by stress are not understood

  • In most preclinical animal models of pain, stress produces analgesia and not hyperalgesia

What This Article Tells Us That Is New
  • When the activity of the sympathetic nervous system was enhanced, stressors worsened pain behaviors through a peripheral α-1 adrenergic receptor

ADRENERGIC neurotransmission is an integral part of the pain and stress response pathways. Studies have demonstrated that hyperalgesia is often associated with enhanced adrenergic sensitivity of primary afferents. Sensory nerves in animals become sensitive to sympathetic nerve stimulation or exogenous addition of the sympathetic adrenergic neurotransmitter, norepinephrine, after nerve injury or in the presence of inflammatory mediators.1–5 Potential mechanisms for the increased primary afferent adrenergic sensitivity include up-regulation of α-2-adrenergic receptors6 and exacerbation of neurogenic inflammation by α-1-adrenergic receptors.7 Some of these mechanisms may occur in posttraumatic neuralgias, such as causalgia, which are sometimes diagnosed or treated with α-adrenergic blockade.8,9 
Adrenergic mechanisms are also involved in the various ways that stress modulates the perception of pain. A classic effect of a variety of acute stressors in humans and in animal models is stress-induced analgesia, which is mediated by descending spinal pathways.10,11 Both opioid and nonopioid mechanisms, which differ with respect to naloxone sensitivity and cross-tolerance with morphine, have been described. Nonopioid descending inhibition of dorsal horn nociceptive transmission is in part mediated by α-2-adrenergic receptors.12 Conversely, pain disorders such as fibromyalgia, irritable bowel syndrome, and migraine headaches can be triggered or exacerbated by stress, particularly chronic stress, in ways that are not well understood. It was recently shown that chronic stress in rats results in increased primary afferent sensitivity to the sympathoadrenal adrenergic molecule, epinephrine, as a result of changes in β-2-adrenergic receptor signaling.13 
The physiologic response to stress is also mediated through sympathoneural outflow of norepinephrine. The sympathetic nervous system (SNS) is not thought to activate primary afferents in the absence of injury. Clinical studies in normal subjects have demonstrated that stimulation of sympathetic activity by physiologic stimuli9 does not cause pain or increase the response of nociceptive sensory neurons to a painful stimulus. This is likely because norepinephrine release is under tight control by α-2A- and α-2C-adrenergic receptors. These α-2 receptors are located on postsynaptic sympathetic nerve endings,14 where they mediate feedback inhibition of norepinephrine release on peripheral terminals of sensory neurons.15 The α-2 receptors are also located in the spinal cord dorsal horn16 and in brain regions associated with pain modulation including the hypothalamus and amygdala.17–19 
The α-2A knockout mice have been described previously with increased SNS outflow during high-frequency stimulation, because of the loss of feedback autoinhibition.14 Despite the absence of functional α-2A adrenoceptors in pathways that modulate pain transmission in mice expressing the D79N α-2A receptor mutation, the mice have normal sensitivity to acute noxious thermal stimuli in a temperature ramp hotplate test20 and in tail immersion tests.21,22 On the other hand, α-2A knockout mice have enhanced referred pain after capsaicin treatment,23 providing evidence of a role of α-2A-adrenergic receptors in attenuating the neuronal response to a sustained noxious stimulus.
Because SNS outflow is stimulated by stress, we hypothesized that loss of α-2A-adrenergic receptor activity, because of pharmacologic blockade or genetic ablation, would reveal SNS facilitation of pain pathways following exposure to stress. Ultrasonic noise was selected as a noninvasive psychologic stressor that involves activation of limbic pathways and the sympathoadrenal axis.24,25 Levine and coworkers have shown that 30 min of intermittent noise stress increases plasma corticosterone in rats. This stress response does not habituate and results in enhancement of bradykinin hyperalgesia over several days.25,26 Periods of acute, continuous noise as short as 5-min durations have been demonstrated to result in analgesia that does not habituate and is opioid-independent.27 
We find that rats and C57/BL6 wild-type (WT) mice develop stress-induced hyperalgesia when they are pretreated systemically with α-2 receptor antagonists. Stress-induced hyperalgesia was also observed in α-2 antagonist–pretreated rats exposed to a classic physical stressor, footshock, under conditions that normally result in nonopioid analgesia.28 The C57/BL6 α-2A knockout mice, in the absence of receptor antagonists, also develop stress-induced hyperalgesia in response to noise stress. Further examination suggests that loss of peripheral α-2 receptor autoinhibition can counterbalance spinal stress-induced analgesia and, in the absence of sufficient descending inhibition, can lead to the development of stress-induced hyperalgesia. The pain facilitatory mechanism is dependent on intact peripheral sympathetic innervation and could potentially be caused by an overflow of norepinephrine within the hyperalgesic location.
Materials and Methods
Animals
The α-2 knockout mice were backcrossed onto a C57BL/6 background and bred from homozygous knockout mice breeding pairs. Age- and sex-matched WT C57BL/6 mice (Charles River, Wilmington, MA) were used as a control group. For confirmatory purposes, additional animals were bred by heterozygote crossing to generate α-2A knockout mice and littermate control groups. The hotplate paw withdrawal responses of these animals with and without stress were shown to be the same as those of the independently bred knockout mice and control groups (data not shown). Mice were 3–5 months old and weighed 20–30 g. Sprague-Dawley rats (Charles River) weighed 250–350 g. Animals received food and water ad libitum  and were kept on a 12-h day-night cycle. All experiments were done in compliance with protocols approved by Allergan, Inc. (Irvine, CA) or The Johns Hopkins University (Baltimore, Maryland) Institutional Animal Care and Use Committees and are consistent with the National Institutes of Health Guide for the Use of Experimental Animals to minimize animal use and discomfort.
Drugs
Drug solutions were prepared as follows: Prazosin (Sigma Chemical Co., St. Louis, MO) and guanethidine (Sigma Chemical Co.) were dissolved in saline, sulprostone (Cayman Chemical, Ann Arbor, MI) and N  -methyl-d-aspartate (NMDA; Sigma Chemical Co.) were dissolved in dimethylsulfoxide, and stock solutions of rauwolscine (Sigma Chemical Co.) and idazoxan (Sigma Chemical Co.) were dissolved with dimethylsulfoxide and subsequently diluted with saline (final concentration of dimethylsulfoxide was less than 1%) for injection.
Intrathecal injections in mice were performed according to the method devised by Hylden and Wilcox.29 A sterile 30-gauge ½-inch needle attached to a microsyringe was inserted between the L5 and L6 vertebrae and a 5-μl volume slowly injected in the subarachnoid space. Intraperitoneal injections were administered in a volume of 1 ml/kg. Intraplantar rauwolscine was injected in a 25-μl volume.
Tactile Allodynia Assessment
Sensitivity to light touch was quantified according to methods published by Gil et al.  30 Briefly, mice were acclimated to brushing of the hind flank with a paintbrush for the first 15 min following intraperitoneal injection of sulprostone or intrathecal injection of NMDA. Starting at 15-min postinjection, the behavioral response to light brushing of the hind flank was scored every 5 min for the time period 15–50 min postinjection. The behavioral response was scored as follows: animals showing aggressive escape responses along with squeaking and biting at the brush are given a score of 2; animals exhibiting mild squeaking with attempts to escape are given a score of 1; animals showing no response to the light stroking of the paintbrush are given a score of 0. The eight timepoint scores were summed for each animal to generate that animal's cumulative pain score (maximum pain score of 16).30 An average of the individual cumulative pain scores was then determined for each treatment group.
Thermal Latency Assessment
To determine thermal withdrawal latencies (in seconds), rats or mice were individually placed on the hotplate surface preset to 50°C. A timer was started immediately and stopped when the animal first lifted and/or licked either hind paw. The maximum withdrawal latency was 20 s, at which time the animals were removed to prevent tissue damage. In experiments with a unilateral intraplantar injection of rauwolscine, the withdrawal latency of each limb (contralateral and ipsilateral) was individually assessed in separate experiments. In chemical sensitization studies in mice, the withdrawal latencies were assessed 30 min following sulprostone or NMDA treatment.
Ultrasonic Noise Stress
The noise-induced stress experiments were conducted in an isolated room. The ultrasonic sound emitters (Ultrasonic Pest Repeller; Weitech, Wavre, Belgium) were attached to the top of each cage and confirmed to produce a 24–75 KHz, 100–105 dB noise at the relevant distance with an ultrasonic probe (UE Systems, Elmsford, NY). Twenty-four h before the initiation of a noise-induced stress experiment, animals were transferred into the test room. The animals were singly caged, and food, water, and 12-h light-dark cycle were unchanged. Intraperitoneal injections of rauwolscine, idazoxan, prazosin, or saline were administered 30 min before stress. Intraplantar and intrathecal injections were administered immediately before stress. The sound was initiated remotely for a 10-min period. Hotplate testing was performed in the same room within 5 min. Each animal was tested on the hotplate only once. The experimenter was blinded to the stress status, genotype, and drug treatment of animals for studies comparing rauwolscine and saline-treated rats (fig. 1), C57BL/6 and α-2A knockout mice (fig. 2A), and sympathectomized and sham rats.
Fig. 1.  Stress-induced hyperalgesia resulting from systemic α-2-adrenergic blockade in rats and wild-type (WT) mice. (A  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in Sprague-Dawley (SD) rats treated with intraperitoneal (IP) saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 6). (B  ) Paw withdrawal latencies after no stress (red bars  ) or footshock stress (blue bars  ) in Sprague-Dawley rats treated with IP saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 12). (C  and D  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in C57BL/6 WT mice treated with IP saline (n = 6) or the α-2-adrenergic receptor antagonists (C  ) 0.1 mg/kg−1rauwolscine (n = 6) or (D  ) 0.03 mg/kg−1idazoxan (n = 6). (E  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in Sprague-Dawley rats treated with intrathecal (IT) saline (n = 6) or 3 μg rauwolscine (n = 6). The antagonists transform stress-induced analgesia into stress-induced hyperalgesia when dosed intraperitoneally and block stress-induced analgesia without inducing hyperalgesia when dosed intrathecally. **=P  < 0.01; ***=P  < 0.001, increase in latency versus  no stress (analgesia); +=P  < 0.05; ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no stress (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 1. 
	Stress-induced hyperalgesia resulting from systemic α-2-adrenergic blockade in rats and wild-type (WT) mice. (A 
	) Paw withdrawal latencies after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in Sprague-Dawley (SD) rats treated with intraperitoneal (IP) saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 6). (B 
	) Paw withdrawal latencies after no stress (red bars 
	) or footshock stress (blue bars 
	) in Sprague-Dawley rats treated with IP saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 12). (C 
	and D 
	) Paw withdrawal latencies after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in C57BL/6 WT mice treated with IP saline (n = 6) or the α-2-adrenergic receptor antagonists (C 
	) 0.1 mg/kg−1rauwolscine (n = 6) or (D 
	) 0.03 mg/kg−1idazoxan (n = 6). (E 
	) Paw withdrawal latencies after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in Sprague-Dawley rats treated with intrathecal (IT) saline (n = 6) or 3 μg rauwolscine (n = 6). The antagonists transform stress-induced analgesia into stress-induced hyperalgesia when dosed intraperitoneally and block stress-induced analgesia without inducing hyperalgesia when dosed intrathecally. **=P 
	< 0.01; ***=P 
	< 0.001, increase in latency versus 
	no stress (analgesia); +=P 
	< 0.05; ++=P 
	< 0.01; +++=P 
	< 0.001, decrease in latency versus 
	no stress (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 1.  Stress-induced hyperalgesia resulting from systemic α-2-adrenergic blockade in rats and wild-type (WT) mice. (A  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in Sprague-Dawley (SD) rats treated with intraperitoneal (IP) saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 6). (B  ) Paw withdrawal latencies after no stress (red bars  ) or footshock stress (blue bars  ) in Sprague-Dawley rats treated with IP saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 12). (C  and D  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in C57BL/6 WT mice treated with IP saline (n = 6) or the α-2-adrenergic receptor antagonists (C  ) 0.1 mg/kg−1rauwolscine (n = 6) or (D  ) 0.03 mg/kg−1idazoxan (n = 6). (E  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in Sprague-Dawley rats treated with intrathecal (IT) saline (n = 6) or 3 μg rauwolscine (n = 6). The antagonists transform stress-induced analgesia into stress-induced hyperalgesia when dosed intraperitoneally and block stress-induced analgesia without inducing hyperalgesia when dosed intrathecally. **=P  < 0.01; ***=P  < 0.001, increase in latency versus  no stress (analgesia); +=P  < 0.05; ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no stress (hyperalgesia). Data are expressed as mean ± SEM.
×
Fig. 2.  Stress-induced hyperalgesia in α-2A knockout (KO) mice. (A  ) Paw withdrawal latencies from a 50°C hotplate in wild-type (WT) and α-2A KO mice after no stress (red bars  , n = 6) or ultrasonic stress (blue bars  , n = 12). (B  ) Paw withdrawal latencies in WT mice (n = 11) and α-2A KO mice (n = 5) tested once on a hotplate at various times after the initiation of 10-min ultrasonic stress. (C  ) Paw withdrawal latencies in α-2A KO mice after no stress (red bars  , n = 6) or ultrasonic stress (blue bars  , n = 6) on 3 consecutive days. The α-2A KO mice exhibit a prolonged nonhabituating hyperalgesia instead of analgesia in response to ultrasonic stress. *=P  < 0.05; ***=P  < 0.001, increase in latency versus  no stress (analgesia); +=P  < 0.05; +++=P  < 0.001, decrease in latency versus  no stress (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 2. 
