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Voltage-gated Sodium Channels Confer Excitability to Human Odontoblasts

2006; Elsevier BV; Volume: 281; Issue: 39 Linguagem: Inglês

10.1074/jbc.m601020200

1083-351X

Bruno Allard, H. Magloire, Marie Lise Couble, Jean Christophe Maurin, Françoise Bleicher,

Neuroscience and Neuropharmacology Research

Odontoblasts are responsible for the dentin formation. They are suspected to play a role in tooth pain transmission as sensor cells because of their close relationship with nerve, but this role has never been evidenced. We demonstrate here that human odontoblasts in vitro produce voltage-gated tetrodotoxin-sensitive Na+ currents in response to depolarization under voltage clamp conditions and are able to generate action potentials. Odontoblasts express neuronal isoforms of α2 and β2 subunits of sodium channels. Co-cultures of odontoblasts with trigeminal neurons indicate a clustering of α2 and β2 sodium channel subunits and, at the sites of cell-cell contact, a co-localization of odontoblasts β2 subunits with peripherin. In vivo, sodium channels are expressed in odontoblasts. AnkyrinG and β2 co-localize, suggesting a link for signal transduction between axons and odontoblasts. Evidence for excitable properties of odontoblasts and clustering of key molecules at the site of odontoblast-nerve contact strongly suggest that odontoblasts may operate as sensor cells that initiate tooth pain transmission. Odontoblasts are responsible for the dentin formation. They are suspected to play a role in tooth pain transmission as sensor cells because of their close relationship with nerve, but this role has never been evidenced. We demonstrate here that human odontoblasts in vitro produce voltage-gated tetrodotoxin-sensitive Na+ currents in response to depolarization under voltage clamp conditions and are able to generate action potentials. Odontoblasts express neuronal isoforms of α2 and β2 subunits of sodium channels. Co-cultures of odontoblasts with trigeminal neurons indicate a clustering of α2 and β2 sodium channel subunits and, at the sites of cell-cell contact, a co-localization of odontoblasts β2 subunits with peripherin. In vivo, sodium channels are expressed in odontoblasts. AnkyrinG and β2 co-localize, suggesting a link for signal transduction between axons and odontoblasts. Evidence for excitable properties of odontoblasts and clustering of key molecules at the site of odontoblast-nerve contact strongly suggest that odontoblasts may operate as sensor cells that initiate tooth pain transmission. The mechanisms underlying dentin sensitivity still remain unclear because of the structural complexity of this tissue including odontoblasts, nerve endings, and the liquid content of surrounding dentinal tubules. Odontoblasts constitute a layer of cells responsible for dentin formation. Each cell has an extension running into the dentinal tubule and bathed in the dentinal fluid. Sensory unmyelinated nerve fibers belonging to the trigeminal ganglion enter the inner dentin and coil around the monopolar processes of odontoblasts (1Byers M.R. Int. Rev. Neurobiol. 1984; 25: 39-94Crossref PubMed Scopus (241) Google Scholar, 2Ibuki T. Kido M.A. Kiyoshima T. Terada Y. Tanaka T. J. Dent. Res. 1996; 75: 1963-1970Crossref PubMed Scopus (36) Google Scholar). A hydrodynamic concept, based on the spatial situation of odontoblasts, nerve endings, and fluid movements in dentinal tubules, postulated that nociceptive responses may result from an increase in intradentinal pressure, which in turn might activate nerve endings. However, nerve terminals do not reach the most sensitive zone of the dentin (dentino-enamel junction), and intradentinal axons could not be directly excited by stimuli producing pain when applied to the teeth (1Byers M.R. Int. Rev. Neurobiol. 1984; 25: 39-94Crossref PubMed Scopus (241) Google Scholar, 3Hildebrand C. Fried K. Tuisku F. Johansson C.S. Progr. Neurobiol. 1995; 45: 165-222Crossref PubMed Scopus (143) Google Scholar). Thus emerged the hypothesis that odontoblasts may initiate tooth pain sensation. Several lines of evidence support this assumption. Recently, we have shown that reelin, a large extracellular matrix glycoprotein elaborated by odontoblasts, could promote adhesion between nerves and cells (4Maurin J.C. Couble M.C. Didier-Bazes M. Brisson C. Magloire H. Bleicher F. Matrix Biol. 2004; 23: 277-285Crossref PubMed Scopus (43) Google Scholar). This close association suggested that odontoblasts and nerve endings may directly interact, although no synaptic structures or any junction could be detected between them (1Byers M.R. Int. Rev. Neurobiol. 