|Coordinate||119,638,705 bp (GRCm38)|
|Base Change||T ⇒ C (forward strand)|
|Gene Name||sodium channel, voltage-gated, type X, alpha|
|Chromosomal Location||119,608,456-119,719,032 bp (-)|
|MGI Phenotype||Homozygotes for a targeted null mutation exhibit impaired perception of pain.|
|Amino Acid Change||Threonine changed to Alanine|
|Institutional Source||Beutler Lab|
|Gene Model||not available|
|Predicted Effect||probably damaging
PolyPhen 2 Score 1.000 (Sensitivity: 0.00; Specificity: 1.00)
|Phenotypic Category||Autosomal Dominant|
|Alleles Listed at MGI|
|Mode of Inheritance||Autosomal Dominant|
|Local Stock||Embryos, Sperm, gDNA|
|Last Updated||2016-05-13 3:09 PM by Stephen Lyon|
After identification of the Possum mutation within the voltage-gated sodium channel α subunit Nav1.8, pain responses of Possum mice to various stimuli were examined since Nav1.8 is expressed in dorsal root ganglia (DRG) (4-7) where it functions to propagate nociceptive signaling in response to noxious cold, heat, and mechanical stimuli (8-10). Homozygous Possum mice displayed significantly increased sensitivity in the cold-plate test (Figure 1A). However, homozygous Possum and wild type mice exhibited similar latencies to paw withdrawal in the hot-plate test, demonstrating normal pain responses to heat stimuli (Figure 1B). Paw withdrawal responses elicited by von Frey filaments applied to the plantar surface did not differ between Possum and wild type mice, either before or after injection of complete Freund’s adjuvant into the paw (Figure 1C). None of the stimuli tested induced immobility in Possum mice. In addition, treatment of neonatal Possum mice with capsaicin to ablate TRPV1-expressing nociceptive C fibers did not abrogate scruffing-induced immobility, indicating that the phenotype is not a response to pain sensed by capsaicin-susceptible sensory neurons. Neither sudden immersion in cold water nor pinching of the tail or feet induced immobility in Possum mice.
In tests of conditioned fear elicited by foot shock paired with visual and auditory cues, Possum homozygotes displayed similar or reduced fear responses relative to wild-type mice (Figure 2). Foot shock alone did not induce the immobility phenotype.
Electroencephalographic (EEG) activity was measured in homozygous Possum mice before and after scruffing, and compared to that of wild type mice given the same treatment (Figure 3). During the baseline period before scruffing, frontal and parietal EEG patterns were similar in Possum and wild-type mice, with no epileptiform or other abnormal activity. Wild-type mice maintained an identical EEG pattern after scruffing. In contrast, scruffing of Possum homozygotes produced a shift in EEG activity from frequencies predominantly in the 4 to 10 Hz range (θ rhythm) during baseline recording to δ frequencies in the 1 to 4 Hz range concomitant with immobility. Coincident with recovery from immobility, EEG activity abruptly returned to and maintained baseline patterns indefinitely. Following a 5-min recovery period, scruffing again resulted in immobility and development of altered EEG activity similar to that observed during the first episode. These data implicate Nav1.8 in modulating the activity of CNS neurons. Measurements of evoked response potentials (ERP) to auditory stimuli in Possum mice suggested that although immobile, they are alert rather than unconscious (Figure 4).
Nav1.8 transcripts have been detected in the heart (11), and three studies reported association between common sequence variants of human SCN10A and prolongation of PR interval, P wave, and QRS complex on electrocardiogram (ECG) (11-13). ECG recordings from wild type and homozygous Possum mice before scruffing revealed similar heart rates (Figure 5A). In contrast, the heart rates of Possum mice were reduced by approximately 50% during the immobile period after scruffing relative to baseline heart rates (Figure 5A). The ECGs recorded for wild type and homozygous Possum mice showed no significant differences in PR interval, P wave duration, or QRS duration prior to scruffing. However, scruffing of Possum mice resulted in irregular RR intervals following clearly defined P waves (Figure 5B), consistent with sinus bradycardia with increased heart rate variability coincident with the Possum response. No significant ECG changes were observed following scruffing of wild type mice. The changes in heart rate and rhythm resolved as the mice became ambulatory. Since bradycardia can cause hypotension and loss of consciousness, the blood pressure of Possum mice was measured, but no fluctuation in blood pressure following scruffing was detected, indicating that immobility is not associated with or caused by changes in blood pressure (Figure 5C).
Since increased vagus nerve discharge can decrease heart rate and cause heart rate variability, we tested whether the bradycardia and marked RR variability in Possum mice resulted from increased vagal tone. Possum homozygotes were treated prior to scruffing with atropine, an anti-cholinergic drug that inhibits the action of the vagus nerve on the heart. Atropine prevented the reduction in heart rate (Figure 5A) and normalized cardiac rhythm during immobility (Figure 5B), but failed to prevent the Possum immobility response itself. No ECG changes were observed with scruffing or atropine administration in wild-type mice. Thus, whereas excessive vagal output to the heart is responsible for bradycardia and RR variability in Possum mice, it is not responsible for the tonic immobility induced by scruffing. Neither epinephrine nor propranolol, administered at large pharmacologic doses, abolished Possum behavior or induced it in wild-type mice.
Electrophysiological properties of the Nav1.8Possum channel
To understand how the Possum mutation affects the function of Nav1.8, whole cell voltage and current clamp methods were used to characterize Nav1.8 currents and excitability of acutely cultured homozygous Possum and wild-type small DRG sensory neurons (1). The Nav1.8 current was isolated from those of other channels, including the other TTX-resistant channel Nav1.9, and the voltage dependence and channel kinetics were determined for the parameters described in Table 1.
TTX-resistant Nav1.8-like currents expressed in homozygous Possum DRG neurons were 4-fold larger than those of wild-type DRG (Figure 6B & D; Table 1) (1). A 3.6-fold increase in ramp-induced inward current was also observed (-180±45 pA/pF (N=6); P=0.034). During long duration steps to subpeak voltages inactivation of Nav1.8-like currents in Possum neurons was impaired compared to that in wild-type neurons (Figure 6G) due to a 1.6-fold slowing of both fast and slow components of fast inactivation (Table 1) and a 2-fold increase in the proportion of the slow component (Figure 6H). There was a significant slowing of activation as well (time to peak, Table 1). No differences between Possum and wild-type DRG neurons were observed for V0.5,act, V0.5,inact, k values, deactivation rates, or recovery from fast or slow inactivation (Figure 6E & F; Table 1) (1). Therefore, the Possum mutation increases the current mediated by Nav1.8 channels by increasing the apparent current density and proportion of slow:fast components and slowing the kinetics of fast inactivation. Since these changes likely heighten the excitability of Nav1.8-expressing neurons, we performed current clamp recordings in the presence of TTX to determine whether Possum neurons are hyperexcitable. Although no detectable differences in resting potential, action potential duration, and membrane resistance were measured at -60 mV, the amount of depolarizing current required to elicit an action potential (rheobase) was profoundly decreased in Possum compared to wild-type neurons as was the voltage threshold, and the number of action potentials elicited during 150 and 900 ms injection of current at twice the rheobase. Thus, Possum small DRG neurons with long duration action potentials are hyperexcitable compared to those of littermate controls (1).
|Nature of Mutation|
The Possum mutation was mapped to Chromosome 9, and corresponds to an A to G transition at position 2403 of the Scn10a transcript, in exon 15 of 27 total exons.