	Stress-induced hyperalgesia in α-2A knockout (KO) mice. (A 
	) Paw withdrawal latencies from a 50°C hotplate in wild-type (WT) and α-2A KO mice after no stress (red bars 
	, n = 6) or ultrasonic stress (blue bars 
	, n = 12). (B 
	) Paw withdrawal latencies in WT mice (n = 11) and α-2A KO mice (n = 5) tested once on a hotplate at various times after the initiation of 10-min ultrasonic stress. (C 
	) Paw withdrawal latencies in α-2A KO mice after no stress (red bars 
	, n = 6) or ultrasonic stress (blue bars 
	, n = 6) on 3 consecutive days. The α-2A KO mice exhibit a prolonged nonhabituating hyperalgesia instead of analgesia in response to ultrasonic stress. *=P 
	< 0.05; ***=P 
	< 0.001, increase in latency versus 
	no stress (analgesia); +=P 
	< 0.05; +++=P 
	< 0.001, decrease in latency versus 
	no stress (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 2.  Stress-induced hyperalgesia in α-2A knockout (KO) mice. (A  ) Paw withdrawal latencies from a 50°C hotplate in wild-type (WT) and α-2A KO mice after no stress (red bars  , n = 6) or ultrasonic stress (blue bars  , n = 12). (B  ) Paw withdrawal latencies in WT mice (n = 11) and α-2A KO mice (n = 5) tested once on a hotplate at various times after the initiation of 10-min ultrasonic stress. (C  ) Paw withdrawal latencies in α-2A KO mice after no stress (red bars  , n = 6) or ultrasonic stress (blue bars  , n = 6) on 3 consecutive days. The α-2A KO mice exhibit a prolonged nonhabituating hyperalgesia instead of analgesia in response to ultrasonic stress. *=P  < 0.05; ***=P  < 0.001, increase in latency versus  no stress (analgesia); +=P  < 0.05; +++=P  < 0.001, decrease in latency versus  no stress (hyperalgesia). Data are expressed as mean ± SEM.
×
Footshock Stress
Rats were singly exposed to 3 min of continuous 60 Hz electric shock applied at an intensity of 3 mA through the floor of a Gemini Passive Avoidance apparatus (San Diego Instruments, San Diego, CA). Unstressed rats were placed in the apparatus without shock for 3 min. An experimenter, masked to stress condition and drug treatment, determined thermal latencies 7 min later.
Surgical Sympathectomy
Lumbar sympathectomy was performed in male Sprague-Dawley rats under isoflurane anesthesia. The lumbar sympathetic chain was exposed by a ventrolateral, retroperitoneal approach. A shallow midline incision was made to separate the skin from the muscle beginning at the level of L2 and terminating at the level of L6. A second midline incision was made through the muscle, ensuring no damage to the liver and intestines. The superficial muscle layers were then retracted, separating the psoas and the quadratus lumborum muscles from the vertebral column and the transverse processes. The sympathetic paravertebral ganglia L2–L6 were removed bilaterally, beginning from the level of the crus of the diaphragm to the most distal ganglion approachable. Pseudosham sympathectomy was identical to lumbar sympathectomy except for removal of the sympathetic paravertebral ganglia. The sympathectomy was functionally confirmed by demonstrating a lack of cold-induced vasoconstriction in the hind paws (data not shown).
Assay of Plasma Corticosterone
Plasma samples were taken from mice after 10 min of ultrasonic stress, and plasma corticosterone level was measured using an immunoassay kit (R&D Systems, Minneapolis, MN).
Electrophysiologic Study
Surgery.
Surgical preparation for neurophysiologic recording was conducted as described previously.31 Urethane was used (1.5–2.0 g/kg−1intraperitoneally) to ensure deep anesthesia in mice during surgery and neurophysiologic recording,32,33 because the potential involvement of α-2A adrenoceptors in isoflurane-induced analgesia may compromise the analgesia and data interpretation in α-2A knockout mice.34,35 Areflexia to sensory stimuli and electrocardiogram was monitored to ensure sufficient depth of anesthesia. Mice were paralyzed with pancuronium bromide (0.15 mg/kg−1intraperitoneally; Elkins-Sinn Inc., Cherry Hill, NJ) during neurophysiologic recording. A laminectomy was performed at vertebral levels T12–L1 to expose lumbar enlargement (L3–L6 spinal segments). The recording segments were continually bathed in a pool of warm saline (37°C) after the dura mater was incised and retracted. Core body temperature was maintained at 36.0–37.0°C with a circulating hot-water pad. A small animal ventilator (Model 683; Harvard Apparatus, South Natick, MA) provided mechanical ventilation (120–140 cycles/min−1, stroke volume 0.2–0.3 ml). Mice were euthanized at the conclusion of each experiment by an overdose of sodium pentobarbital (300 mg/kg−1intraperitoneally).
Dorsal Horn Neuron Recording.
Extracellular recordings of single neuronal activity in the lumbar-dorsal horn (segment L4–L5) were obtained by using fine-tip (less than 1.0 μm) tungsten microelectrodes (8 mΩ at 1 kHz; Frederick Haer & Co., Brunswick, ME) that were advanced using an electronic micropositioner. A real-time, computer-based data acquisition and processing system (DAPSYS 6; Brian Turnquist, Ph.D., Johns Hopkins University, Baltimore, Maryland) provided window discriminators for real-time sorting of the amplified action potential (AP) waveforms. Mechanical stimuli were used to search for dorsal horn neurons with cutaneous receptive fields located in the central plantar area of the hind paw. Deep wide dynamic range (WDR) cells (300–700 μm) that respond to both innocuous and noxious mechanical stimuli were defined as described previously.31,36,37 Electrical stimulus was applied through a pair of fine needles inserted subcutaneously across the central plantar area of the hind paw at 0.3–0.4 cm apart. Based on the axon conduction velocities, WDR neurons showed both A-fiber (0–40 ms) and C-fiber (40–250 ms)–mediated response to single intracutaneous electrical stimulus at intensity above the C-fiber activation threshold.31,38 The stimulus intensity-response functions of A- and C-fiber–mediated responses were determined by application of graded intracutaneous electrical stimuli (0.05–5.0 mA, 2.0 ms). The intensity that evoked at least one spike within the A-fiber and C-fiber latency range was considered the A-fiber and C-fiber threshold, respectively. The responses evoked by A- and C-fibers were quantified by separating the AP firing on a latency basis. WDR neurons were further assessed for their ability to show AP windup response to repeated intracutaneous electrical stimuli that are suprathreshold for C-fiber activation. Three stimulus trains (16 pulses, 3.0 mA, 2.0 ms) were applied at 0.2 Hz, 0.5 Hz, and 1.0 Hz, and with a 10-min interval between each trial. The experimenter was blinded to the treatment of mice in the prazosin studies.
Statistical Analysis
Data are presented as mean ± SEM. A P  value less than 0.05 was considered significant in all studies. In behavioral studies, single comparisons between stressed and unstressed groups were done by independent samples two-tailed Student t  tests using Microsoft Excel 2007. GraphPad Prism 5.0 software (GraphPad Software, Inc., La Jolla, CA) was used for multiple comparisons. In the time course study for figure 2B, the responses at each timepoint were compared with baseline using a one-way ANOVA with a Dunnett multiple comparison test. In the repeated stress study for figure 2C, the responses of stressed and unstressed groups on each day were compared by a two-way ANOVA with a post hoc  Bonferroni correction. The F value, a ratio of the variance between groups to the variance within groups, is reported as F(df  between, df  (between+within)) = X, where df  = degrees of freedom. For sulprostone and NMDA dose-response curves, one-way ANOVA with a Dunnett multiple comparison test was used to compare each concentration to vehicle, and two-way ANOVA with a post hoc  Bonferroni correction was used to compare the same drug concentration between genotypes. In electrophysiology studies, STATISTICA 6.0 software (StatSoft, Inc., Tulsa, OK) was used to conduct all statistical analyses. The number of APs evoked by graded electrical stimuli was compared between two genotypes, using a two-way mixed-model ANOVA with Tukey honestly significant difference post hoc  test. An independent sample two-tailed Student t  test was used to compare the recording depth, latency, and threshold for activation of A-fiber and C-fiber–mediated responses, respectively, between the two groups. For analysis of windup, the primary parameter studied was the number of APs in the C-component response evoked by each stimulus in a train of repetitive electrical stimulation. Because the number of APs in the C-component varies among WDR neurons, the raw data for each cell were normalized, with 100% representing the response to the first stimulation in each trial (input). The normalized responses among cells were then averaged. Windup graphs were created by plotting the normalized values against the stimulation number in a train of 16 stimuli. A two-way mixed-model ANOVA (Tukey honestly significant difference post hoc  test) was used to compare windup functions and the averaged C-components for the stimuli 7–16 of the trial, which reflects the plateau level of windup in its maintenance phase, at each frequency tested between the two genotypes.31 A two-way repeated-measures ANOVA (Tukey honestly significant difference post hoc  test) was used to compare electrophysiology data between preprazosin and postprazosin conditions.
Results
Effect of Pharmacologic Blockade of α-2 Receptors on Modulation of Pain by Stress
Intraperitoneal α-2-Adrenergic Antagonists Transform Stress-induced Analgesia to Hyperalgesia.
To test if α-2 receptors influence stress-modulated pain behavior, rats were systemically treated with vehicle or the α-2 antagonist rauwolscine (0.1 mg kg−1intraperitoneally). Thirty minutes postinjection, animals were exposed to either 10 min of normal noise (nonstress group) or ultrasonic noise (stress group). Paw withdrawal thermal latencies to a 50°C hotplate were immediately assessed by an observer masked to treatment condition (fig. 1A). Stressed vehicle-treated rats exhibited increased paw withdrawal latencies (analgesia) in comparison with unstressed animals (14.9 ± 1.5 s stressed vs.  12.6 ± 0.3 s unstressed; P  = 0.15, n = 6/group). Paw withdrawal latencies of unstressed rauwolscine-treated rats were similar to unstressed vehicle-treated animals, suggesting that rauwolscine did not alter normal pain perception. Interestingly, stressed rauwolscine-treated animals had significantly decreased paw withdrawal latencies (hyperalgesia) versus  those of unstressed rauwolscine-treated rats (8.8 ± 0.4 s immediately following ultrasonic stress vs  . 11.9 ± 0.5 s without stress; P  = 0.0016, n = 6/group).
In order to test whether the α-2 antagonist transformation of stress-induced analgesia into stress-induced hyperalgesia is generalizable to other stressors, we tested the effect of systemic rauwolscine treatment (0.1 mg kg−1intraperitoneally) on the thermal pain sensitivity after footshock in rats. Electric footshock is an extensively studied nonhabituating physical stressor.11,28 Depending on the intensity and duration, the footshock results in stress-induced analgesia that is either opioid-dependent or -independent. A 3-min, 3 mA footshock results in opioid-independent analgesia.28 Results similar to ultrasonic noise stress were obtained using this paradigm in a masked study (fig. 1B). Stressed vehicle-treated rats had increased paw withdrawal latencies (analgesia) in comparison with unstressed animals (15.4 ± 1.3 s stressed vs  . 10.8 ± 0.6 s unstressed; P  = 0.0087, n = 6/group). In contrast, stressed rauwolscine-treated rats had significantly decreased paw withdrawal latencies (hyperalgesia) compared with unstressed rauwolscine-treated rats (10.1 ± 0.8 s immediately following footshock stress vs  . 12.2 ± 0.6 s without stress; P  = 0.0442, n = 12/group).
The effect of ultrasonic stress was extended to mice to enable the use of genetic α-2A knockout mice for further mechanistic studies. Exposure of WT mice to a 10-min ultrasonic stress increased plasma corticosterone levels threefold (from 39.2 ± 6.7 to 151.0 ± 30.0 ng/ ml−1; P  = 0.0051, n = 6/group) and produced stress-induced analgesia, consistent with previous studies using noise.27 In a separate experiment, systemic pretreatment (30 min) with α-2 antagonists, either intraperitoneal 0.1 mg/kg−1rauwolscine (fig. 1C) or 0.03 mg/kg−1idazoxan (fig. 1D), decreased paw withdrawal latencies in stressed mice compared with unstressed mice (rauwolscine: 8.4 ± 0.5 s stressed vs  . 12.6 ± 0.4 s without stress, P  = 0.0004, n = 6/group; idazoxan: 8.4 ± 0.3 s stressed versus  12.0 ± 0.6 s without stress, P  = 0.0007, n = 6/group). Without stress, paw withdrawal latencies of antagonist-treated mice were indistinguishable from those of vehicle-treated mice. Vehicle-treated mice (n = 6/group) exhibited normal stress-induced analgesia. The antagonist effect was dose-dependent. A 0.01 mg/kg−1intraperitoneal rauwolscine dose did not decrease stress-prolonged paw withdrawal latencies (17.4 ± 1.0 s with rauwolscine vs  . 17.9 ± 0.9 s with vehicle, n = 6/group) whereas a 0.03 mg/kg−1intraperitoneal dose partially inhibited stress-induced analgesia (14.9 ± 0.8 s, n = 6). The 0.1 mg/kg−1intraperitoneal rauwolscine dose resulted in stress-induced hyperalgesia (8.4 ± 0.5 s). Thus, systemic treatment with α-2 antagonists, which presumably blocks receptor function both peripherally and centrally, causes a loss of stress-induced analgesia and a gain of behavioral hyperalgesia in rats and WT mice. It is unclear if these two behavioral alterations are distinct and separable mechanisms, or simply the net result of a loss of α-2-mediated spinal inhibition.