1984; 25: 39-94Crossref PubMed Scopus (241) Google Scholar, 2Ibuki T. Kido M.A. Kiyoshima T. Terada Y. Tanaka T. J. Dent. Res. 1996; 75: 1963-1970Crossref PubMed Scopus (36) Google Scholar, 3Hildebrand C. Fried K. Tuisku F. Johansson C.S. Progr. Neurobiol. 1995; 45: 165-222Crossref PubMed Scopus (143) Google Scholar). Along this line, two kinds of mechanosensitive K+ channels (KCa and TREK-1) have been identified in human odontoblasts (5Allard B. Couble M.L. Magloire H. Bleicher F. J. Biol. Chem. 2000; 275: 25556-25561Abstract Full Text Full Text PDF PubMed Scopus (72) Google Scholar, 6Magloire H. Lesage F. Couble M.L. Lazdunski M. Bleicher F. J. Dent. Res. 2003; 82: 542-545Crossref PubMed Scopus (59) Google Scholar). This finding indicated that odontoblasts might be able to convert pain-evoking fluid displacement within dentinal tubules into electrical signals, strengthening their possible role as tooth sensor cells. The view that odontoblasts could detect and transduce painful stimuli into electric signals questioned the possibility that these cells display excitable properties and possess voltage-gated sodium channels. These later have indeed been detected in non-excitable mineralizing cells (7Black J.A. Waxman S.G. Dev. Neurosci. 1996; 18: 139-152Crossref PubMed Scopus (45) Google Scholar) like osteoblasts where sodium channel Nav1.2 mRNA and protein were identified (8Black J.A. Westenbroek R. Catterall W.A. Waxman S.G. Mol. Brain Res. 1995; 34: 89-98Crossref PubMed Scopus (20) Google Scholar). In teeth, voltage-gated Na+ channels have been previously evidenced in vitro on dental pulp cell by electrophysiological investigation (9Davidson R.M. Arch. Oral Biol. 1994; 39: 613-620Crossref PubMed Scopus (40) Google Scholar). However, the identity of the cultured cells under study and the expression of odontoblast key genes were not established, thus casting doubt about the cell type displaying voltage-gated sodium channel activity. To overcome these difficulties, we recently set up a unique cell culture system allowing the differentiation of human dental pulp cells into odontoblasts at the morphological, molecular, and functional levels (5Allard B. Couble M.L. Magloire H. Bleicher F. J. Biol. Chem. 2000; 275: 25556-25561Abstract Full Text Full Text PDF PubMed Scopus (72) Google Scholar, 10Couble M.L. Farges J.C. Bleicher F. Perrat-Mabillon B. Boudeulle M. Magloire H. Calcif. Tissue Int. 2000; 66: 129-138Crossref PubMed Scopus (218) Google Scholar, 11Buchaille R. Couble M.L. Magloire H. Bleicher F. Matrix Biol. 2000; 19: 421-430Crossref PubMed Scopus (61) Google Scholar). In the present study, we took advantage of this cell model to apply the patch clamp technique and determine whether a voltage-gated Na+ channel is functional in the odontoblast plasma membrane. In parallel, we investigated the molecular isoforms of sodium channel subunits and their spatial distribution in relation with key molecular components at sites of close contact between odontoblasts and nerves in odontoblasts co-cultivated with trigeminal ganglions and in human dental pulp in vivo. Cell Culture—Dental pulps cells were obtained from sound human third molar germs that were extracted for orthodontics reasons. Informed consent was obtained from the patients in accordance with French legal requirements (article 672-1, public health code). Explants were grown in Eagle's basal medium (Invitrogen) supplemented with ascorbic acid, antibiotics, fetal calf serum, and 10 mm sodium β-glycerophosphate as described previously (10Couble M.L. Farges J.C. Bleicher F. Perrat-Mabillon B. Boudeulle M. Magloire H. Calcif. Tissue Int. 2000; 66: 129-138Crossref PubMed Scopus (218) Google Scholar). After 2-3 weeks of culture, the cells differentiated into odontoblasts exhibiting typical features at the morphological (eccentric position of the nucleus, cellular extension, junctional complexes, intracellular organelles) and functional (type I collagen, dentin sialophosphoprotein, enamelysin, osteoadherin) level. Co-culture Assays—Trigeminal ganglion explants from 1-day-old Sprague-Dawley rat pups were co-cultured with human odontoblasts as recently described (4Maurin J.C. Couble M.C. Didier-Bazes M. Brisson C. Magloire H. Bleicher F. Matrix Biol. 2004; 23: 277-285Crossref