The mutated nucleotide is indicated in red lettering, and results in a threonine to alanine change at residue 790 of the Nav1.8 protein.
The sodium channels form part of the ion channel superfamily that includes voltage-gated potassium and calcium channels. The 1957 amino acid protein Scn10a (also called PN3, SNS, and hereafter Nav1.8) is a voltage-gated sodium channel α subunit. The α subunit, of approximately 220-260 kD, is the pore-forming entity of sodium channels, and may be joined by one or more auxiliary β subunits that modify the kinetics and voltage dependence of channel gating, and regulate channel localization and interaction with cell adhesion molecules, extracellular matrix and cytoskeletal components (14). Nine proteins (referring to α subunits) comprise the mammalian sodium channel family, and all are greater than 50% identical in the transmembrane and extracellular domains, although the intracellular domains are not highly conserved [reviewed in (15)]. They are named by principal permeating ion (Na), principal physiological regulator (voltage, indicated as the abbreviated subscript, v), gene subfamily number (currently only 1), and specific channel isoform number (1-9, assigned based on the order in which they were identified). Splice variants are identified by lowercase letters following the channel isoform number. (See record for TremorD for a description of a Nav1.6 mutation.)
Nav1.8, like the other sodium channel α subunits, contains four homologous domains (I-IV) each consisting of six transmembrane α helices (S1-S6) (Figure 7) (5;6;16). A membrane-reentrant extracellular loop called the “pore loop” is located between the S5 and S6 helices in each of the four domains [see (15;17) and references therein for detailed information on sodium channel structure]. The pore loops line the outer, narrow entry to the pore, and each loop contains a pair of amino acids that form outer and inner rings serving as the ion selectivity filter in the outer pore of the channel. The outer ring of acidic residues is EEDD, while the inner ring is DEKA. A single amino acid residue in the pore loop of domain I determines the affinity of different sodium channels for the pore blocker tetrodotoxin. For example, rat cardiac sodium channels bind tetrodotoxin with 200-fold lower affinity than brain or skeletal sodium channels because of the substitution of an aromatic tyrosine or phenylalanine residue with cysteine (18;19). In Nav1.8, this position (amino acid 356) is occupied by a serine residue (2;4;5), which renders the channel tetrodotoxin-insensitive (IC50 ≈ 60-100 μM) (20). The S4 helices constitute the voltage sensors of the channel, and contain positively charged amino acid residues (arginine and/or lysine) at every third position. Depolarization of the membrane allows the S4 segments to move outward and initiate a conformational change that opens the pore. The short, intracellular loop between domain III, S6 and domain IV, S1 functions as the inactivation gate, which folds into the channel and blocks the pore from the inside during sustained depolarization of the membrane. A hydrophobic triad of isoleucine, phenylalanine and methionine (IFM) within this loop is critical for fast inactivation (see Background), and glycine and proline residues flanking the IFM motif serve as hinges to allow closure of the inactivation gate. The S5 and S6 helices line the inner, wider exit from the pore, and local anesthetics (e.g. procaine, etidocaine, lidocaine) and related antiepileptic (e.g. phenytoin) and antiarrhythmic drugs (e.g. lidocaine, quinidine) all bind from inside the cell to overlapping sites within this pore to block ionic current through the channel. Amino acids in the S6 segments from at least three of the four domains contribute to drug binding, with residues from the S6 helix of domain IV (F1764 and Y1771) being the most important (21;22). Together, these residues are thought to comprise the only known receptor site for local anesthetics.
The crystal structure of a voltage-gated Na+ channel (closed-pore conformation) from Arcobacter butzleri (NavAb) has been solved at 2.7Å resolution [Figure 8; PDB:3RVY & PDB: 3RW0 (23)]. NavAb is a member of the NaChBac bacterial channel family that is considered an ancestor of vertebrate Nav channels. Similar to other voltage-gated ion channels, NavAb has four subunits/domains that create an ion-conducting pore surrounded by voltage sensors (23). Payandeh et al. (2011) propose that the S1N helix and S2-S3 loop shield the intracellular surface of the voltage sensing domain and that the voltage-sensor domains and S4-S5 linkers dilate the central pore by pivoting together around a hinge at the base of the pore (23). The pore module of NavAb has an outer funnel-like vestibule, a selectivity filter, a central cavity, and an intracellular activation gate (23). The pore (P)-helices stabilize cations in the central cavity through helical-dipole interactions and the second pore-helix (P2-helix) forms an extracellular funnel in NavAb (23).
The Possum mutation is a threonine to alanine substitution at residue 790 of Nav1.8, located in the S5 helix of domain II, at the cytoplasmic interface of the channel.
Northern blot and RT-PCR analysis indicates that Nav1.8 is highly expressed in small-diameter sensory neurons of dorsal root and trigeminal ganglia, in both newborn and adult mice (5;6). Among dorsal root ganglion sensory neurons, Nav1.8 is predominantly expressed in nociceptive neurons with C fibers (89% positive for Nav1.8 immunoreactivity) or Aδ fibers (93% positive), and less in neurons with Aα/β fibers (21% of total neurons of this type positive) (7). Neurons with C fibers unresponsive to nociceptive stimuli also express Nav1.8 (7). C fibers (unmyelinated) and A fibers (myelinated) convey “slow” (0.5-2 m/s) and “fast” (3-75 m/s) pain signals from the skin, respectively. C fibers respond to thermal, mechanical, and chemical stimuli, as well as to changes in homeostasis of cardiovascular, respiratory, energy, and fluid systems (24). A fibers are divided into Aα/β and Aδ fibers, which respond to stretch stimuli or pressure, cold, and homeostatic stimuli, respectively.