Intrathecal α-2-Adrenergic Antagonists Block Development of Stress-induced Analgesia.
The role of α-2 receptors in descending inhibition is well established. To test whether the blockade of spinal α-2 receptors is sufficient to transform stress-induced analgesia into stress-induced hyperalgesia, mice were injected intrathecally with vehicle or 3 μg rauwolscine, which is an equivalent total body dose to 0.1 mg/kg−1intraperitoneal treatment in mice weighing approximately 30 g (fig. 1E). Intrathecal vehicle-treated animals exhibited normal thermal paw withdrawal latencies and developed significant stress-induced analgesia (18.2 ± 0.5 s stressed vs  . 12.0 ± 0.6 s without stress; P  < 0.0001, n = 6/group). Paw withdrawal latencies of unstressed rauwolscine-treated mice were similar to those of unstressed vehicle-treated mice. However, paw withdrawal latencies of stressed mice treated with 3 μg intrathecal rauwolscine were not significantly different from those in the unstressed mice (13.1 ± 1.1 s stressed vs  . 11.4 ± 0.6 s unstressed; P  = 0.24, n = 6/group). Lower concentrations of intrathecal rauwolscine (0.3 and 1 μg) did not block stress-induced analgesia (data not shown). Intrathecal rauwolscine blocked the development of stress-induced analgesia but did not result in the development of stress-induced hyperalgesia.
Loss of α-2A Receptor Activity in Knockout Mice Results in Stress-induced Hyperalgesia
Rauwolscine is a highly selective α-2 receptor antagonist, but it does not exhibit selectivity among the α-2 receptors. Thus, to characterize the receptor subtype responsible for the loss of analgesia and gain of hyperalgesia, we studied the α-2A genetic knockout mouse. The WT and α-2A knockout mice were exposed to ultrasonic sound, and thermal latencies were determined by a masked observer at various times after ultrasonic exposure. As previously reported, thermal response latencies (unstressed) were similar between WT mice and α-2A knockout mice. The WT mice exhibited stress-induced analgesia immediately after stress (16.8 ± 0.7 s stressed vs.  11.1 ± 0.8 s unstressed; P  = 0.0001, n = 6 unstressed, 12 stressed; fig. 2A). In contrast, paw withdrawal latencies of α-2A knockout mice were significantly decreased immediately after ultrasonic stress, compared with no stress (8.9 ± 0.4 s stressed vs.  12.3 ± 0.8 s unstressed; P  = 0.0008, n = 6 unstressed, 12 stressed; fig. 2A). The analgesia in WT mice (n = 11) was only significant immediately following stress (fig. 2B), but the stress-induced hyperalgesia in the α-2A knockout mice (n = 5) lasted up to 30 min after stress (fig. 2B; F (5,29) = 9.6; P  < 0.0001 for comparison to prestress baseline). In addition, the stress-induced hyperalgesia did not habituate when α-2A knockout mice were stressed on three consecutive days (fig. 2C). Two-way ANOVA demonstrated a significant group effect (stressed vs.  unstressed α-2A knockout; F (1,20) = 53.96; P  < 0.0001, n = 6/group), but no effect of time. The α-2A knockout mice exhibited a loss of stress-induced analgesia and a gain of stress-induced behavioral hyperalgesia, mirroring the finding in genetically unaltered rodents treated systemically with α-2 antagonists.
WDR Neurons in α-2A Knockout Mice Exhibit Facilitation of Windup Response to Repeated Electrical Stimuli
The hyperalgesia in α-2A knockout mice was further characterized using electrophysiologic recordings from WDR neurons in the deep dorsal horn that receive converging inputs from afferent A- and C-fibers39,40 and exhibit increased excitability in response to repetitive noxious stimuli.31,41,42 Repeated electrophysiologic stimuli in anesthetized rodents have many parallels with footshock and other behavioral stressors and enable a more mechanistic investigation of the α-2A knockout mice hyperalgesia.28,31,43,44 The α-2A knockout mice exhibit normal electrophysiologic responses to single painful electrical stimuli, consistent with their normal thermal response latencies. There were no significant differences between the α-2A knockout (n = 62) and WT (n = 47) WDR neuronal response to graded intracutaneous electrical stimuli (0.05–5.0 mA, 2.0 ms) in the mean number of APs in the A-component and C-component (figs. 3A, B). The latency and threshold of the first C-fiber–mediated AP were not significantly different between the α-2A knockout (123.4 ± 3.9 ms, 1.67 ± 0.18 mA) and WT groups (129.5 ± 4.0 ms, 1.57 ± 0.17 mA). The latency and threshold of the first A-fiber–mediated AP were also comparable between the two genotypes (data not shown).
Fig. 3.  Deep wide dynamic range (WDR) neurons in α-2A knockout (KO) mice show enhanced windup response, compared with that in wild-type (WT) mice. Deep WDR neurons in α-2A KO (n = 62) and WT (n = 47) mice showed similar stimulus intensity-response functions of (A  ) A-fiber and (B  ) C-fiber–mediated responses to graded intracutaneous electrical stimuli applied to the receptive field (0.05–5.0 mA, 2.0 ms). Data are expressed as mean ± SEM number of action potentials (AP). (C  –E  ) C-component responses of deep WDR neurons in WT mice (n = 47) and in α-2A knockout mice (n = 62) to repetitive electrical stimulation (16 pulses, 3.0 mA, 2.0 ms) applied at frequencies of (C  ) 0.2 Hz, (D  ) 0.5 Hz, and (E  ) 1.0 Hz, respectively, are plotted against the stimulation number of each trial. The WDR neurons in α-2A knockout mice, but not in the WT mice, displayed windup to 0.2 Hz stimulation in addition to 0.5 Hz and 1.0 Hz stimulation. (F  ) The averaged C-fiber–mediated responses for stimulus 7–16 during the stimulation are plotted for various frequencies. Data are normalized by the response evoked by the first stimulation of each trial. **=P  < 0.01 and ***=P  < 0.001 versus  the input value; # =P  < 0.05 versus  the WT group. Data are expressed as mean ± SEM.
Fig. 3. 
	Deep wide dynamic range (WDR) neurons in α-2A knockout (KO) mice show enhanced windup response, compared with that in wild-type (WT) mice. Deep WDR neurons in α-2A KO (n = 62) and WT (n = 47) mice showed similar stimulus intensity-response functions of (A 
	) A-fiber and (B 
	) C-fiber–mediated responses to graded intracutaneous electrical stimuli applied to the receptive field (0.05–5.0 mA, 2.0 ms). Data are expressed as mean ± SEM number of action potentials (AP). (C  –E 
	) C-component responses of deep WDR neurons in WT mice (n = 47) and in α-2A knockout mice (n = 62) to repetitive electrical stimulation (16 pulses, 3.0 mA, 2.0 ms) applied at frequencies of (C 
	) 0.2 Hz, (D 
	) 0.5 Hz, and (E 
	) 1.0 Hz, respectively, are plotted against the stimulation number of each trial. The WDR neurons in α-2A knockout mice, but not in the WT mice, displayed windup to 0.2 Hz stimulation in addition to 0.5 Hz and 1.0 Hz stimulation. (F 
	) The averaged C-fiber–mediated responses for stimulus 7–16 during the stimulation are plotted for various frequencies. Data are normalized by the response evoked by the first stimulation of each trial. **=P 
	< 0.01 and ***=P 
	< 0.001 versus 
	the input value; # =P 
	< 0.05 versus 
	the WT group. Data are expressed as mean ± SEM.
Fig. 3.  Deep wide dynamic range (WDR) neurons in α-2A knockout (KO) mice show enhanced windup response, compared with that in wild-type (WT) mice. Deep WDR neurons in α-2A KO (n = 62) and WT (n = 47) mice showed similar stimulus intensity-response functions of (A  ) A-fiber and (B  ) C-fiber–mediated responses to graded intracutaneous electrical stimuli applied to the receptive field (0.05–5.0 mA, 2.0 ms). Data are expressed as mean ± SEM number of action potentials (AP). (C  –E  ) C-component responses of deep WDR neurons in WT mice (n = 47) and in α-2A knockout mice (n = 62) to repetitive electrical stimulation (16 pulses, 3.0 mA, 2.0 ms) applied at frequencies of (C  ) 0.2 Hz, (D  ) 0.5 Hz, and (E  ) 1.0 Hz, respectively, are plotted against the stimulation number of each trial. The WDR neurons in α-2A knockout mice, but not in the WT mice, displayed windup to 0.2 Hz stimulation in addition to 0.5 Hz and 1.0 Hz stimulation. (F  ) The averaged C-fiber–mediated responses for stimulus 7–16 during the stimulation are plotted for various frequencies. Data are normalized by the response evoked by the first stimulation of each trial. **=P  < 0.01 and ***=P  < 0.001 versus  the input value; # =P  < 0.05 versus  the WT group. Data are expressed as mean ± SEM.
×
In WT mice, many deep WDR neurons showed a windup response to repeated conditioning stimuli applied at frequencies of 0.5 Hz and 1.0 Hz, but rarely to 0.2 Hz stimulation (figs. 3C–E). The plateau level of windup measured as the averaged C-component responses during stimuli 7–16 of the trial were significantly increased at 0.5 Hz (185.3 ± 15.9%; P  = 0.0004) and 1.0 Hz (177.1 ± 17.2%; P  = 0.0008) stimulation, but not at 0.2 Hz (135.8 ± 6.8%; P  = 0.34), compared with the input (fig. 3F). In α-2A knockout mice, many WDR neurons exhibited strong windup to 0.2 Hz stimulation in addition to 0.5 and 1.0 Hz stimulation (figs. 3C–E). There were significant increases in the averaged C-component responses for stimuli 7–16 of the trial during all three frequencies tested (0.2 Hz: 199.4 ± 15.9%, P  = 0.0003; 0.5 Hz: 208.6 ± 15.9%, P  = 0.0003; 1.0 Hz: 165.8 ± 13.1%, P  = 0.0011), compared with the baseline input (fig. 3F). Importantly, the plateau level of windup to 0.2 Hz stimulation in α-2A knockout mice was significantly greater than that in WT mice (P  = 0.018; fig. 3F). Thus, the α-2A knockout mice exhibit increased sensitivity to sustained activation of nociceptive afferents by electrical stimuli, revealing a facilitatory mechanism that is normally inhibited by the α-2A receptor.
Chemical-induced Peripheral, But Not Central, Sensitization Enhanced in α-2A Knockout Mice
To further localize the facilitatory mechanism, we investigated the effect of distinct sensitizing agents on the response of the knockout mice to light stroking with a paint brush or to a hotplate.30 Peripheral sensitization was elicited with sulprostone, a selective noninflammatory EP1/EP3 prostaglandin receptor agonist, and tactile allodynia and thermal hyperalgesia were measured. The dose response of sulprostone-induced sensitization to mechanical and thermal stimuli was shifted to the left 10-fold in the α-2A knockout mice (figs. 4A, B). Significant mechanical allodynia occurred at intraperitoneal sulprostone doses ≥300 ng/kg−1(n = 6/group) in WT mice and ≥30 ng kg−1(n = 6/group) in α-2A knockout mice, and significant thermal hyperalgesia occurred at 1,000 ng/ kg−1(n = 6) sulprostone in WT mice and at 100 ng/kg−1(n = 6) and 300 ng/kg−1(n = 7) sulprostone in α-2A knockout mice. The responses to mechanical and thermal stimuli were significantly different between genotypes at the 30 ng/kg−1and 100 ng/kg−1doses (mechanical, P  < 0.001; thermal, P  < 0.01). Thus, peripheral sensitization was facilitated in the α-2A knockout mice even in the absence of ultrasonic stress.
Fig. 4.  α-2A Knockout (KO) mice show enhanced response to peripheral sensitizing agent. Dose-responses in wild-type (WT; red squares  ) and α-2A KO (blue circles  ) mice of intraperitoneal (IP) sulprostone effects on (A  ) tactile pain scores (n = 6, except n = 5 in 10 ng/kg−1KO group) and (B  ) thermal paw withdrawal latencies (n = 6, except n = 5 in 300 ng/kg−1WT group, n = 7 in 300 ng/kg−−1KO group, and n = 6 data from two experiments were combined for 30 ng kg–1WT and KO groups). Dose-responses in WT (red squares  ) and α-2A KO (blue circles  ) mice of intrathecal (IT) N  -methyl-d-aspartate (NMDA) effects on (C  ) tactile pain scores (n = 6, except n = 6 data from two experiments were combined for 100 ng/kg−1WT group), and (D  ) thermal paw withdrawal latencies (n = 6). The α-2A KO mice exhibit increased sensitivity to intraperitoneal sulprostone, but not intrathecal NMDA. §=P  < 0.001, increase in pain score versus  no drug (allodynia); ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no drug (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 4. 