PubMed Scopus (43) Google Scholar) except that the cultures were performed without embedding in collagen gel. After 3 days, they were routinely prepared for double immunodetection of α2/β2 subunits and peripherin/β2 and analyzed with a scanning laser confocal microscope Zeiss LSM 510 (Carl Zeiss, Le Pecq, France) using ×40/1.3 oil immersion objective. Figures were processed using Adobe PhotoShop 6.0 (Adobe Systems, San Jose, CA). RNA Extraction and RT-PCR—Total RNAs were extracted from the cultured cells using the Qiagen RNeasy kit and protocol (Qiagen, Chatsworth, CA). Purified RNA (3 μg) was reverse-transcribed using random hexamers as primers and converted into cDNA by means of the StrataScript™ RT 3The abbreviations used are: RT, reverse transcription; TTX, tetrodotoxin. kit (Stratagene, La Jolla, CA). PCR amplification was then realized from a 10th of the RT mixture in 50 μl containing 10 mm Tris-HCl, pH 8.3, 50 mm KCl, 1.5 mm MgCl2, 200 μm dNTPs, 2 units of TaqDNA polymerase, and 30 pmol of each sodium channel (SCN) degenerated primers. These primers were designed to hybridize to human SCN1A, SCN2A, and SCN3A genes. The forward primer was 5′-GTTGTGAATGCHCTTDTWGGAG-3′, and the reverse primer was 5′-CTTGAAGCAGAGANAGATANCC-3′. An amplification was also realized with SCN2B primers (forward primer, 5′-CAAATCACCCTCTCCCGTAGCC-3′; reverse primer, 5′-CGTTTCTCAGCATCACCGACAC-3′ corresponding to bp positions 123-144 and 500-521, respectively, of the human sequence (GenBank™ AF049498). The amplification was carried out for 35 cycles (1 min at 94 °C, 1 min at 50 °C (SCN1A, -2A, -3A) or 60°C (SCN2B), and 1 min at 72 °C followed by 10 min at 72 °C). Finally, PCR amplification was also realized with primers designed to hybridize to human cardiac SCN5A gene (forward primer, 5′-CATCGGAGAGCCCCTGGAGGAC-3′; reverse primer, 5′-GACTCGGAAGGTGCGTAAGGCTGA-3′. corresponding to bp positions 419-441 and 840-864, respectively, of the human sequence NM198056). The amplification was carried out for 30 cycles at 60 °C). Restriction Enzyme Analysis—Four independent PCR amplifications were performed and then desalted and concentrated 5-fold by filtration through a microconcentrator (Amicon Inc., Beverly, MA). An aliquot of 8 μl was incubated in a 10-μl final volume for 2 h at adequate temperature with enzyme as described by manufacturer's instructions. For SCN2B restriction analysis, a single PCR reaction was 5-fold concentrated, and an aliquot of 5 μl was digested in a 10-μl final volume. The digests (5 μl) along with an untreated sample and DNA marker were size-fractionated by electrophoresis in a non-denaturating 6% polyacrylamide gel (mini-gel apparatus, Bio-Rad) using a constant 40 V field. Gel was stained for 30 min in Vistra Green and imaged on a FluorImager (Amersham Biosciences, Orsay, France). In Situ Hybridization—The material consisted of culture samples and sound non-erupted human third molars prepared as described previously in Refs. 10Couble M.L. Farges J.C. Bleicher F. Perrat-Mabillon B. Boudeulle M. Magloire H. Calcif. Tissue Int. 2000; 66: 129-138Crossref PubMed Scopus (218) Google Scholar and 12Bleicher F. Couble M.L. Farges J.C. Couble P. Magloire H. Matrix Biol. 1999; 18: 133-143Crossref PubMed Scopus (103) Google Scholar. For detection of the SCN2A and SCN2B transcripts, in situ hybridization was performed using an antisense single-stranded DNA probe (12Bleicher F. Couble M.L. Farges J.C. Couble P. Magloire H. Matrix Biol. 1999; 18: 133-143Crossref PubMed Scopus (103) Google Scholar) with a specific activity of about 2.5 × 106 cpm/pmol. Sense primers were used for the synthesis of the control probes. The images were processed using Adobe PhotoShop 6.0 (Adobe Systems). Finally, pulp tissue from tooth germs was routinely processed (Masson's trichrome staining) for light microscopic observation. Immunochemistry—Cryostat sections of pulps were reacted for double staining with anti-α2/anti-β2 subunits (mouse monoclonal antibodies at 10 μg/ml, Upstate Biotechnology, Lake Placid, NY; rabbit polyclonal antibodies at 10 μg/ml; Alomone Labs, Jerusalem, Israel); anti-β2 subunits/anti-peripherin (mouse monoclonal Mab 1527, chemicon, Temecula, CA); anti-β2 subunits/anti-ankyrinG (mouse monoclonal antibodies at 10 μg/ml, Zymed Laboratories Inc., South San Franscisco, CA), and anti-ankyrinG/anti-β-tubulin (H-235, Santa Cruz Biotechnology, Santa Cruz, CA). Subsequently, the slices were rinsed and then incubated (45 min at