Nav1.8 is not detected in other peripheral or central neurons, nor in glia or non-neuronal tissues. However, Nav1.8 mRNA and protein are expressed within cerebellar Purkinje cells in mice with experimental allergic encephalomyelitis (EAE), a model for multiple sclerosis, and in post-mortem tissue of humans with multiple sclerosis (25). The degree of upregulation of Nav1.8 expression positively correlates with EAE duration and worsening, and expression of Nav1.8 has been shown to perturb the firing patterns of cerebellar Purkinje cells (26;27). Abnormal Nav1.8 expression in the CNS has been hypothesized to contribute to clinical abnormalities such as ataxia in multiple sclerosis and EAE (25). Analysis of EST counts suggests that Nav1.8 is also expressed at low levels in the inner ear (3 Scn10a ESTs present out of a total pool of 38356 ESTs; data from UniGene’s EST ProfileViewer; UniGene Accession # 333688).
A recent report from Verkerk and colleagues examined NaV1.8 expression in the heart (28). They observed staining within intracardiac ganglia located in the pulmonary vein region; staining within the heart was less evident with most expression within the myocardium in between cardiomyocytes (28). Co-localization with neural proteins (i.e., Tubb3) indicates that NaV1.8 is localized to neural tissues within the myocardium (28). Examination of NaV1.8 localization in isolated intracardiac neurons found that NaV1.8 confirmed that NaV1.8 is expressed in neurons of the heart (28). Expression levels of NaV1.8 were variable within the intracardiac neurons. Furthermore, NaV1.8 was expressed in only a small subset of neurons of sympathetic origin; the majority of neurons are cholinergic in origin (28).
The voltage-gated sodium channels (VGSCs or Nav) mediate the rapid influx of sodium that underlies the depolarizing rising phase of action potentials in neurons and excitable cells [Figure 9 & 10; reviewed in (17)]. In a seminal paper, Hodgkin and Huxley demonstrated the three key features that now characterize the sodium channel: voltage-dependent activation, rapid inactivation, and selective ion conductance (29). VGSCs typically open (“activate”) within a millisecond in response to membrane depolarizations (Figure 10), often leading to a regenerative all or none depolarization typical of action potentials in neurons. Once activated, VGSCs do not remain open for long, and current through VGSCs can be terminated within approximately one millisecond by a process known as “fast inactivation” mediated by the intracellular inactivation gate folding into the channel and blocking the pore (see Protein Prediction). Recovery from inactivation occurs after the cell membrane potential is repolarized to negative membrane potentials (mediated by other ion channels), allowing sodium channels to return to the resting or closed state in which they are again ready to open in response to membrane depolarization.
Although all sodium channels generally function as described, distinct sodium channels differ in their precise functioning, and the sodium currents measured in various neuronal cell types are not homogeneous. In particular, inactivation kinetics can vary widely between distinct channel isoforms. Based on sensitivity to blockage by tetrodotoxin (TTX), a toxin found in the liver of the puffer fish, sodium channels are divided into two groups: TTX-sensitive channels that are typically fast inactivating (decay time from peak current <5 ms at room temperature), and TTX-resistant channels that are typically slowly inactivating (decay time from peak current 5-10 ms at room temperature). Central nervous system (CNS) neurons are known to express relatively homogeneous fast inactivating TTX-sensitive currents, while peripheral dorsal root ganglia neurons express currents containing both fast inactivating TTX-sensitive and slowly inactivating TTX-resistant components (30;31). It has been proposed that the slower TTX-resistant currents might serve to prolong the duration of the action potential to modulate neurotransmitter release.
The dorsal root ganglion (DRG) neurons of the peripheral nervous system project axons to the CNS, and serve to relay sensory information detected by dendrites innervating organs such as the skin, muscles, and internal organs to the CNS. Thus, DRG neurons sense and transmit information about pain (as well as other) sensations from the periphery, and are a large focus of pain research. Increased or decreased pain sensations can result from the altered electrical excitability of DRG neurons, and VGSCs, which determine the excitability of neurons, have been implicated in this process. Nav1.8 is a slowly inactivating TTX-resistant channel expressed in neurons of the dorsal root ganglia.
Targeted deletion of Nav1.8 in mice has provided insights into the specific role of Nav1.8 in pain states. Nav1.8-null mice display reduced thermo- and mechanoreceptive pain responses, and reduced responses to inflammatory pain stimuli in several tests (8;32). Slightly but significantly increased latencies are observed in the paw-withdrawal and tail-flick responses to a radiant heat stimulus, although latency in the hot plate test is similar between mutants and wild type animals. Pain thresholds in the tail pressure test are increased in Nav1.8-null mice. Mutant mice show reduced thermal hyperalgesia induced by inflammatory stimuli such as intraplantar injection of carrageenan or systemic injection of nerve growth factor (8;32). In these tests, injection of the inflammatory stimulus decreases paw-flick latency to heat applied to the paw; Nav1.8-null mice display a slightly longer paw-flick latency compared to wild type animals. Electrophysiological analyses demonstrate that small DRG neurons from Nav1.8-null mice are less likely to fire action potentials, consistent with the analgesia observed in behavioral studies (33). However, Nav1.8-deficient small DRG neurons have also been reported to exhibit lowered thresholds of electrical activation and increased current densities of TTX-sensitive channels (8). These may be compensatory changes for the lack of Nav1.8 (8).
Nav1.8 is required for sensing cold pain and pain in the cold (10). Electrophysiological recordings from cold-sensitive neurons innervating the skin demonstrate that TTX-sensitive VGSCs become inactive at low temperatures, while the inactivation properties of Nav1.8 are cold-resistant. Responsiveness to mechanical stimulation at low temperatures is impaired in neurons lacking Nav1.8. Nav1.8-null mice display greatly reduced foot-lifting behavior relative to wild type mice in the cold-plate test, in which animals are placed on a plate held at 0° C. Thus, Nav1.8 function is critical and may be specialized for perception of cold pain and pain in the cold.
In addition to a role in primary pain states, Nav1.8 has been implicated in neuropathic pain, although this function remains controversial. Neuropathic pain is chronic pain such as shooting or burning pain, or tingling and numbness, and is frequently induced by tissue and nerve damage. Neuropathic pain is hypothesized to result from the spontaneous firing of pain-sensing neurons, in part due to the aberrant expression and function of VGSCs. Spontaneous activity in damaged sensory neurons is reportedly reduced in Nav1.8-null mice relative to wild type (34), and knockdown of Nav1.8 has been shown to reverse neuropathic pain induced by spinal nerve injury in rats (35). However, other studies have found no role for Nav1.8 in neuropathic pain (32;36). In addition, Nav1.8 mRNA and protein expression in axotomized small DRG neurons are dramatically reduced in models of neuropathic pain (37;38). It has been suggested that compensatory changes in expression of other channels may support the ectopic firing of injured neurons, or that altered Nav1.8 activity in uninjured neurons contributes to their hyperactivity, both possibilities that may lead to development of neuropathic pain.