	α-2A Knockout (KO) mice show enhanced response to peripheral sensitizing agent. Dose-responses in wild-type (WT; red squares 
	) and α-2A KO (blue circles 
	) mice of intraperitoneal (IP) sulprostone effects on (A 
	) tactile pain scores (n = 6, except n = 5 in 10 ng/kg−1KO group) and (B 
	) thermal paw withdrawal latencies (n = 6, except n = 5 in 300 ng/kg−1WT group, n = 7 in 300 ng/kg−−1KO group, and n = 6 data from two experiments were combined for 30 ng kg–1WT and KO groups). Dose-responses in WT (red squares 
	) and α-2A KO (blue circles 
	) mice of intrathecal (IT) N 
	-methyl-d-aspartate (NMDA) effects on (C 
	) tactile pain scores (n = 6, except n = 6 data from two experiments were combined for 100 ng/kg−1WT group), and (D 
	) thermal paw withdrawal latencies (n = 6). The α-2A KO mice exhibit increased sensitivity to intraperitoneal sulprostone, but not intrathecal NMDA. §=P 
	< 0.001, increase in pain score versus 
	no drug (allodynia); ++=P 
	< 0.01; +++=P 
	< 0.001, decrease in latency versus 
	no drug (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 4.  α-2A Knockout (KO) mice show enhanced response to peripheral sensitizing agent. Dose-responses in wild-type (WT; red squares  ) and α-2A KO (blue circles  ) mice of intraperitoneal (IP) sulprostone effects on (A  ) tactile pain scores (n = 6, except n = 5 in 10 ng/kg−1KO group) and (B  ) thermal paw withdrawal latencies (n = 6, except n = 5 in 300 ng/kg−1WT group, n = 7 in 300 ng/kg−−1KO group, and n = 6 data from two experiments were combined for 30 ng kg–1WT and KO groups). Dose-responses in WT (red squares  ) and α-2A KO (blue circles  ) mice of intrathecal (IT) N  -methyl-d-aspartate (NMDA) effects on (C  ) tactile pain scores (n = 6, except n = 6 data from two experiments were combined for 100 ng/kg−1WT group), and (D  ) thermal paw withdrawal latencies (n = 6). The α-2A KO mice exhibit increased sensitivity to intraperitoneal sulprostone, but not intrathecal NMDA. §=P  < 0.001, increase in pain score versus  no drug (allodynia); ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no drug (hyperalgesia). Data are expressed as mean ± SEM.
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To test whether the α-2 knockout mice also have an increase in susceptibility to central sensitizing stimuli, WT and α-2 knockout mice were injected intrathecally with varying concentrations of NMDA, which mimics the activation of dorsal horn neurons by the excitatory transmitter glutamate. Intrathecal NMDA induced a dose-dependent tactile allodynia (n = 6/group, except n = 6 data from two experiments combined for 100 ng/kg−1WT group) and thermal hyperalgesia (n = 6/group) with a similar dose-response in WT and knockout mice (figs. 4C, D). There were no significant between-genotype differences at any dose.
Systemic α-1-Adrenergic Receptor Blockade Prevents the Development of Stress-induced Hyperalgesia and Enhanced Windup Response in α-2A Knockout Mice
A previous study has demonstrated that in α-2A knockout mice the sympathetic nerves lose normal autoinhibition, resulting in increased sympathetic outflow during high-frequency stimulation, but autoinhibition of basal norepinephrine release is normal.14 Because stress can stimulate the SNS, we investigated whether the enhanced windup and stress-induced hyperalgesia in the α-2A knockout mice were potentially dependent on increased sympathoneural outflow and subsequent α-1 receptor activation. The effect of postsynaptic blockade with the α-1 receptor antagonist prazosin was determined. Recordings from WDR neurons were conducted in the presence or absence of prazosin in a blinded manner. Treatment of the α-2A knockout mice with prazosin (100 ng/kg−1intraperitoneally45) did not affect the A-fiber and C-fiber–mediated response of WDR neurons (n = 18) to single electrical stimuli (figs. 5A, B), but suppressed windup to repetitive stimuli at frequencies of 0.2, 0.5, and 1.0 Hz (figs. 5C–F). The averaged C-component responses for the stimulus 7–16 of the trial were significantly reduced from the respective preprazosin levels (0.2 Hz: 217.1 ± 26.0% vs  . 160.6 ± 13.6%, P  = 0.0021; 0.5 Hz: 223.7 ± 28.4% vs.  166.6 ± 22.9%, P  = 0.018; 1.0 Hz: 197.8 ± 20.2% vs.  135.9 ± 20.1%, P  = 0.0007; fig. 5F). Systemic pretreatment (30 min) with 100 ng/kg−1intraperitoneal prazosin had no effect on the thermal latencies of unstressed WT or α-2A knockout mice (n = 6/group, fig. 6A). The antagonist did not decrease stress-induced analgesia in the WT mice. However, the antagonist prevented the development of the α-2A knockout mouse stress-induced hyperalgesic behavior but did not restore stress-induced analgesia (n = 6/group, fig. 6A). Intrathecal injection of 10 ng prazosin, which is a threefold greater total body dose than 100 ng/kg−1intraperitoneally in mice weighing approximately 30 g, did not prevent stress-induced hyperalgesia in α-2A knockout mice (n = 6/group, fig. 6B).
Fig. 5.  Systemic administration of prazosin attenuates windup levels without changing A-fiber and C-fiber–mediated responses of wide dynamic range (WDR) neurons to graded electrical stimulation in α-2A knockout (KO) mice. (A  and B  ) In α-2A KO mice, systemic administration of the α-1 receptor antagonist prazosin (0.1 μg/kg−1intraperitoneal) did not significantly change the (A  ) A-fiber and (B  ) C-fiber–mediated responses (number of action potentials, AP) of WDR neurons (n = 18) to graded electrical stimulation. (C  –E  ) Prazosin suppressed windup levels across (C  ) 0.2 Hz, (D  ) 0.5 Hz, and (E  ) 1.0 Hz stimulation in α-2A KO mice. (F  ) The averaged C-component responses for the stimulus 7–16 of the trial were also significantly reduced during 0.2, 0.5, and 1.0 Hz stimulation after prazosin treatment, compared with the preprazosin condition. Data are normalized by the response evoked by the first stimulation of each trial. # =P  < 0.05; ## =P  < 0.01; ### =P  < 0.001 versus  preprazosin condition. Data are expressed as mean ± SEM.
Fig. 5. 
	Systemic administration of prazosin attenuates windup levels without changing A-fiber and C-fiber–mediated responses of wide dynamic range (WDR) neurons to graded electrical stimulation in α-2A knockout (KO) mice. (A 
	and B 
	) In α-2A KO mice, systemic administration of the α-1 receptor antagonist prazosin (0.1 μg/kg−1intraperitoneal) did not significantly change the (A 
	) A-fiber and (B 
	) C-fiber–mediated responses (number of action potentials, AP) of WDR neurons (n = 18) to graded electrical stimulation. (C  –E 
	) Prazosin suppressed windup levels across (C 
	) 0.2 Hz, (D 
	) 0.5 Hz, and (E 
	) 1.0 Hz stimulation in α-2A KO mice. (F 
	) The averaged C-component responses for the stimulus 7–16 of the trial were also significantly reduced during 0.2, 0.5, and 1.0 Hz stimulation after prazosin treatment, compared with the preprazosin condition. Data are normalized by the response evoked by the first stimulation of each trial. # =P 
	< 0.05; ## =P 
	< 0.01; ### =P 
	< 0.001 versus 
	preprazosin condition. Data are expressed as mean ± SEM.
Fig. 5.  Systemic administration of prazosin attenuates windup levels without changing A-fiber and C-fiber–mediated responses of wide dynamic range (WDR) neurons to graded electrical stimulation in α-2A knockout (KO) mice. (A  and B  ) In α-2A KO mice, systemic administration of the α-1 receptor antagonist prazosin (0.1 μg/kg−1intraperitoneal) did not significantly change the (A  ) A-fiber and (B  ) C-fiber–mediated responses (number of action potentials, AP) of WDR neurons (n = 18) to graded electrical stimulation. (C  –E  ) Prazosin suppressed windup levels across (C  ) 0.2 Hz, (D  ) 0.5 Hz, and (E  ) 1.0 Hz stimulation in α-2A KO mice. (F  ) The averaged C-component responses for the stimulus 7–16 of the trial were also significantly reduced during 0.2, 0.5, and 1.0 Hz stimulation after prazosin treatment, compared with the preprazosin condition. Data are normalized by the response evoked by the first stimulation of each trial. # =P  < 0.05; ## =P  < 0.01; ### =P  < 0.001 versus  preprazosin condition. Data are expressed as mean ± SEM.
×
Fig. 6.  Inhibition of sympathetic outflow prevents stress-induced hyperalgesia in α-2A knockout (KO) mice. (A  –C  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in wild-type (WT) and α-2A KO mice after pretreatment with a saline control (n = 6) or the α-1 receptor antagonist prazosin, by (A  ) intraperitoneal (IP, 0.1 μg/kg−1; n = 6) or (B  ) intrathecal (10 ng; n = 6) injection, or (C  ) after guanethidine (guan) sympathectomy (n = 8, except n = 10 in guanethidine-treated KO group). (D  ) Tactile pain scores (n = 6, except n = 5 in 100, 300, 3,000 ng/kg−1KO groups) and (E  ) paw withdrawal latencies (n = 6, except n = 4 in 100 ng/kg−1KO group and n = 7 in 3,000 ng/kg−1KO groups) in response to IP sulprostone in WT and α-2A KO mice with guanethidine sympathectomy (green, WT; light blue, KO) compared with data without guanethidine sympathectomy from figures 4A  and B  (red, WT; blue, KO). Intraperitoneal prazosin and guanethidine sympathectomy prevent hyperalgesia in response to stress and sulprostone in α-2A KO mice. **=P  < 0.01; ***=P  < 0.001, increase in latency versus  no stress (analgesia); §=P  < 0.001, increase in pain score versus  no sulprostone (allodynia); +=P  < 0.05; ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no stress or versus  no sulprostone (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 6. 
	Inhibition of sympathetic outflow prevents stress-induced hyperalgesia in α-2A knockout (KO) mice. (A  –C 
	) Paw withdrawal latencies after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in wild-type (WT) and α-2A KO mice after pretreatment with a saline control (n = 6) or the α-1 receptor antagonist prazosin, by (A 
	) intraperitoneal (IP, 0.1 μg/kg−1; n = 6) or (B 
	) intrathecal (10 ng; n = 6) injection, or (C 
	) after guanethidine (guan) sympathectomy (n = 8, except n = 10 in guanethidine-treated KO group). (D 
	) Tactile pain scores (n = 6, except n = 5 in 100, 300, 3,000 ng/kg−1KO groups) and (E 
	) paw withdrawal latencies (n = 6, except n = 4 in 100 ng/kg−1KO group and n = 7 in 3,000 ng/kg−1KO groups) in response to IP sulprostone in WT and α-2A KO mice with guanethidine sympathectomy (green, WT; light blue, KO) compared with data without guanethidine sympathectomy from figures 4A 
	and B 
	(red, WT; blue, KO). Intraperitoneal prazosin and guanethidine sympathectomy prevent hyperalgesia in response to stress and sulprostone in α-2A KO mice. **=P 
	< 0.01; ***=P 
	< 0.001, increase in latency versus 
	no stress (analgesia); §=P 
	< 0.001, increase in pain score versus 
	no sulprostone (allodynia); +=P 
	< 0.05; ++=P 
	< 0.01; +++=P 
	< 0.001, decrease in latency versus 
	no stress or versus 
	no sulprostone (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 6.  Inhibition of sympathetic outflow prevents stress-induced hyperalgesia in α-2A knockout (KO) mice. (A  –C  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in wild-type (WT) and α-2A KO mice after pretreatment with a saline control (n = 6) or the α-1 receptor antagonist prazosin, by (A  ) intraperitoneal (IP, 0.1 μg/kg−1; n = 6) or (B  ) intrathecal (10 ng; n = 6) injection, or (C  ) after guanethidine (guan) sympathectomy (n = 8, except n = 10 in guanethidine-treated KO group). (D  ) Tactile pain scores (n = 6, except n = 5 in 100, 300, 3,000 ng/kg−1KO groups) and (E  ) paw withdrawal latencies (n = 6, except n = 4 in 100 ng/kg−1KO group and n = 7 in 3,000 ng/kg−1KO groups) in response to IP sulprostone in WT and α-2A KO mice with guanethidine sympathectomy (green, WT; light blue, KO) compared with data without guanethidine sympathectomy from figures 4A  and B  (red, WT; blue, KO). Intraperitoneal prazosin and guanethidine sympathectomy prevent hyperalgesia in response to stress and sulprostone in α-2A KO mice. **=P  < 0.01; ***=P  < 0.001, increase in latency versus  no stress (analgesia); §=P  < 0.001, increase in pain score versus  no sulprostone (allodynia); +=P  < 0.05; ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no stress or versus  no sulprostone (hyperalgesia). Data are expressed as mean ± SEM.
×
Role of Postganglionic Sympathetic Outflow in Enhanced Pain Response
Chemical Sympathectomy with Guanethidine Blocks Stress-induced Hyperalgesia and Chemical-induced Peripheral Sensitization in α-2A Knockout Mice.