room temperature) with Alexa Fluor 594 goat anti-mouse IgG (Molecular Probes, Eugene, OR) for α2 subunits, ankyrinG, and peripherin and with Alexa Fluor 488 goat anti-rabbit IgG (Molecular Probes) for β2 subunits and β-tubulin. They were then washed, mounted in phosphate-buffered saline-glycerol, and observed under scanning laser confocal microscopy using ×40/1.3 or ×63/1.4 oil immersion objective. Peripherin, α2 subunits, and ankyrinG were assigned a red color; β2 subunits and β-tubulin a green color with the laser scanning software. Co-localization consequently resulted in a yellow color. Negative controls were carried out by omitting the primary antibodies or by incubating with normal mouse or rabbit IgG. Figures were processed using Adobe PhotoShop 6.0 (Adobe Systems). Electrophysiology—Membrane currents and potentials were recorded in the whole cell configuration on cultured odontoblasts using a patch clamp amplifier (model RK 400; Bio-Logic, Claix, France). Data acquisition and generation of command voltage pulses were done using the pClamp9 software (Axon Instruments Inc.) driving an A/D, D/A converter (Digidata 1322A, Axon Instruments Inc.). Cell capacitance, used to calculate the density of currents (A/F), was determined by integration of a control current trace obtained with a 10-mV depolarizing pulse from -90 mV. Leak currents were subtracted from all recordings using a 10-mV depolarizing pulse from the holding potential supposing a linear evolution of leak current with depolarization. Individual curves of the voltage dependence of the Na+ current density were fitted with Equation 1. I(V)=Gmax(V-Vrev)/{1+exp[(V0.5-V)/k]}(Eq. 1) where I(V) is the density of the current measured, V is the test pulse, Gmax is the maximum conductance, Vrev is the apparent reversal potential, V0.5 is the half-activation voltage, and k is a steepness factor. Individual curves of the voltage dependence of the steady-state inactivation of the Na+ current were fitted with the Equation 2. I/Imax=1/{1+exp[(V-V0.5)/k]}(Eq. 2) where Imax is the maximal current, V is the conditioning pulse, V0.5 is the half-maximal inactivation voltage, and k is a steepness factor. All experiments were carried out at room temperature (20-24 °C). Solutions and Chemicals—Pipettes were filled with (in mm): 120 potassium aspartate, 5 KCl, 5 MgCl2, 10 glucose, 3 K2ATP, 5 Na2-CP, 0.4 Na3-GTP, 5 EGTA, 10 Hepes, pH 7.2. The bath solution corresponded to a Tyrode solution containing (in mm): 140 NaCl or 140 choline chloride, 5 KCl, 2.5 CaCl2, 2 MgCl2,10 Hepes, pH 7.2. Tetrodotoxin (TTX) (Sigma) was diluted to the required concentration in the bath solution. Voltages were corrected for liquid junction potentials calculated to be 10 mV with the solutions used. Dye Microinjection in Odontoblasts in Co-culture—For intracellular staining of odontoblasts co-cultivated with trigeminal ganglions, micropipettes filled with an internal solution containing Lucifer yellow CH (100 μm, Sigma) were sealed on odontoblasts, and the patch membrane was ruptured to allow the dye to diffuse into the cell. Cells were imaged using a ×20 objective on an inverted microscope (Olympus IMT2) equipped for epifluorescence. Images were captured every 2 min after dye injection with a Coolsnapfx charge-coupled device camera (Roper Scientific, Evry, France). Injected cells were chosen as a function of their apparent close vicinity with the thin nerve fibers from trigeminal ganglions. Statistics—Non-linear least-squares fits were performed using a Marquadt-Levenberg algorithm routine included in MicroCal Origin. Data values are presented as means ± S.E. Characterization of Voltage-gated Sodium Channels and Voltage Responses in Cultured Odontoblasts—Cultured odontoblasts were depolarized by steps of 50-ms duration from a holding potential of -90 mV. All the odontoblasts tested (n = 13) displayed a voltage-gated inward current that rapidly inactivated (Fig. 1A). The average time to peak of this inward current was 2.9 ± 0.4 ms at 0 mV. Fig. 1B presents the mean current-voltage relationships established for the peak current. The threshold of activation was around -40 mV, and currents peaked at 0 mV and reversed at + 55 ± 3.6 mV. For each cell, the current-voltage relationship was fitted using Equation 1 (see "Experimental Procedures"). Mean values for Gmax, Vrev, V0.5, and k were 336 ± 52 S/F, +55 ± 3.6 mV, -13 ± 1.9 mV, and 4.1 ± 0.4 mV, respectively. The voltage dependence of the inactivation