Nav1.8 does appear to modulate neuropathic pain caused by mutations in the Nav1.7 channel. Nav1.7 is expressed in small DRG neurons (39), and exhibits TTX sensitivity, as well as rapid activation and inactivation properties (40). These channels likely contribute the predominant TTX-sensitive current found in small DRG neurons (41). Strikingly, nonsense mutations in Nav1.7 result in a complete lack of pain sensation in humans that appear otherwise healthy, except for deficits in olfaction in some patients (42;43) (OMIM *603415, #243000). Similarly, selective deletion of Nav1.7 in small DRG neurons in mice (using a Cre-lox system in which Cre is expressed from the Nav1.8 promoter) reduces mechanical and thermal hypersensitivity associated with acute or inflammatory pain (44). Mice completely lacking Nav1.7 die just after birth because of a failure to feed, possibly due to anosmia or hyposmia similar to that documented in human patients (44). Conversely, point mutations that alter the gating properties of Nav1.7 can cause increased pain sensations and neuropathy, as in inherited erythromelalgia (also called erythermalgia, OMIM #133020) for which the primary symptom is severe chronic burning pain sensations in the hands and feet. The disease is caused by Nav1.7 mutations that increase neuronal hyperexcitability, for example by causing hyperpolarizing shifts in the voltage-dependence of channel activation, thereby lowering the threshold of the neurons for firing action potentials (45). Nav1.8 channels have been shown to contribute to the hyperexcitability of DRG neurons with mutant Nav1.7 channels. The erythromelalgia mutation L858H produces a depolarizing shift in resting membrane potential and decreases action potential threshold in DRG neurons (46). This hyperexcitability is supported by the presence of Nav1.8, which, due to its depolarized voltage-dependence of activation and inactivation, permits the neurons to generate action potentials and sustain repetitive firing despite a depolarized resting membrane potential. Superior cervical ganglion neurons do not express Nav1.8, and the same Nav1.7 mutation depolarizes the resting membrane potential but renders these cells hypoexcitable.
The Possum mutation, a threonine to alanine substitution in transmembrane helix S5 in domain II, alters the physiology of Nav1.8 channels by increasing current density and slowing the kinetics of inactivation. Precedent exists for the hyperactivation of sodium channels by dominant missense mutations located adjacent to the cytoplasmic leaflet of the plasma membrane lipid bilayer. Hyperkalemic periodic paralysis syndrome (HYPP, OMIM #170500) is caused by mutations in SCN4A, encoding the skeletal muscle sodium channel Nav1.4 (47). The disease is an autosomal dominant disorder characterized by temporary limb weakness that occurs spontaneously or is triggered by rest after exercise, consumption of potassium-rich foods, stress or fatigue (48). A progressive, fixed, interattack weakness may also develop in some patients. The two most common mutations causing HYPP are T704M and M1592V, accounting for 75% of all cases (48). The threonine to methionine substitution at position 704 of human Nav1.4, hyperactivates the channel by shifting the voltage-dependence of activation in the hyperpolarizing direction and dramatically impairing slow inactivation (49). The gain-of-function mutation is dominant because only a small amount of noninactivating sodium current is sufficient to cause repetitive firing and steady depolarization of muscle cells leading to periodic paralysis. Notably, T704 of Nav1.4 is orthologous to T790 of Nav1.8 on sequence alignment.
Similar dominant mutations in human Nav1.7 cause erythromelalgia by increasing neuronal hyperexcitability. When their sequences are aligned, the L858H mutation of Nav1.7 would lie adjacent to the threonine mutated in Possum (it would correspond to L789 of mouse Nav1.8). Nav1.7 L858 is the last amino acid of the linker between helices S4 and S5 in domain II. The L858H mutation shifts the voltage-dependence of activation in the hyperpolarizing direction and also slows the deactivation time of the channel (50). Another mutation, A863P (within domain II, helix 5, four amino acids from the Possum mutation in the corresponding Nav1.8 sequence), causes the same types of defects in channel function, again resulting in hyperexcitability of neurons (51).
The threonine mutated in Possum is conserved in all nine of the known VGSCs in both human and mouse, as are at least 7 of the 10 surrounding amino acids. It is likely that alanine, which is nonpolar and hydrophobic, fails to form the electrostatic interactions normally mediated by the polar threonine residue, thereby changing channel conformation and properties. Another factor that may be involved in the effect of the Possum mutation is the change in size of the amino acid side chain. Side chain size of S241 in the domain I S4-S5 linker of Nav1.7 was found to be a critical determinant of channel properties (52).
The normal responses of Possum mice to noxious heat and punctate mechanical stimuli argue against the idea that excessive pain exists and that it triggers the immobility phenotype in scruffed Possum mice. Among DRG, Nav1.8 is predominantly expressed in nociceptive neurons with C fibers and Aδ fibers, and less in neurons with Aα/β fibers (7). Nociceptive C fibers ablated by capsaicin are not required for the induction of immobility in Possum mice. Thus, sensory fibers resistant to neonatal capsaicin ablation, which include Aδ fibers and Mrgprd+ mechanosensitive C fibers (53), may instead play an integral role in the immobility response to scruffing, and may be necessary and sufficient for sensing and propagating the signals induced by such physical manipulation. However, it cannot be ruled out that developmental compensatory mechanisms impart susceptibility to the immobility phenotype, or that the phenotype is mediated by events other than acute activation of mutant Nav1.8 channels in nociceptors during scruffing.
It was reported previously that nonsynonymous coding sequence variants of human SCN10A are associated with increased PR interval, P wave duration, and QRS duration in ECGs, and that Nav1.8-deficient mice have decreased PR intervals (11-13). Scruffed Possum mice experienced vagus nerve-stimulated sinus bradycardia and highly irregular RR intervals on ECG concomitant with immobility. These data do not permit us to discern whether the effects of Nav1.8Possum on cardiac conduction are intrinsic to cardiomyocytes or secondary to neurotransmission via DRG neurons. Expression and localization analysis by Verkerk et al. (2012) indicate that the expression of Nav1.8 is predominant in intracardiac neurons; expression in cardiomyoctes was not detected (28). Furthermore, Verkerk et al. (2012) show that Nav1.8 within the intracardiac neurons regulates neuronal action potential firing frequency (28). The pathways leading the effects on cardiac conduction remain unclear. Verkerk et al. (2012) speculate that the neurons that are controlled by Nav1.8 regulate the release of neurotransmitters and/or neuropeptides (28). The neurotransmitters/neuropeptides can subsequently act by a direct effect on a myocyte or indirectly through other neurons. Observation of normal blood pressures during immobility and the inability to block immobility with atropine support the conclusion that the cardiac abnormalities are independent of the behavioral Possum phenotype. The ability to restore normal cardiac rhythm and prevent bradycardia using atropine demonstrates the existence of a novel reflex arc activated by a discrete stimulus (scruffing), and having as one output a strong vagal response.