We investigated whether the postganglionic SNS was required for the stress-induced thermal hyperalgesia in α-2A knockout mice. Chemical ablation of the mouse SNS with guanethidine (50 mg/kg−1intraperitoneally) 1 day before testing did not alter baseline thermal latencies. Compared with vehicle-treated WT mice (n = 8), the guanethidine-treated WT mice (n = 8) exhibited slightly reduced stress-induced analgesia. The vehicle-treated α-2A knockout mice (n = 8) developed stress-induced thermal hyperalgesia, but the guanethidine-treated α-2A knockout mice (n = 10) did not (fig. 6C), demonstrating that the stress-induced thermal hyperalgesia requires the SNS.
We also investigated whether the postganglionic SNS was required for the enhanced sensitivity to the peripheral sensitization by sulprostone. The WT and α-2A knockout mice were chemically sympathectomized by guanethidine (50 mg/kg−1intraperitoneally) treatment. Sulprostone sensitivity, both mechanical (fig. 6D) and thermal (fig. 6E), was decreased 30-fold to 100-fold in α-2A knockout mice 1 day after guanethidine sympathectomy. Guanethidine sympathectomy also decreased the sensitivity of WT mice to sulprostone, but to a lesser extent, so that the sympathectomized WT and α-2A knockout mice exhibited similar responsiveness. Significant mechanical allodynia was only observed at 1,000 ng/kg−1(n = 6) in WT mice and 3,000 ng/kg−1(n = 5) in α-2A knockout mice with a significant between-genotype difference at 1,000 ng/kg−1(P  < 0.001, fig. 6D). Significant thermal hyperalgesia occurred at ≥1,000 ng/kg−1(n = 6/group) in WT mice and 3,000 ng/kg−1(n = 7) in α-2A knockout mice with no between-genotype differences (fig. 6E).
Surgical Sympathectomy: Postganglionic Sympathetic Nerves Critical to the Development of Stress-induced Hyperalgesia.
Guanethidine treatment could potentially have additional nonselective actions, and hence the effects of surgical sympathectomy were studied. In order to investigate the effect of surgical sympathectomy and better isolate peripheral drug effects, we conducted studies in the rat model rather than in mice. To determine whether a loss of peripheral α-2 receptor function is sufficient to decrease paw withdrawal latencies, rats were unilaterally injected with intraplantar rauwolscine (1 μg) immediately before stress. The paw with-drawal latencies of the ipsilateral and contralateral paws were independently determined by a masked observer in separate experiments. Contralateral paw withdrawal latencies were significantly increased in stressed sham sympathectomy rats compared with unstressed control rats (16.1 ± 1.2 s following stress and 12.6 ± 0.5 s without stress; P  = 0.014, n = 12 unstressed, 11 stressed), demonstrating that in the stressed animals spinal-mediated inhibition and its behavioral manifestation (analgesia) are intact (fig. 7A). In contrast, ipsilateral paw withdrawal latencies in sham sympathectomy rats were not increased following stress (11.5 ± 0.7 s following stress and 11.8 ± 0.6 s without stress; P  = 0.76, n = 12/group), demonstrating an effect of intraplantar rauwolscine that is limited to the injected paw (fig. 7B). The SNS dependence of the intraplantar rauwolscine-mediated prevention of increased paw withdrawal latencies was determined by surgical ablation of the L2–L5 postganglionic chain. Rats that had a surgical sympathectomy and were treated with intraplantar rauwolscine exhibited stress-induced analgesia in both paws, with ipsilateral paw withdrawal latencies of 18.8 ± 0.4 s following stress and 12.5 ± 0.7 s without stress (P  < 0.0001, n = 13 unstressed, 12 stressed; fig. 7B) and contralateral paw withdrawal latencies of 17.3 ± 0.7 s following stress and 11.1 ± 0.6 s without stress (P  < 0.0001, n = 11 unstressed, 12 stressed; fig. 7A). Hence, pain facilitation caused by local blockade of α-2 receptors on postganglionic sympathetic nerves can counterbalance spinal inhibition and negate its behavioral manifestation (analgesia).
Fig. 7.  Stress-induced hyperalgesic response in rats ablated by sympathectomy. (A  ) Paw withdrawal latencies of paws contralateral to 1 μg rauwolscine-injected paws after no stress (red bars  ) or ultrasonic stress (blue bars  ) in sham (n = 12 unstressed, 11 stressed) or surgically sympathectomized (n = 11 unstressed, 12 stressed) Sprague-Dawley rats. Stress-induced analgesia was unaffected by contralateral intraplantar rauwolscine injection or sympathectomy. (B  ) Paw withdrawal latencies of 1 μg rauwolscine-injected paw after no stress (red bars  ) or ultrasonic stress (blue bars  ) in sham (n = 12) or surgically sympathectomized (n = 13 unstressed, 12 stressed) Sprague-Dawley rats. Intraplantar rauwolscine blocked and sympathectomy restored a stress-induced analgesia response in the ipsilateral rauwolscine-treated paw. *=P  < 0.05; ***=P  < 0.001 versus  no stress (analgesia). Data are expressed as mean ± SEM.
Fig. 7. 
	Stress-induced hyperalgesic response in rats ablated by sympathectomy. (A 
	) Paw withdrawal latencies of paws contralateral to 1 μg rauwolscine-injected paws after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in sham (n = 12 unstressed, 11 stressed) or surgically sympathectomized (n = 11 unstressed, 12 stressed) Sprague-Dawley rats. Stress-induced analgesia was unaffected by contralateral intraplantar rauwolscine injection or sympathectomy. (B 
	) Paw withdrawal latencies of 1 μg rauwolscine-injected paw after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in sham (n = 12) or surgically sympathectomized (n = 13 unstressed, 12 stressed) Sprague-Dawley rats. Intraplantar rauwolscine blocked and sympathectomy restored a stress-induced analgesia response in the ipsilateral rauwolscine-treated paw. *=P 
	< 0.05; ***=P 
	< 0.001 versus 
	no stress (analgesia). Data are expressed as mean ± SEM.
Fig. 7.  Stress-induced hyperalgesic response in rats ablated by sympathectomy. (A  ) Paw withdrawal latencies of paws contralateral to 1 μg rauwolscine-injected paws after no stress (red bars  ) or ultrasonic stress (blue bars  ) in sham (n = 12 unstressed, 11 stressed) or surgically sympathectomized (n = 11 unstressed, 12 stressed) Sprague-Dawley rats. Stress-induced analgesia was unaffected by contralateral intraplantar rauwolscine injection or sympathectomy. (B  ) Paw withdrawal latencies of 1 μg rauwolscine-injected paw after no stress (red bars  ) or ultrasonic stress (blue bars  ) in sham (n = 12) or surgically sympathectomized (n = 13 unstressed, 12 stressed) Sprague-Dawley rats. Intraplantar rauwolscine blocked and sympathectomy restored a stress-induced analgesia response in the ipsilateral rauwolscine-treated paw. *=P  < 0.05; ***=P  < 0.001 versus  no stress (analgesia). Data are expressed as mean ± SEM.
×
Discussion
α-2-Adrenergic receptor regulation is integral at many levels of the stress pathway. The results of the described studies demonstrate a balance between pain inhibitory/analgesic and pain facilitatory/hyperalgesic mechanisms activated by stress that is shifted toward analgesia by α-2 receptor activity. α-2A- and α-2C-adrenergic receptors are located in the spinal cord dorsal horn.16 Previous studies with α-2 knockout mice have demonstrated that the α-2A receptor is necessary for spinal analgesia with α-2 agonists20–22 and that the α-2C receptor interacts with the opioid system in the spinal cord.46 The lack of stress-induced analgesia after treatment with two different α-2 antagonists (fig. 1) and in the α-2A knockout mice (fig. 2) demonstrates a physiologic role for the spinal α-2A receptors and is consistent with pharmacologic studies using spinal idazoxan and yohimbine that demonstrated that descending inhibition of dorsal horn nociceptive inputs is mediated by α-2-adrenergic receptors.12 
The unmasking of stress-induced hyperalgesia after α-2 antagonist treatment or in the α-2A knockout mice reveals an underlying pain facilitatory mechanism activated by acute stress that is normally attenuated by α-2 receptors. The hyperalgesia can be induced by both a psychologic stressor (ultrasonic noise) and a physical stressor (noxious footshock), suggesting that it may involve a common pathway activated by different types of stressors (figs. 1A, B). Despite the differences between the two stressors, both induce a nonhabituating, opioid-independent analgesia when the α-2A receptor is functional and activate the hypothalamic-pituitary-adrenal axis and SNS.24,25,47 
Multiple lines of evidence demonstrate that the observed stress-induced hyperalgesia is mechanistically distinct from stress-induced analgesia, and not just because of the loss of spinally mediated analgesia. For example, 3 μg intrathecal rauwolscine treatment blocked stress-induced analgesia without the development of hyperalgesia. In contrast, an equivalent total body dose administered systemically (intraperitoneal, 0.1 mg/kg−1) blocked analgesia and produced hyperalgesia (figs. 1C, E). The opposite result was also true. A 100-ng/kg−1intraperitoneal dose, but not a similar intrathecal total body dose (10 ng), of the α-1 antagonist prazosin (figs. 6A, B), or guanethidine treatment (fig. 6C) blocked the development of stress-induced hyperalgesia in α-2A knockout mice but did not produce analgesia. These findings illustrate that the loss of analgesia and gain of hyperalgesia (or vice versa  ) are distinct mechanisms involving different sites of action.
Repeated nociceptive electrical stimuli applied to the footpads to induce windup share obvious common features with footshock stress, including activation of primary afferents, midbrain noradrenergic pathways, the SNS, and spinal and supraspinal descending inhibitory circuits.28,31,43,44 The same frequency of electrical stimulation (0.5 Hz) that activates noradrenergic neurons in the locus coeruleus and induces descending pain inhibitory mechanisms also induces windup of dorsal horn WDR neurons.31,43,44 Because of these similarities to standard stressors, electrophysiologic assessment of the deep dorsal horn WDR neuron response to repetitive noxious electrical stimuli was used to dissect the hyperalgesia mechanism.
The pain facilitatory/hyperalgesic mechanism is detectable in the α-2A knockout mice as a decreased frequency threshold for developing short-term neuronal sensitization to repeated electrical stimuli. The dorsal horn WDR neuron responses to acute intracutaneous electrical stimuli were similar between the α-2A knockout and WT mice (figs. 3A, B), demonstrating normal nociception. However, WDR neuronal responses differed with repetitive electrical stimuli that cause progressive increase in dorsal horn neuronal excitability, called windup (figs. 3C–E). WDR neurons in normal rodents rarely exhibit windup to conditioning electrical stimulation at a frequency less than 0.3 Hz.31,48 In line with this observation, 0.2 Hz stimulation did not induce significant windup in WT mice in the current study. However, there was windup to the 0.2 Hz stimulus in α-2A knockout mice, demonstrating a decreased frequency threshold for the induction of windup. Interestingly, this pattern of facilitated windup is similar to that previously observed in μ-opioid receptor knockout mice.31 
To further localize the pain facilitation mechanism, sensitizing agents were applied at various points in the pain pathway. The α-2A knockout mice exhibited a 10-fold decrease in the concentration of the noninflammatory prostaglandin analog sulprostone that caused dynamic tactile allodynia in response to a paint brush, and there was a 3- to 10-fold decrease in the concentration of sulprostone that reduced paw withdrawal latency to a thermal stimulus (figs. 4A, B). The increased sensitivity to both tactile and thermal stimuli suggests that both A- and C-fibers may be affected. There was no increase in the pain behavior to spinal NMDA in α-2A knockout mice (figs. 4C, D), consistent with a peripheral, and not postsynaptic spinal, location of the facilitation mechanism.
The decreased sensitization thresholds to sustained chemical and electrical stimuli in the α-2A knockout mice and the decreased thermal threshold following exposure to noise and footshock stress suggests that the α-2 receptor normally attenuates a mechanism that facilitates the pain response to sustained stimuli. Multiple lines of evidence presented in this article point to a previously unrecognized role of the postganglionic SNS and sympathetic overflow in uninjured animals for the facilitated pain responses. The increased sensitivity of the α-2A knockout mice was reversed by various sympatholytic treatments. Because postsynaptic α-1-adrenergic receptors mediate many of the excitatory actions of the SNS, the role of α-1 receptor activation was tested by coadministration with the α-1 antagonist prazosin. Systemic prazosin did not alter normal thermal sensitivity, but completely blocked the development of stress-induced thermal hyperalgesia in the α-2A knockout mice (fig. 6A). Spinal administration of 10 ng prazosin was ineffective, despite being a greater total body dose than the effective 100 ng/kg−1intraperitoneal dose, consistent with a peripheral site of action (fig. 6B). Intraperitoneal prazosin treatment also suppressed windup to repetitive electrical stimuli at all frequencies in the α-2A knockout mice (figs. 5C–F). This result indicates that activation of peripheral α-1 receptors in the absence of α-2A receptors may lower the frequency threshold for the induction of windup, and also enhance the windup response at higher frequencies of stimulation. The finding is consistent with previous reports that α-1 receptor activation enhances neurogenic inflammation7 and opposes α-2 receptor-mediated analgesia.45 
Guanethidine treatment depletes norepinephrine from postsynaptic SNS nerve endings, resulting in a transient chemical sympathectomy.49 As with prazosin, guanethidine pretreatment did not affect thermal response in the absence of stress but eliminated hyperalgesia caused by ultrasonic stress in the α-2A knockout mice (fig. 6C). Guanethidine sympathectomy also dramatically increased the concentration threshold for sulprostone sensitization 30- to 100-fold in the α-2A knockout mice and increased, to a smaller extent, the sensitization threshold in WT mice (figs. 6D, E). Thus, a SNS dependent decrease of sensory thresholds can also occur in WT mice, but it is more pronounced in α-2A knockout mice.