Neither excessive pain nor altered cardiac conduction was responsible for the immobility phenotype, yet the mechanistic basis of the behavior remains unknown. We hypothesize that scruffing-induced immobility in Possum mice is equivalent to the phenomenon of manipulation-induced tonic immobility or pinch-induced catalepsy reported to result from repeated pinching of the scruff of mice (54;55). Although no quantitative standard exists to define tonic immobility, experimentally induced tonic immobility is well accepted to be induced by some form of physical restraint, and to be characterized by a transient state of enhanced muscular rigidity, ‘waxy flexibility’, and altered EEG patterns indicative of enhanced alertness (56-58), that terminate abruptly after varying duration (2;3), exactly as observed in Possum mutants. Existing data support a genetic basis for tonic immobility (59), but genes contributing to this behavior, whether experimentally or naturally induced, have not been identified. In addition, no class of sensory neurons has previously been implicated in this response. Sodium conduction in DRG neurons, occurring via Nav1.8, may be one factor responsible for this behavior.
Although the neural substrates of manipulation-induced tonic immobility remain poorly defined, evidence suggests that they include the brainstem (60), particularly the parabrachial region (PB) (61), and the ventrolateral periaqueductal gray (PAG) (62;63) that, respectively, relay nociceptive information to the cortex and amygdala, and modulate sensory afferent output from the spinal cord. Dopaminergic, cholinergic, GABAergic, and opioid signaling in these and other areas are thought to mediate manipulation-induced tonic immobility (63;64). It may be that scruffing, an arguably intense stimulus, super-activates these nuclei through stimulation of DRG neurons rendered hyperexcitable by Nav1.8Possum and leads to the dramatic immobility observed in Possum mice. The sensitivity of the scruff to stimulation leading to immobility may reflect the evolutionarily ancient underpinnings of this behavior, which is thought to represent an antipredatory action that reduces both the appeal and detection of prey by predators (2;65). Possum mice represent a novel animal model for studying this state, which has been variable and difficult to elicit in mice.
Altered EEG patterns, observed only during immobility, also raise the possibility of direct function(s) for Nav1.8 in CNS neurons, which may contribute mechanistically to the behavior. Although brain expression of Nav1.8 has not been reported (4-7), small amounts or highly localized expression below the level of detection by standard assays cannot be ruled out.
|Primers||Primers cannot be located by automatic search.|
Possum genotyping is performed by amplifying the region containing the mutation using PCR, followed by sequencing of the amplified region to detect the single nucleotide transition.
Possum (F): 5’-TGAAACAGATGGCAGACAAGCCTC -3’
Possum (R): 5’- GCCTAGCACCATCACTGTCAAGAAG -3’
1) 95°C 2:00
2) 95°C 0:30
3) 56°C 0:30
4) 72°C 1:00
5) repeat steps (2-4) 29X
6) 72°C 7:00
7) 4°C ∞
Primers for sequencing
Possum_seq(F): 5’- TCAATTTAGCGACCACTGGAAG -3’
Possum_seq(R): 5’- AGATGTAGTCCTGGCTGACCTC -3’
The following sequence of 602 nucleotides (from Genbank genomic region NC_000075 for linear genomic sequence of Scn10a) is amplified:
55321 agatggcaga caagcctcac taatgtgagg ccctggatct gccagttggt ggagtacatt
55381 tcaatttagc gaccactgga aggtgatcag agctctgagt gagatgtaaa aagaaaagtc
55441 tccacaaaca gccccacccc aaactcatga gatgtcttgg tgcttgtccc acaagcttgg
55501 cttccagtga agacttcagt tatgagatgg tgagaagaga cctgagacag tgtctctttc
55561 cacagcttcg ggtcttcaag ctggccaagt cctggcccac cctgaacatg ctcatcaaga
55621 tcatcgggaa ctctgtgggg gccctgggca acctgacctt catcctggcc atcatcgtct
55681 ttatcttcgc cctggtggga aagcagctcc tctcagagaa ctatgggtgc cgcagggatg
55741 gcatctccgt gtggaatggt gagaggctgc gctggcacat gtgtgacttc ttccattcct
55801 tcctcgtcgt cttccggatc ctctgcgggg agtggatcga gaacatgtgg gtctgcatgg
55861 aggtcagcca ggactacatc tgcctcaccc tcttcttgac agtgatggtg ctaggc
Primer binding sites are underlined; sequencing primer binding sites are highlighted in gray; the mutated A is indicated in red.
1. Blasius, A. L., Dubin, A. E., Petrus, M. J., Lim, B. K., Narezkina, A., Criado, J. R., Wills, D. N., Xia, Y., Moresco, E. M., Ehlers, C., Knowlton, K. U., Patapoutian, A., and Beutler, B. (2011) Hypermorphic Mutation of the Voltage-Gated Sodium Channel Encoding Gene Scn10a Causes a Dramatic Stimulus-Dependent Neurobehavioral Phenotype. Proc. Natl. Acad. Sci. U. S. A.. 108, 19413-19418.
2. Gallup, G. G.,Jr. (1974) Animal Hypnosis: Factual Status of a Fictional Concept. Psychol. Bull.. 81, 836-853.
3. Klemm, W. R. (2001) Behavioral Arrest: In Search of the Neural Control System. Prog. Neurobiol.. 65, 453-471.
4. Novakovic, S. D., Tzoumaka, E., McGivern, J. G., Haraguchi, M., Sangameswaran, L., Gogas, K. R., Eglen, R. M., and Hunter, J. C. (1998) Distribution of the Tetrodotoxin-Resistant Sodium Channel PN3 in Rat Sensory Neurons in Normal and Neuropathic Conditions. J. Neurosci.. 18, 2174-2187.
5. Akopian, A. N., Sivilotti, L., and Wood, J. N. (1996) A Tetrodotoxin-Resistant Voltage-Gated Sodium Channel Expressed by Sensory Neurons. Nature. 379, 257-262.
6. Sangameswaran, L., Delgado, S. G., Fish, L. M., Koch, B. D., Jakeman, L. B., Stewart, G. R., Sze, P., Hunter, J. C., Eglen, R. M., and Herman, R. C. (1996) Structure and Function of a Novel Voltage-Gated, Tetrodotoxin-Resistant Sodium Channel Specific to Sensory Neurons. J. Biol. Chem.. 271, 5953-5956.
7. Djouhri, L., Fang, X., Okuse, K., Wood, J. N., Berry, C. M., and Lawson, S. N. (2003) The TTX-Resistant Sodium Channel Nav1.8 (SNS/PN3): Expression and Correlation with Membrane Properties in Rat Nociceptive Primary Afferent Neurons. J. Physiol.. 550, 739-752.
8. Akopian, A. N., Souslova, V., England, S., Okuse, K., Ogata, N., Ure, J., Smith, A., Kerr, B. J., McMahon, S. B., Boyce, S., Hill, R., Stanfa, L. C., Dickenson, A. H., and Wood, J. N. (1999) The Tetrodotoxin-Resistant Sodium Channel SNS has a Specialized Function in Pain Pathways. Nat. Neurosci.. 2, 541-548.
9. Abrahamsen, B., Zhao, J., Asante, C. O., Cendan, C. M., Marsh, S., Martinez-Barbera, J. P., Nassar, M. A., Dickenson, A. H., and Wood, J. N. (2008) The Cell and Molecular Basis of Mechanical, Cold, and Inflammatory Pain. Science. 321, 702-705.
10. Zimmermann, K., Leffler, A., Babes, A., Cendan, C. M., Carr, R. W., Kobayashi, J., Nau, C., Wood, J. N., and Reeh, P. W. (2007) Sensory Neuron Sodium Channel Nav1.8 is Essential for Pain at Low Temperatures. Nature. 447, 855-858.
11. Chambers, J. C., Zhao, J., Terracciano, C. M., Bezzina, C. R., Zhang, W., Kaba, R., Navaratnarajah, M., Lotlikar, A., Sehmi, J. S., Kooner, M. K., Deng, G., Siedlecka, U., Parasramka, S., El-Hamamsy, I., Wass, M. N., Dekker, L. R., de Jong, J. S., Sternberg, M. J., McKenna, W., Severs, N. J., de Silva, R., Wilde, A. A., Anand, P., Yacoub, M., Scott, J., Elliott, P., Wood, J. N., and Kooner, J. S. (2010) Genetic Variation in SCN10A Influences Cardiac Conduction. Nat. Genet.. 42, 149-152.
12. Holm, H., Gudbjartsson, D. F., Arnar, D. O., Thorleifsson, G., Thorgeirsson, G., Stefansdottir, H., Gudjonsson, S. A., Jonasdottir, A., Mathiesen, E. B., Njolstad, I., Nyrnes, A., Wilsgaard, T., Hald, E. M., Hveem, K., Stoltenberg, C., Lochen, M. L., Kong, A., Thorsteinsdottir, U., and Stefansson, K. (2010) Several Common Variants Modulate Heart Rate, PR Interval and QRS Duration. Nat. Genet.. 42, 117-122.
13. Pfeufer, A., van Noord, C., Marciante, K. D., Arking, D. E., Larson, M. G., Smith, A. V., Tarasov, K. V., Muller, M., Sotoodehnia, N., Sinner, M. F., Verwoert, G. C., Li, M., Kao, W. H., Kottgen, A., Coresh, J., Bis, J. C., Psaty, B. M., Rice, K., Rotter, J. I., Rivadeneira, F., Hofman, A., Kors, J. A., Stricker, B. H., Uitterlinden, A. G., van Duijn, C. M., Beckmann, B. M., Sauter, W., Gieger, C., Lubitz, S. A., Newton-Cheh, C., Wang, T. J., Magnani, J. W., Schnabel, R. B., Chung, M. K., Barnard, J., Smith, J. D., Van Wagoner, D. R., Vasan, R. S., Aspelund, T., Eiriksdottir, G., Harris, T. B., Launer, L. J., Najjar, S. S., Lakatta, E., Schlessinger, D., Uda, M., Abecasis, G. R., Muller-Myhsok, B., Ehret, G. B., Boerwinkle, E., Chakravarti, A., Soliman, E. Z., Lunetta, K. L., Perz, S., Wichmann, H. E., Meitinger, T., Levy, D., Gudnason, V., Ellinor, P. T., Sanna, S., Kaab, S., Witteman, J. C., Alonso, A., Benjamin, E. J., and Heckbert, S. R. (2010) Genome-Wide Association Study of PR Interval. Nat. Genet.. 42, 153-159.
14. Isom, L. L. (2001) Sodium Channel Beta Subunits: Anything but Auxiliary. Neuroscientist. 7, 42-54.
15. Catterall, W. A., Goldin, A. L., and Waxman, S. G. (2005) International Union of Pharmacology. XLVII. Nomenclature and Structure-Function Relationships of Voltage-Gated Sodium Channels. Pharmacol. Rev.. 57, 397-409.
16. Souslova, V. A., Fox, M., Wood, J. N., and Akopian, A. N. (1997) Cloning and Characterization of a Mouse Sensory Neuron Tetrodotoxin-Resistant Voltage-Gated Sodium Channel Gene, Scn10a. Genom.. 41, 201-209.
17. Catterall, W. A. (2000) From Ionic Currents to Molecular Mechanisms: The Structure and Function of Voltage-Gated Sodium Channels. Neuron. 26, 13-25.
18. Backx, P. H., Yue, D. T., Lawrence, J. H., Marban, E., and Tomaselli, G. F. (1992) Molecular Localization of an Ion-Binding Site within the Pore of Mammalian Sodium Channels. Science. 257, 248-251.
19. Satin, J., Kyle, J. W., Chen, M., Bell, P., Cribbs, L. L., Fozzard, H. A., and Rogart, R. B. (1992) A Mutant of TTX-Resistant Cardiac Sodium Channels with TTX-Sensitive Properties. Science. 256, 1202-1205.
20. Sivilotti, L., Okuse, K., Akopian, A. N., Moss, S., and Wood, J. N. (1997) A Single Serine Residue Confers Tetrodotoxin Insensitivity on the Rat Sensory-Neuron-Specific Sodium Channel SNS. FEBS Lett.. 409, 49-52.
21. Ragsdale, D. S., McPhee, J. C., Scheuer, T., and Catterall, W. A. (1996) Common Molecular Determinants of Local Anesthetic, Antiarrhythmic, and Anticonvulsant Block of Voltage-Gated Na+ Channels. Proc. Natl. Acad. Sci. U. S. A.. 93, 9270-9275.