The potential for SNS postganglionic nerves to mediate development of stress-induced pain facilitation in normal, uninjured animals was also demonstrated in the rats with rauwolscine blockade of α-2 receptors. Intraplantar injection of rauwolscine prevented increased paw withdrawal latency of the injected paw following stress (fig. 7B, sham) even though stress-induced analgesia was still apparent in the prolonged withdrawal response of the contralateral paw (fig. 7A, sham), demonstrating that rauwolscine was acting locally on peripheral α-2 receptors. The rauwolscine effect was prevented by surgical removal of lumbar sympathetic ganglia (fig. 7B, sympathectomy). Hence, the facilitatory mechanism that is normally attenuated by α-2 receptor activation requires postganglionic sympathetic fibers. This peripheral mechanism likely involves SNS overflow because of decreased α-2 receptor-mediated feedback inhibition of neurotransmitter release from SNS postganglionic nerve endings. Previous studies of hyperalgesia evoked by immune mediators50 have implicated sympathoadrenal enhancement of primary afferent sensitivity developing over several days. Because the effect of stress in this study is acute and the preganglionic innervation of the adrenal medulla was unaffected by the lumbar sympathectomy, this study does not involve a sympathoadrenal mechanism but demonstrates sympathoneuronal enhancement of primary afferent responses.
The behavioral outcome of the effects of stress on pain sensation appears to reflect a balance between descending spinal pain inhibitory mechanisms and SNS-dependent pain facilitation. This was demonstrated by the different effect of intraperitoneal (fig. 1A) and intraplantar injection of rauwolscine (fig. 7B). The stress-induced reduction in thermal response latency following local intraplantar injection was less than that seen following systemic intraperitoneal rauwolscine injection, presumably because descending inhibition was not disrupted by the intraplantar injection. Although stress-induced analgesia is distinct from the stress-induced hyperalgesia mechanism, a reduction of descending inhibition is needed to reveal the stress-induced hyperalgesia. The increased thermal response latencies of contralateral paws (fig. 7A) compared with that of ipsilateral paws (fig. 7B) after intraplantar rauwolscine injection further demonstrate that analgesia is only manifested when peripheral pain facilitation is attenuated. Interestingly, evidence for physiologic antagonism between spinal inhibition and the SNS was shown in early studies characterizing footshock-induced analgesia. Watkins et al.  showed that inhibition of norepinephrine outflow from SNS postganglionic fibers with bretylium tosylate enhanced stress-induced analgesia.47 
Previous findings demonstrate that the SNS can interact with pain fibers without previous injury or inflammation, resulting in a decreased response threshold. It has been shown in rabbits that sympathetic stimulation can affect the electrical properties of unmyelinated sensory neurons without activating them,51 and intradermal injection of norepinephrine and other α-agonists resulted in a decreased thermal pain threshold in normal subjects.52 This study demonstrates that when SNS outflow is disinhibited and descending inhibition is diminished, as occurs in the α-2A knockout mice or after treatment with systemic rauwolscine, the SNS effect on primary afferents can be amplified, unmasking stress-induced hyperalgesia (see model in fig. 8). Activation of nociceptive afferents can elicit preganglionic sympathetic neuron activation via  spinal and supraspinal pathways.50 When SNS outflow is increased and descending inhibition is diminished, the effects of stress and sensitizing and nociceptive stimuli could be expected to result in a positive feedback loop that triggers enhanced sensation of pain.
Fig. 8.  Model of stress-induced hyperalgesia. (1  ) Spinal α-2-adrenergic receptors on central terminals of sensory afferents and dorsal horn projection neurons mediate descending adrenergic inhibition, resulting in stress-induced analgesia. (2  ) Peripheral α-2 receptors on sympathetic postganglionic nerves (SPGNs) mediate feedback inhibition of norepinephrine release in response to stress. (3  ) In α-2A knockout mice or following treatment with α-2 antagonists (intraperitoneal or intraplantar), α-2 feedback inhibition is reduced, resulting in dysregulated (enhanced) norepinephrine release from SPGNs and sensitization of sensory afferents (4  ), which leads to stress-induced hyperalgesia when descending adrenergic inhibition is reduced. Role of α-1-adrenergic activation (4  ) in stress-induced hyperalgesia and decreased sensory afferent thresholds to repeated transcutaneous electrical stimuli was demonstrated by prazosin block. Role of SPGNs in stress-induced hyperalgesia and enhanced sensitivity of sensory afferents to prostaglandin E2receptor (EP) activation (4  ) was demonstrated by guanethidine depletion of norepinephrine and surgical sympathectomy. For simplicity, the α-1-adrenergic receptor is drawn on the sensory afferent, but sensitization could also be indirect via  another cell type such as a monocyte (5  ). Dysregulated sympathetic outflow (3  ) can result in a positive feedback loop between sensory afferents and sympathetic nerves via  spinal and supraspinal pathways when descending inhibition is reduced.
Fig. 8. 
	Model of stress-induced hyperalgesia. (1 
	) Spinal α-2-adrenergic receptors on central terminals of sensory afferents and dorsal horn projection neurons mediate descending adrenergic inhibition, resulting in stress-induced analgesia. (2 
	) Peripheral α-2 receptors on sympathetic postganglionic nerves (SPGNs) mediate feedback inhibition of norepinephrine release in response to stress. (3 
	) In α-2A knockout mice or following treatment with α-2 antagonists (intraperitoneal or intraplantar), α-2 feedback inhibition is reduced, resulting in dysregulated (enhanced) norepinephrine release from SPGNs and sensitization of sensory afferents (4 
	), which leads to stress-induced hyperalgesia when descending adrenergic inhibition is reduced. Role of α-1-adrenergic activation (4 
	) in stress-induced hyperalgesia and decreased sensory afferent thresholds to repeated transcutaneous electrical stimuli was demonstrated by prazosin block. Role of SPGNs in stress-induced hyperalgesia and enhanced sensitivity of sensory afferents to prostaglandin E2receptor (EP) activation (4 
	) was demonstrated by guanethidine depletion of norepinephrine and surgical sympathectomy. For simplicity, the α-1-adrenergic receptor is drawn on the sensory afferent, but sensitization could also be indirect via 
	another cell type such as a monocyte (5 
	). Dysregulated sympathetic outflow (3 
	) can result in a positive feedback loop between sensory afferents and sympathetic nerves via 
	spinal and supraspinal pathways when descending inhibition is reduced.
Fig. 8.  Model of stress-induced hyperalgesia. (1  ) Spinal α-2-adrenergic receptors on central terminals of sensory afferents and dorsal horn projection neurons mediate descending adrenergic inhibition, resulting in stress-induced analgesia. (2  ) Peripheral α-2 receptors on sympathetic postganglionic nerves (SPGNs) mediate feedback inhibition of norepinephrine release in response to stress. (3  ) In α-2A knockout mice or following treatment with α-2 antagonists (intraperitoneal or intraplantar), α-2 feedback inhibition is reduced, resulting in dysregulated (enhanced) norepinephrine release from SPGNs and sensitization of sensory afferents (4  ), which leads to stress-induced hyperalgesia when descending adrenergic inhibition is reduced. Role of α-1-adrenergic activation (4  ) in stress-induced hyperalgesia and decreased sensory afferent thresholds to repeated transcutaneous electrical stimuli was demonstrated by prazosin block. Role of SPGNs in stress-induced hyperalgesia and enhanced sensitivity of sensory afferents to prostaglandin E2receptor (EP) activation (4  ) was demonstrated by guanethidine depletion of norepinephrine and surgical sympathectomy. For simplicity, the α-1-adrenergic receptor is drawn on the sensory afferent, but sensitization could also be indirect via  another cell type such as a monocyte (5  ). Dysregulated sympathetic outflow (3  ) can result in a positive feedback loop between sensory afferents and sympathetic nerves via  spinal and supraspinal pathways when descending inhibition is reduced.
×
Physiologically, disinhibition of SNS outflow and reduced descending inhibition could result from α-2 receptor desensitization or depletion of norepinephrine during chronic stress. It has been reported that administration of a high dose of the α-2 receptor agonist clonidine to rats results in a delayed thermal and tactile hypersensitivity associated with changes in spinal cord excitatory neurotransmission.53 It is possible that this result is caused by α-2 receptor desensitization and mimics the effects of sustained norepinephrine outflow during chronic stress. Although the experiments reported here have focused on pain responses to acute stressors, the potential role of dysregulated SNS outflow and descending inhibition in chronic pain disorders is highlighted by our findings that the hyperalgesia, unlike the analgesia, persisted substantially longer than the stress (fig. 2B) and that the hyperalgesia did not habituate to repeated stress (fig. 2C). This mechanism could potentially contribute to episodes of heightened pain sensitivity in conditions such as irritable bowel syndrome and fibromyalgia that have been associated with autonomic dysfunction and excess sympathetic activity.54–56 
The authors thank Brian Kobilka, Ph.D. (Professor, Department of Molecular and Cellular Physiology, Stanford University School of Medicine, Palo Alto, California), for originally supplying the α-2 receptor knockout mouse lines; Lauren Luhrs, Ph.D. (Principal Scientist, Biologic Sciences, Allergan, Inc., Irvine, California), and Veena Viswanath, Ph.D. (Principal Scientist, Biologic Sciences, Allergan, Inc.), for comments on the manuscript; Larry Wheeler, Ph.D. (Senior Vice President, Biologic Sciences, Allergan, Inc.), for his support of the project; and Lisa Rubin, B.A. (Executive Secretary, Biologic Sciences, Allergan, Inc.), for editorial assistance. Sushma Soni, B.Sc., B.Com. (Senior Medical Writer, Wolters Kluwer, Yardley, Pennsylvania), also provided editorial assistance (copyediting and formatting).
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Fig. 1.  Stress-induced hyperalgesia resulting from systemic α-2-adrenergic blockade in rats and wild-type (WT) mice. (A  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in Sprague-Dawley (SD) rats treated with intraperitoneal (IP) saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 6). (B  ) Paw withdrawal latencies after no stress (red bars  ) or footshock stress (blue bars  ) in Sprague-Dawley rats treated with IP saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 12). (C  and D  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in C57BL/6 WT mice treated with IP saline (n = 6) or the α-2-adrenergic receptor antagonists (C  ) 0.1 mg/kg−1rauwolscine (n = 6) or (D  ) 0.03 mg/kg−1idazoxan (n = 6). (E  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in Sprague-Dawley rats treated with intrathecal (IT) saline (n = 6) or 3 μg rauwolscine (n = 6). The antagonists transform stress-induced analgesia into stress-induced hyperalgesia when dosed intraperitoneally and block stress-induced analgesia without inducing hyperalgesia when dosed intrathecally. **=P  < 0.01; ***=P  < 0.001, increase in latency versus  no stress (analgesia); +=P  < 0.05; ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no stress (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 1. 
	Stress-induced hyperalgesia resulting from systemic α-2-adrenergic blockade in rats and wild-type (WT) mice. (A 
	) Paw withdrawal latencies after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in Sprague-Dawley (SD) rats treated with intraperitoneal (IP) saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 6). (B 
	) Paw withdrawal latencies after no stress (red bars 
	) or footshock stress (blue bars 
	) in Sprague-Dawley rats treated with IP saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 12). (C 
	and D 
	) Paw withdrawal latencies after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in C57BL/6 WT mice treated with IP saline (n = 6) or the α-2-adrenergic receptor antagonists (C 
	) 0.1 mg/kg−1rauwolscine (n = 6) or (D 
	) 0.03 mg/kg−1idazoxan (n = 6). (E 
	) Paw withdrawal latencies after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in Sprague-Dawley rats treated with intrathecal (IT) saline (n = 6) or 3 μg rauwolscine (n = 6). The antagonists transform stress-induced analgesia into stress-induced hyperalgesia when dosed intraperitoneally and block stress-induced analgesia without inducing hyperalgesia when dosed intrathecally. **=P 
	< 0.01; ***=P 
	< 0.001, increase in latency versus 
	no stress (analgesia); +=P 
	< 0.05; ++=P 
	< 0.01; +++=P 
	< 0.001, decrease in latency versus 
	no stress (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 1.  Stress-induced hyperalgesia resulting from systemic α-2-adrenergic blockade in rats and wild-type (WT) mice. (A  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in Sprague-Dawley (SD) rats treated with intraperitoneal (IP) saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 6). (B  ) Paw withdrawal latencies after no stress (red bars  ) or footshock stress (blue bars  ) in Sprague-Dawley rats treated with IP saline (n = 6) or 0.1 mg/kg−1rauwolscine (n = 12). (C  and D  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in C57BL/6 WT mice treated with IP saline (n = 6) or the α-2-adrenergic receptor antagonists (C  ) 0.1 mg/kg−1rauwolscine (n = 6) or (D  ) 0.03 mg/kg−1idazoxan (n = 6). (E  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in Sprague-Dawley rats treated with intrathecal (IT) saline (n = 6) or 3 μg rauwolscine (n = 6). The antagonists transform stress-induced analgesia into stress-induced hyperalgesia when dosed intraperitoneally and block stress-induced analgesia without inducing hyperalgesia when dosed intrathecally. **=P  < 0.01; ***=P  < 0.001, increase in latency versus  no stress (analgesia); +=P  < 0.05; ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no stress (hyperalgesia). Data are expressed as mean ± SEM.