22. Ragsdale, D. S., McPhee, J. C., Scheuer, T., and Catterall, W. A. (1994) Molecular Determinants of State-Dependent Block of Na+ Channels by Local Anesthetics. Science. 265, 1724-1728.
23. Payandeh, J., Scheuer, T., Zheng, N., and Catterall, W. A. (2011) The Crystal Structure of a Voltage-Gated Sodium Channel. Nature. 475, 353-358.
24. Craig, A. D. (2003) Interoception: The Sense of the Physiological Condition of the Body. Curr. Opin. Neurobiol.. 13, 500-505.
25. Black, J. A., Dib-Hajj, S., Baker, D., Newcombe, J., Cuzner, M. L., and Waxman, S. G. (2000) Sensory Neuron-Specific Sodium Channel SNS is Abnormally Expressed in the Brains of Mice with Experimental Allergic Encephalomyelitis and Humans with Multiple Sclerosis. Proc. Natl. Acad. Sci. U. S. A.. 97, 11598-11602.
26. Craner, M. J., Kataoka, Y., Lo, A. C., Black, J. A., Baker, D., and Waxman, S. G. (2003) Temporal Course of Upregulation of Na(v)1.8 in Purkinje Neurons Parallels the Progression of Clinical Deficit in Experimental Allergic Encephalomyelitis. J. Neuropathol. Exp. Neurol.. 62, 968-975.
27. Renganathan, M., Gelderblom, M., Black, J. A., and Waxman, S. G. (2003) Expression of Nav1.8 Sodium Channels Perturbs the Firing Patterns of Cerebellar Purkinje Cells. Brain Res.. 959, 235-242.
28. Verkerk, A. O., Remme, C. A., Schumacher, C. A., Scicluna, B. P., Wolswinkel, R., de Jonge, B., Bezzina, C. R., and Veldkamp, M. W. (2012) Functional NaV1.8 Channels in Intracardiac Neurons: The Link between SCN10A and Cardiac Electrophysiology. Circ. Res.. 111, 333-343.
29. HODGKIN, A. L., and HUXLEY, A. F. (1952) A Quantitative Description of Membrane Current and its Application to Conduction and Excitation in Nerve. J. Physiol.. 117, 500-544.
30. Kostyuk, P. G., Veselovsky, N. S., and Tsyndrenko, A. Y. (1981) Ionic Currents in the Somatic Membrane of Rat Dorsal Root Ganglion Neurons-I. Sodium Currents. Neuroscience. 6, 2423-2430.
31. Roy, M. L., and Narahashi, T. (1992) Differential Properties of Tetrodotoxin-Sensitive and Tetrodotoxin-Resistant Sodium Channels in Rat Dorsal Root Ganglion Neurons. J. Neurosci.. 12, 2104-2111.
32. Kerr, B. J., Souslova, V., McMahon, S. B., and Wood, J. N. (2001) A Role for the TTX-Resistant Sodium Channel Nav 1.8 in NGF-Induced Hyperalgesia, but Not Neuropathic Pain. Neuroreport. 12, 3077-3080.
33. Renganathan, M., Cummins, T. R., and Waxman, S. G. (2001) Contribution of Na(v)1.8 Sodium Channels to Action Potential Electrogenesis in DRG Neurons. J. Neurophysiol.. 86, 629-640.
34. Roza, C., Laird, J. M., Souslova, V., Wood, J. N., and Cervero, F. (2003) The Tetrodotoxin-Resistant Na+ Channel Nav1.8 is Essential for the Expression of Spontaneous Activity in Damaged Sensory Axons of Mice. J. Physiol. 550, 921-926.
35. Lai, J., Gold, M. S., Kim, C. S., Bian, D., Ossipov, M. H., Hunter, J. C., and Porreca, F. (2002) Inhibition of Neuropathic Pain by Decreased Expression of the Tetrodotoxin-Resistant Sodium Channel, NaV1.8. Pain. 95, 143-152.
36. Nassar, M. A., Levato, A., Stirling, L. C., and Wood, J. N. (2005) Neuropathic Pain Develops Normally in Mice Lacking both Nav1.7 and Nav1.8. Mol. Pain. 1, 24.
37. Cummins, T. R., and Waxman, S. G. (1997) Downregulation of Tetrodotoxin-Resistant Sodium Currents and Upregulation of a Rapidly Repriming Tetrodotoxin-Sensitive Sodium Current in Small Spinal Sensory Neurons After Nerve Injury. J. Neurosci.. 17, 3503-3514.
38. Dib-Hajj, S., Black, J. A., Felts, P., and Waxman, S. G. (1996) Down-Regulation of Transcripts for Na Channel Alpha-SNS in Spinal Sensory Neurons Following Axotomy. Proc. Natl. Acad. Sci. U. S. A.. 93, 14950-14954.
39. Djouhri, L., Newton, R., Levinson, S. R., Berry, C. M., Carruthers, B., and Lawson, S. N. (2003) Sensory and Electrophysiological Properties of Guinea-Pig Sensory Neurones Expressing Nav 1.7 (PN1) Na+ Channel Alpha Subunit Protein. J. Physiol. 546, 565-576.
40. Klugbauer, N., Lacinova, L., Flockerzi, V., and Hofmann, F. (1995) Structure and Functional Expression of a New Member of the Tetrodotoxin-Sensitive Voltage-Activated Sodium Channel Family from Human Neuroendocrine Cells. EMBO J.. 14, 1084-1090.
41. Cummins, T. R., Howe, J. R., and Waxman, S. G. (1998) Slow Closed-State Inactivation: A Novel Mechanism Underlying Ramp Currents in Cells Expressing the hNE/PN1 Sodium Channel. J. Neurosci.. 18, 9607-9619.
42. Cox, J. J., Reimann, F., Nicholas, A. K., Thornton, G., Roberts, E., Springell, K., Karbani, G., Jafri, H., Mannan, J., Raashid, Y., Al-Gazali, L., Hamamy, H., Valente, E. M., Gorman, S., Williams, R., McHale, D. P., Wood, J. N., Gribble, F. M., and Woods, C. G. (2006) An SCN9A Channelopathy Causes Congenital Inability to Experience Pain. Nature. 444, 894-898.