×
Fig. 2.  Stress-induced hyperalgesia in α-2A knockout (KO) mice. (A  ) Paw withdrawal latencies from a 50°C hotplate in wild-type (WT) and α-2A KO mice after no stress (red bars  , n = 6) or ultrasonic stress (blue bars  , n = 12). (B  ) Paw withdrawal latencies in WT mice (n = 11) and α-2A KO mice (n = 5) tested once on a hotplate at various times after the initiation of 10-min ultrasonic stress. (C  ) Paw withdrawal latencies in α-2A KO mice after no stress (red bars  , n = 6) or ultrasonic stress (blue bars  , n = 6) on 3 consecutive days. The α-2A KO mice exhibit a prolonged nonhabituating hyperalgesia instead of analgesia in response to ultrasonic stress. *=P  < 0.05; ***=P  < 0.001, increase in latency versus  no stress (analgesia); +=P  < 0.05; +++=P  < 0.001, decrease in latency versus  no stress (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 2. 
	Stress-induced hyperalgesia in α-2A knockout (KO) mice. (A 
	) Paw withdrawal latencies from a 50°C hotplate in wild-type (WT) and α-2A KO mice after no stress (red bars 
	, n = 6) or ultrasonic stress (blue bars 
	, n = 12). (B 
	) Paw withdrawal latencies in WT mice (n = 11) and α-2A KO mice (n = 5) tested once on a hotplate at various times after the initiation of 10-min ultrasonic stress. (C 
	) Paw withdrawal latencies in α-2A KO mice after no stress (red bars 
	, n = 6) or ultrasonic stress (blue bars 
	, n = 6) on 3 consecutive days. The α-2A KO mice exhibit a prolonged nonhabituating hyperalgesia instead of analgesia in response to ultrasonic stress. *=P 
	< 0.05; ***=P 
	< 0.001, increase in latency versus 
	no stress (analgesia); +=P 
	< 0.05; +++=P 
	< 0.001, decrease in latency versus 
	no stress (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 2.  Stress-induced hyperalgesia in α-2A knockout (KO) mice. (A  ) Paw withdrawal latencies from a 50°C hotplate in wild-type (WT) and α-2A KO mice after no stress (red bars  , n = 6) or ultrasonic stress (blue bars  , n = 12). (B  ) Paw withdrawal latencies in WT mice (n = 11) and α-2A KO mice (n = 5) tested once on a hotplate at various times after the initiation of 10-min ultrasonic stress. (C  ) Paw withdrawal latencies in α-2A KO mice after no stress (red bars  , n = 6) or ultrasonic stress (blue bars  , n = 6) on 3 consecutive days. The α-2A KO mice exhibit a prolonged nonhabituating hyperalgesia instead of analgesia in response to ultrasonic stress. *=P  < 0.05; ***=P  < 0.001, increase in latency versus  no stress (analgesia); +=P  < 0.05; +++=P  < 0.001, decrease in latency versus  no stress (hyperalgesia). Data are expressed as mean ± SEM.
×
Fig. 3.  Deep wide dynamic range (WDR) neurons in α-2A knockout (KO) mice show enhanced windup response, compared with that in wild-type (WT) mice. Deep WDR neurons in α-2A KO (n = 62) and WT (n = 47) mice showed similar stimulus intensity-response functions of (A  ) A-fiber and (B  ) C-fiber–mediated responses to graded intracutaneous electrical stimuli applied to the receptive field (0.05–5.0 mA, 2.0 ms). Data are expressed as mean ± SEM number of action potentials (AP). (C  –E  ) C-component responses of deep WDR neurons in WT mice (n = 47) and in α-2A knockout mice (n = 62) to repetitive electrical stimulation (16 pulses, 3.0 mA, 2.0 ms) applied at frequencies of (C  ) 0.2 Hz, (D  ) 0.5 Hz, and (E  ) 1.0 Hz, respectively, are plotted against the stimulation number of each trial. The WDR neurons in α-2A knockout mice, but not in the WT mice, displayed windup to 0.2 Hz stimulation in addition to 0.5 Hz and 1.0 Hz stimulation. (F  ) The averaged C-fiber–mediated responses for stimulus 7–16 during the stimulation are plotted for various frequencies. Data are normalized by the response evoked by the first stimulation of each trial. **=P  < 0.01 and ***=P  < 0.001 versus  the input value; # =P  < 0.05 versus  the WT group. Data are expressed as mean ± SEM.
Fig. 3. 
	Deep wide dynamic range (WDR) neurons in α-2A knockout (KO) mice show enhanced windup response, compared with that in wild-type (WT) mice. Deep WDR neurons in α-2A KO (n = 62) and WT (n = 47) mice showed similar stimulus intensity-response functions of (A 
	) A-fiber and (B 
	) C-fiber–mediated responses to graded intracutaneous electrical stimuli applied to the receptive field (0.05–5.0 mA, 2.0 ms). Data are expressed as mean ± SEM number of action potentials (AP). (C  –E 
	) C-component responses of deep WDR neurons in WT mice (n = 47) and in α-2A knockout mice (n = 62) to repetitive electrical stimulation (16 pulses, 3.0 mA, 2.0 ms) applied at frequencies of (C 
	) 0.2 Hz, (D 
	) 0.5 Hz, and (E 
	) 1.0 Hz, respectively, are plotted against the stimulation number of each trial. The WDR neurons in α-2A knockout mice, but not in the WT mice, displayed windup to 0.2 Hz stimulation in addition to 0.5 Hz and 1.0 Hz stimulation. (F 
	) The averaged C-fiber–mediated responses for stimulus 7–16 during the stimulation are plotted for various frequencies. Data are normalized by the response evoked by the first stimulation of each trial. **=P 
	< 0.01 and ***=P 
	< 0.001 versus 
	the input value; # =P 
	< 0.05 versus 
	the WT group. Data are expressed as mean ± SEM.
Fig. 3.  Deep wide dynamic range (WDR) neurons in α-2A knockout (KO) mice show enhanced windup response, compared with that in wild-type (WT) mice. Deep WDR neurons in α-2A KO (n = 62) and WT (n = 47) mice showed similar stimulus intensity-response functions of (A  ) A-fiber and (B  ) C-fiber–mediated responses to graded intracutaneous electrical stimuli applied to the receptive field (0.05–5.0 mA, 2.0 ms). Data are expressed as mean ± SEM number of action potentials (AP). (C  –E  ) C-component responses of deep WDR neurons in WT mice (n = 47) and in α-2A knockout mice (n = 62) to repetitive electrical stimulation (16 pulses, 3.0 mA, 2.0 ms) applied at frequencies of (C  ) 0.2 Hz, (D  ) 0.5 Hz, and (E  ) 1.0 Hz, respectively, are plotted against the stimulation number of each trial. The WDR neurons in α-2A knockout mice, but not in the WT mice, displayed windup to 0.2 Hz stimulation in addition to 0.5 Hz and 1.0 Hz stimulation. (F  ) The averaged C-fiber–mediated responses for stimulus 7–16 during the stimulation are plotted for various frequencies. Data are normalized by the response evoked by the first stimulation of each trial. **=P  < 0.01 and ***=P  < 0.001 versus  the input value; # =P  < 0.05 versus  the WT group. Data are expressed as mean ± SEM.
×
Fig. 4.  α-2A Knockout (KO) mice show enhanced response to peripheral sensitizing agent. Dose-responses in wild-type (WT; red squares  ) and α-2A KO (blue circles  ) mice of intraperitoneal (IP) sulprostone effects on (A  ) tactile pain scores (n = 6, except n = 5 in 10 ng/kg−1KO group) and (B  ) thermal paw withdrawal latencies (n = 6, except n = 5 in 300 ng/kg−1WT group, n = 7 in 300 ng/kg−−1KO group, and n = 6 data from two experiments were combined for 30 ng kg–1WT and KO groups). Dose-responses in WT (red squares  ) and α-2A KO (blue circles  ) mice of intrathecal (IT) N  -methyl-d-aspartate (NMDA) effects on (C  ) tactile pain scores (n = 6, except n = 6 data from two experiments were combined for 100 ng/kg−1WT group), and (D  ) thermal paw withdrawal latencies (n = 6). The α-2A KO mice exhibit increased sensitivity to intraperitoneal sulprostone, but not intrathecal NMDA. §=P  < 0.001, increase in pain score versus  no drug (allodynia); ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no drug (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 4. 
	α-2A Knockout (KO) mice show enhanced response to peripheral sensitizing agent. Dose-responses in wild-type (WT; red squares 
	) and α-2A KO (blue circles 
	) mice of intraperitoneal (IP) sulprostone effects on (A 
	) tactile pain scores (n = 6, except n = 5 in 10 ng/kg−1KO group) and (B 
	) thermal paw withdrawal latencies (n = 6, except n = 5 in 300 ng/kg−1WT group, n = 7 in 300 ng/kg−−1KO group, and n = 6 data from two experiments were combined for 30 ng kg–1WT and KO groups). Dose-responses in WT (red squares 
	) and α-2A KO (blue circles 
	) mice of intrathecal (IT) N 
	-methyl-d-aspartate (NMDA) effects on (C 
	) tactile pain scores (n = 6, except n = 6 data from two experiments were combined for 100 ng/kg−1WT group), and (D 
	) thermal paw withdrawal latencies (n = 6). The α-2A KO mice exhibit increased sensitivity to intraperitoneal sulprostone, but not intrathecal NMDA. §=P 
	< 0.001, increase in pain score versus 
	no drug (allodynia); ++=P 
	< 0.01; +++=P 
	< 0.001, decrease in latency versus 
	no drug (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 4.  α-2A Knockout (KO) mice show enhanced response to peripheral sensitizing agent. Dose-responses in wild-type (WT; red squares  ) and α-2A KO (blue circles  ) mice of intraperitoneal (IP) sulprostone effects on (A  ) tactile pain scores (n = 6, except n = 5 in 10 ng/kg−1KO group) and (B  ) thermal paw withdrawal latencies (n = 6, except n = 5 in 300 ng/kg−1WT group, n = 7 in 300 ng/kg−−1KO group, and n = 6 data from two experiments were combined for 30 ng kg–1WT and KO groups). Dose-responses in WT (red squares  ) and α-2A KO (blue circles  ) mice of intrathecal (IT) N  -methyl-d-aspartate (NMDA) effects on (C  ) tactile pain scores (n = 6, except n = 6 data from two experiments were combined for 100 ng/kg−1WT group), and (D  ) thermal paw withdrawal latencies (n = 6). The α-2A KO mice exhibit increased sensitivity to intraperitoneal sulprostone, but not intrathecal NMDA. §=P  < 0.001, increase in pain score versus  no drug (allodynia); ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no drug (hyperalgesia). Data are expressed as mean ± SEM.
×
Fig. 5.  Systemic administration of prazosin attenuates windup levels without changing A-fiber and C-fiber–mediated responses of wide dynamic range (WDR) neurons to graded electrical stimulation in α-2A knockout (KO) mice. (A  and B  ) In α-2A KO mice, systemic administration of the α-1 receptor antagonist prazosin (0.1 μg/kg−1intraperitoneal) did not significantly change the (A  ) A-fiber and (B  ) C-fiber–mediated responses (number of action potentials, AP) of WDR neurons (n = 18) to graded electrical stimulation. (C  –E  ) Prazosin suppressed windup levels across (C  ) 0.2 Hz, (D  ) 0.5 Hz, and (E  ) 1.0 Hz stimulation in α-2A KO mice. (F  ) The averaged C-component responses for the stimulus 7–16 of the trial were also significantly reduced during 0.2, 0.5, and 1.0 Hz stimulation after prazosin treatment, compared with the preprazosin condition. Data are normalized by the response evoked by the first stimulation of each trial. # =P  < 0.05; ## =P  < 0.01; ### =P  < 0.001 versus  preprazosin condition. Data are expressed as mean ± SEM.
Fig. 5. 
	Systemic administration of prazosin attenuates windup levels without changing A-fiber and C-fiber–mediated responses of wide dynamic range (WDR) neurons to graded electrical stimulation in α-2A knockout (KO) mice. (A 
	and B 
	) In α-2A KO mice, systemic administration of the α-1 receptor antagonist prazosin (0.1 μg/kg−1intraperitoneal) did not significantly change the (A 
	) A-fiber and (B 
	) C-fiber–mediated responses (number of action potentials, AP) of WDR neurons (n = 18) to graded electrical stimulation. (C  –E 
	) Prazosin suppressed windup levels across (C 
	) 0.2 Hz, (D 
	) 0.5 Hz, and (E 
	) 1.0 Hz stimulation in α-2A KO mice. (F 
	) The averaged C-component responses for the stimulus 7–16 of the trial were also significantly reduced during 0.2, 0.5, and 1.0 Hz stimulation after prazosin treatment, compared with the preprazosin condition. Data are normalized by the response evoked by the first stimulation of each trial. # =P 
	< 0.05; ## =P 
	< 0.01; ### =P 
	< 0.001 versus 
	preprazosin condition. Data are expressed as mean ± SEM.
Fig. 5.  Systemic administration of prazosin attenuates windup levels without changing A-fiber and C-fiber–mediated responses of wide dynamic range (WDR) neurons to graded electrical stimulation in α-2A knockout (KO) mice. (A  and B  ) In α-2A KO mice, systemic administration of the α-1 receptor antagonist prazosin (0.1 μg/kg−1intraperitoneal) did not significantly change the (A  ) A-fiber and (B  ) C-fiber–mediated responses (number of action potentials, AP) of WDR neurons (n = 18) to graded electrical stimulation. (C  –E  ) Prazosin suppressed windup levels across (C  ) 0.2 Hz, (D  ) 0.5 Hz, and (E  ) 1.0 Hz stimulation in α-2A KO mice. (F  ) The averaged C-component responses for the stimulus 7–16 of the trial were also significantly reduced during 0.2, 0.5, and 1.0 Hz stimulation after prazosin treatment, compared with the preprazosin condition. Data are normalized by the response evoked by the first stimulation of each trial. # =P  < 0.05; ## =P  < 0.01; ### =P  < 0.001 versus  preprazosin condition. Data are expressed as mean ± SEM.
×
Fig. 6.  Inhibition of sympathetic outflow prevents stress-induced hyperalgesia in α-2A knockout (KO) mice. (A  –C  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in wild-type (WT) and α-2A KO mice after pretreatment with a saline control (n = 6) or the α-1 receptor antagonist prazosin, by (A  ) intraperitoneal (IP, 0.1 μg/kg−1; n = 6) or (B  ) intrathecal (10 ng; n = 6) injection, or (C  ) after guanethidine (guan) sympathectomy (n = 8, except n = 10 in guanethidine-treated KO group). (D  ) Tactile pain scores (n = 6, except n = 5 in 100, 300, 3,000 ng/kg−1KO groups) and (E  ) paw withdrawal latencies (n = 6, except n = 4 in 100 ng/kg−1KO group and n = 7 in 3,000 ng/kg−1KO groups) in response to IP sulprostone in WT and α-2A KO mice with guanethidine sympathectomy (green, WT; light blue, KO) compared with data without guanethidine sympathectomy from figures 4A  and B  (red, WT; blue, KO). Intraperitoneal prazosin and guanethidine sympathectomy prevent hyperalgesia in response to stress and sulprostone in α-2A KO mice. **=P  < 0.01; ***=P  < 0.001, increase in latency versus  no stress (analgesia); §=P  < 0.001, increase in pain score versus  no sulprostone (allodynia); +=P  < 0.05; ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no stress or versus  no sulprostone (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 6. 
	Inhibition of sympathetic outflow prevents stress-induced hyperalgesia in α-2A knockout (KO) mice. (A  –C 
	) Paw withdrawal latencies after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in wild-type (WT) and α-2A KO mice after pretreatment with a saline control (n = 6) or the α-1 receptor antagonist prazosin, by (A 
	) intraperitoneal (IP, 0.1 μg/kg−1; n = 6) or (B 
	) intrathecal (10 ng; n = 6) injection, or (C 
	) after guanethidine (guan) sympathectomy (n = 8, except n = 10 in guanethidine-treated KO group). (D 
	) Tactile pain scores (n = 6, except n = 5 in 100, 300, 3,000 ng/kg−1KO groups) and (E 
	) paw withdrawal latencies (n = 6, except n = 4 in 100 ng/kg−1KO group and n = 7 in 3,000 ng/kg−1KO groups) in response to IP sulprostone in WT and α-2A KO mice with guanethidine sympathectomy (green, WT; light blue, KO) compared with data without guanethidine sympathectomy from figures 4A 
	and B 
	(red, WT; blue, KO). Intraperitoneal prazosin and guanethidine sympathectomy prevent hyperalgesia in response to stress and sulprostone in α-2A KO mice. **=P 
	< 0.01; ***=P 
	< 0.001, increase in latency versus 
	no stress (analgesia); §=P 
	< 0.001, increase in pain score versus 
	no sulprostone (allodynia); +=P 
	< 0.05; ++=P 
	< 0.01; +++=P 
	< 0.001, decrease in latency versus 
	no stress or versus 
	no sulprostone (hyperalgesia). Data are expressed as mean ± SEM.
Fig. 6.  Inhibition of sympathetic outflow prevents stress-induced hyperalgesia in α-2A knockout (KO) mice. (A  –C  ) Paw withdrawal latencies after no stress (red bars  ) or ultrasonic stress (blue bars  ) in wild-type (WT) and α-2A KO mice after pretreatment with a saline control (n = 6) or the α-1 receptor antagonist prazosin, by (A  ) intraperitoneal (IP, 0.1 μg/kg−1; n = 6) or (B  ) intrathecal (10 ng; n = 6) injection, or (C  ) after guanethidine (guan) sympathectomy (n = 8, except n = 10 in guanethidine-treated KO group). (D  ) Tactile pain scores (n = 6, except n = 5 in 100, 300, 3,000 ng/kg−1KO groups) and (E  ) paw withdrawal latencies (n = 6, except n = 4 in 100 ng/kg−1KO group and n = 7 in 3,000 ng/kg−1KO groups) in response to IP sulprostone in WT and α-2A KO mice with guanethidine sympathectomy (green, WT; light blue, KO) compared with data without guanethidine sympathectomy from figures 4A  and B  (red, WT; blue, KO). Intraperitoneal prazosin and guanethidine sympathectomy prevent hyperalgesia in response to stress and sulprostone in α-2A KO mice. **=P  < 0.01; ***=P  < 0.001, increase in latency versus  no stress (analgesia); §=P  < 0.001, increase in pain score versus  no sulprostone (allodynia); +=P  < 0.05; ++=P  < 0.01; +++=P  < 0.001, decrease in latency versus  no stress or versus  no sulprostone (hyperalgesia). Data are expressed as mean ± SEM.
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Fig. 7.  Stress-induced hyperalgesic response in rats ablated by sympathectomy. (A  ) Paw withdrawal latencies of paws contralateral to 1 μg rauwolscine-injected paws after no stress (red bars  ) or ultrasonic stress (blue bars  ) in sham (n = 12 unstressed, 11 stressed) or surgically sympathectomized (n = 11 unstressed, 12 stressed) Sprague-Dawley rats. Stress-induced analgesia was unaffected by contralateral intraplantar rauwolscine injection or sympathectomy. (B  ) Paw withdrawal latencies of 1 μg rauwolscine-injected paw after no stress (red bars  ) or ultrasonic stress (blue bars  ) in sham (n = 12) or surgically sympathectomized (n = 13 unstressed, 12 stressed) Sprague-Dawley rats. Intraplantar rauwolscine blocked and sympathectomy restored a stress-induced analgesia response in the ipsilateral rauwolscine-treated paw. *=P  < 0.05; ***=P  < 0.001 versus  no stress (analgesia). Data are expressed as mean ± SEM.
Fig. 7. 
	Stress-induced hyperalgesic response in rats ablated by sympathectomy. (A 
	) Paw withdrawal latencies of paws contralateral to 1 μg rauwolscine-injected paws after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in sham (n = 12 unstressed, 11 stressed) or surgically sympathectomized (n = 11 unstressed, 12 stressed) Sprague-Dawley rats. Stress-induced analgesia was unaffected by contralateral intraplantar rauwolscine injection or sympathectomy. (B 
	) Paw withdrawal latencies of 1 μg rauwolscine-injected paw after no stress (red bars 
	) or ultrasonic stress (blue bars 
	) in sham (n = 12) or surgically sympathectomized (n = 13 unstressed, 12 stressed) Sprague-Dawley rats. Intraplantar rauwolscine blocked and sympathectomy restored a stress-induced analgesia response in the ipsilateral rauwolscine-treated paw. *=P 
	< 0.05; ***=P 
	< 0.001 versus 
	no stress (analgesia). Data are expressed as mean ± SEM.
Fig. 7.  Stress-induced hyperalgesic response in rats ablated by sympathectomy. (A  ) Paw withdrawal latencies of paws contralateral to 1 μg rauwolscine-injected paws after no stress (red bars  ) or ultrasonic stress (blue bars  ) in sham (n = 12 unstressed, 11 stressed) or surgically sympathectomized (n = 11 unstressed, 12 stressed) Sprague-Dawley rats. Stress-induced analgesia was unaffected by contralateral intraplantar rauwolscine injection or sympathectomy. (B  ) Paw withdrawal latencies of 1 μg rauwolscine-injected paw after no stress (red bars  ) or ultrasonic stress (blue bars  ) in sham (n = 12) or surgically sympathectomized (n = 13 unstressed, 12 stressed) Sprague-Dawley rats. Intraplantar rauwolscine blocked and sympathectomy restored a stress-induced analgesia response in the ipsilateral rauwolscine-treated paw. *=P  < 0.05; ***=P  < 0.001 versus  no stress (analgesia). Data are expressed as mean ± SEM.
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Fig. 8.  Model of stress-induced hyperalgesia. (1  ) Spinal α-2-adrenergic receptors on central terminals of sensory afferents and dorsal horn projection neurons mediate descending adrenergic inhibition, resulting in stress-induced analgesia. (2  ) Peripheral α-2 receptors on sympathetic postganglionic nerves (SPGNs) mediate feedback inhibition of norepinephrine release in response to stress. (3  ) In α-2A knockout mice or following treatment with α-2 antagonists (intraperitoneal or intraplantar), α-2 feedback inhibition is reduced, resulting in dysregulated (enhanced) norepinephrine release from SPGNs and sensitization of sensory afferents (4  ), which leads to stress-induced hyperalgesia when descending adrenergic inhibition is reduced. Role of α-1-adrenergic activation (4  ) in stress-induced hyperalgesia and decreased sensory afferent thresholds to repeated transcutaneous electrical stimuli was demonstrated by prazosin block. Role of SPGNs in stress-induced hyperalgesia and enhanced sensitivity of sensory afferents to prostaglandin E2receptor (EP) activation (4  ) was demonstrated by guanethidine depletion of norepinephrine and surgical sympathectomy. For simplicity, the α-1-adrenergic receptor is drawn on the sensory afferent, but sensitization could also be indirect via  another cell type such as a monocyte (5  ). Dysregulated sympathetic outflow (3  ) can result in a positive feedback loop between sensory afferents and sympathetic nerves via  spinal and supraspinal pathways when descending inhibition is reduced.
Fig. 8. 
	Model of stress-induced hyperalgesia. (1 
	) Spinal α-2-adrenergic receptors on central terminals of sensory afferents and dorsal horn projection neurons mediate descending adrenergic inhibition, resulting in stress-induced analgesia. (2 
	) Peripheral α-2 receptors on sympathetic postganglionic nerves (SPGNs) mediate feedback inhibition of norepinephrine release in response to stress. (3 
	) In α-2A knockout mice or following treatment with α-2 antagonists (intraperitoneal or intraplantar), α-2 feedback inhibition is reduced, resulting in dysregulated (enhanced) norepinephrine release from SPGNs and sensitization of sensory afferents (4 
	), which leads to stress-induced hyperalgesia when descending adrenergic inhibition is reduced. Role of α-1-adrenergic activation (4 
	) in stress-induced hyperalgesia and decreased sensory afferent thresholds to repeated transcutaneous electrical stimuli was demonstrated by prazosin block. Role of SPGNs in stress-induced hyperalgesia and enhanced sensitivity of sensory afferents to prostaglandin E2receptor (EP) activation (4 
	) was demonstrated by guanethidine depletion of norepinephrine and surgical sympathectomy. For simplicity, the α-1-adrenergic receptor is drawn on the sensory afferent, but sensitization could also be indirect via 
	another cell type such as a monocyte (5 
	). Dysregulated sympathetic outflow (3 
	) can result in a positive feedback loop between sensory afferents and sympathetic nerves via 
	spinal and supraspinal pathways when descending inhibition is reduced.
Fig. 8.  Model of stress-induced hyperalgesia. (1  ) Spinal α-2-adrenergic receptors on central terminals of sensory afferents and dorsal horn projection neurons mediate descending adrenergic inhibition, resulting in stress-induced analgesia. (2  ) Peripheral α-2 receptors on sympathetic postganglionic nerves (SPGNs) mediate feedback inhibition of norepinephrine release in response to stress. (3  ) In α-2A knockout mice or following treatment with α-2 antagonists (intraperitoneal or intraplantar), α-2 feedback inhibition is reduced, resulting in dysregulated (enhanced) norepinephrine release from SPGNs and sensitization of sensory afferents (4  ), which leads to stress-induced hyperalgesia when descending adrenergic inhibition is reduced. Role of α-1-adrenergic activation (4  ) in stress-induced hyperalgesia and decreased sensory afferent thresholds to repeated transcutaneous electrical stimuli was demonstrated by prazosin block. Role of SPGNs in stress-induced hyperalgesia and enhanced sensitivity of sensory afferents to prostaglandin E2receptor (EP) activation (4  ) was demonstrated by guanethidine depletion of norepinephrine and surgical sympathectomy. For simplicity, the α-1-adrenergic receptor is drawn on the sensory afferent, but sensitization could also be indirect via  another cell type such as a monocyte (5  ). Dysregulated sympathetic outflow (3  ) can result in a positive feedback loop between sensory afferents and sympathetic nerves via  spinal and supraspinal pathways when descending inhibition is reduced.
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