43. Goldberg, Y. P., MacFarlane, J., MacDonald, M. L., Thompson, J., Dube, M. P., Mattice, M., Fraser, R., Young, C., Hossain, S., Pape, T., Payne, B., Radomski, C., Donaldson, G., Ives, E., Cox, J., Younghusband, H. B., Green, R., Duff, A., Boltshauser, E., Grinspan, G. A., Dimon, J. H., Sibley, B. G., Andria, G., Toscano, E., Kerdraon, J., Bowsher, D., Pimstone, S. N., Samuels, M. E., Sherrington, R., and Hayden, M. R. (2007) Loss-of-Function Mutations in the Nav1.7 Gene Underlie Congenital Indifference to Pain in Multiple Human Populations. Clin. Genet.. 71, 311-319.
44. Nassar, M. A., Stirling, L. C., Forlani, G., Baker, M. D., Matthews, E. A., Dickenson, A. H., and Wood, J. N. (2004) Nociceptor-Specific Gene Deletion Reveals a Major Role for Nav1.7 (PN1) in Acute and Inflammatory Pain. Proc. Natl. Acad. Sci. U. S. A.. 101, 12706-12711.
45. Dib-Hajj, S. D., Rush, A. M., Cummins, T. R., Hisama, F. M., Novella, S., Tyrrell, L., Marshall, L., and Waxman, S. G. (2005) Gain-of-Function Mutation in Nav1.7 in Familial Erythromelalgia Induces Bursting of Sensory Neurons. Brain. 128, 1847-1854.
46. Rush, A. M., Dib-Hajj, S. D., Liu, S., Cummins, T. R., Black, J. A., and Waxman, S. G. (2006) A Single Sodium Channel Mutation Produces Hyper- Or Hypoexcitability in Different Types of Neurons. Proc. Natl. Acad. Sci. U. S. A.. 103, 8245-8250.
47. Ptacek, L. J., George, A. L.,Jr., Griggs, R. C., Tawil, R., Kallen, R. G., Barchi, R. L., Robertson, M., and Leppert, M. F. (1991) Identification of a Mutation in the Gene Causing Hyperkalemic Periodic Paralysis. Cell. 67, 1021-1027.
48. Venance, S. L., Cannon, S. C., Fialho, D., Fontaine, B., Hanna, M. G., Ptacek, L. J., Tristani-Firouzi, M., Tawil, R., and Griggs, R. C. (2006) The Primary Periodic Paralyses: Diagnosis, Pathogenesis and Treatment. Brain. 129, 8-17.
49. Bendahhou, S., Cummins, T. R., Tawil, R., Waxman, S. G., and Ptacek, L. J. (1999) Activation and Inactivation of the Voltage-Gated Sodium Channel: Role of Segment S5 Revealed by a Novel Hyperkalaemic Periodic Paralysis Mutation. J. Neurosci.. 19, 4762-4771.
50. Cummins, T. R., Dib-Hajj, S. D., and Waxman, S. G. (2004) Electrophysiological Properties of Mutant Nav1.7 Sodium Channels in a Painful Inherited Neuropathy. J. Neurosci.. 24, 8232-8236.
51. Harty, T. P., Dib-Hajj, S. D., Tyrrell, L., Blackman, R., Hisama, F. M., Rose, J. B., and Waxman, S. G. (2006) Na(V)1.7 Mutant A863P in Erythromelalgia: Effects of Altered Activation and Steady-State Inactivation on Excitability of Nociceptive Dorsal Root Ganglion Neurons. J. Neurosci.. 26, 12566-12575.
52. Lampert, A., Dib-Hajj, S. D., Tyrrell, L., and Waxman, S. G. (2006) Size Matters: Erythromelalgia Mutation S241T in Nav1.7 Alters Channel Gating. J. Biol. Chem.. 281, 36029-36035.
53. Cavanaugh, D. J., Lee, H., Lo, L., Shields, S. D., Zylka, M. J., Basbaum, A. I., and Anderson, D. J. (2009) Distinct Subsets of Unmyelinated Primary Sensory Fibers Mediate Behavioral Responses to Noxious Thermal and Mechanical Stimuli. Proc. Natl. Acad. Sci. U. S. A.. 106, 9075-9080.
54. Brown, J., and Handley, S. L. (1980) The Development of Catalepsy in Drug-Free Mice on Repeated Testing. Neuropharmacology. 19, 675-678.
55. Ornstein, K., and Amir, S. (1981) Pinch-Induced Catalepsy in Mice. J. Comp. Physiol. Psychol.. 95, 827-835.
56. Klemm, W. R. (1965) Drug Potentiation of Hypnotic Restraint of Rabbits, as Indicated by Behavior and Brain Electrical Activity. Lab. Anim. Care. 15, 163-167.
57. Barrat, E. S. (1965) EEG Correlates of Tonic Immobility in the Opossum (Didelphis Virginiana). Electroencephalography and clinical neurophysiology. 18, 709-711.
58. Klemm, W. R. (1966) Electroencephalographic-Behavioral Dissociations during Animal Hypnosis. Electroencephalogr. Clin. Neurophysiol.. 21, 365-372.
59. Kulikov, A. V., Bazovkina, D. V., Kondaurova, E. M., and Popova, N. K. (2008) Genetic Structure of Hereditary Catalepsy in Mice. Genes Brain Behav.. 7, 506-512.
60. Klemm, W. R. (1976) Identity of Sensory and Motor Systems that are Critical to the Immobility Reflex ("Animal Hypnosis"). J. Neurosci. Res.. 2, 57-69.
61. Menescal-de-Oliveira, L., and Hoffmann, A. (1993) The Parabrachial Region as a Possible Region Modulating Simultaneously Pain and Tonic Immobility. Behav. Brain Res.. 56, 127-132.
62. Morgan, M. M., Whitney, P. K., and Gold, M. S. (1998) Immobility and Flight Associated with Antinociception Produced by Activation of the Ventral and lateral/dorsal Regions of the Rat Periaqueductal Gray. Brain Res.. 804, 159-166.
63. Monassi, C. R., Leite-Panissi, C. R., and Menescal-de-Oliveira, L. (1999) Ventrolateral Periaqueductal Gray Matter and the Control of Tonic Immobility. Brain Res. Bull.. 50, 201-208.
64. Fleischmann, A., and Urca, G. (1988) Clip-Induced Analgesia and Immobility in the Mouse: Pharmacological Characterization. Neuropharmacology. 27, 641-648.
|Science Writers||Eva Marie Y. Moresco|
|Illustrators||Diantha La Vine|
|Authors||Amanda L. Blasius, Adrienne E. Dubin, Matt J. Petrus, Byung-Kwan Lim, Anna Narezkina, Jose R. Criado, Derek N. Wills, Yu Xia, Cindy L. Ehlers, Kirk U. Knowlton, Ardem Patapoutian, Bruce Beutler|