process was then investigated using a steady-state inactivation protocol. A 50-ms test pulse was delivered to 0 mV, a membrane potential at which the current was maximal, and was preceded by a 50-ms depolarizing prepulse of increasing amplitude. Fig. 1C shows that for predepolarizations up to -40 mV, the current that was activated during the test pulse remained unaltered. For higher depolarizations, the inward current during the test depolarization progressively decreased and then completely vanished for a predepolarization to 0 mV. For each cell, the inactivation curve was fitted using Equation 2 (see "Experimental Procedures"). The corresponding mean inactivation curve indicated mean values for V0.5 and k of -26 ± 1.5 and 8.6 ± 0.6 mV, respectively. Voltage dependence, kinetic properties, and reversal potential of the inward current strongly suggested that this current corresponds to a voltagegated Na+ current. Indeed, in all odontoblasts tested, we found that TTX completely and reversibly abolished the inward current elicited by a depolarizing pulse to 0 mV (Fig. 2A). Adding increasing concentrations of TTX from 10 to 1000 nm in a cumulative manner indicated a half-maximal inhibition of the current with 45 nm. Additionally, in two cells, the substitution of choline for Na+ led to an almost complete and a reversible abolition of the inward current (Fig. 2C). Taken together, these data demonstrate that odontoblasts express a functional voltage-gated TTX-sensitive Na+ channel.FIGURE 2Effect of TTX and removal of Na+ on inward currents and voltage responses in odontoblasts. In A-C, currents were obtained in response to a voltage pulse to 0 mV from a holding potential of -90 mV. In B, left panel, increasing concentrations of TTX were added in the external. Each trace corresponds to five superimposed current traces obtained at a given TTX concentration indicated next to each current trace. The right panel shows the corresponding relationship between the relative current amplitude and the TTX concentration fitted by a Hill equation (relative current = 1/(1+(x/k)n) with k = 45 nm and n = 1.1). In D, under current clamp conditions, the internal potential was held around -80 mV by passing a constant negative current. In the left panel, voltage responses were obtained in response to injection of depolarizing currents of 0.5-ms duration in 1-pA increments from a starting value of +15 pA. The right panel shows two consecutive spikes evoked by injection of two current pulses of 0.5-ms duration given to +20 pA and separated by a 60-ms interval. In E, spikes were evoked by injection of current pulses of 0.5-ms duration given to +20 pA (left panel) and +12 pA (right panel). The stars indicate the voltage responses evoked after the addition of 2 μm TTX (left panel) and after substitution of 140 mm choline for 140 mm Na+ (right panel) in the external solution. The middle panel illustrates the voltage responses of the left panel on an expanded scale.View Large Image Figure ViewerDownload Hi-res image Download (PPT) Given the high density of the voltage-gated Na+ inward current together with the low density of outward current that developed in response to depolarization, we speculated that odontoblasts might be able to produce regenerative voltage responses. We then investigated the electrical excitability of odontoblasts by performing current clamp experiments. Depolarizing currents of increasing amplitude and 0.5-ms duration were injected into the cells from a membrane potential held around -80 mV by applying constant negative current. In all three cells tested with this protocol, infraliminar stimulations induced electrotonic response, whereas a spike bringing the membrane potential around +45 mV developed in response to current injection higher than 18 pA (Fig. 2D, left panel). Fig. 2C, right panel, shows that train of action potentials could even be elicited in response to supraliminar repetitive stimulation of the cells at a frequency up to 18 Hz without any decrease in spike amplitude. Finally, as expected, spikes were totally inhibited by the addition of TTX in the bath or substitution of choline for Na+ in the external solution, confirming that the spike resulted from the activation of the voltage-gated TTX-sensitive Na+ current (Fig. 2E). Brain Sodium Channel Subunits in Cultured Odontoblasts— The presence of functional voltage-gated Na+ channel in cultured odontoblasts prompted us to look for what kind of sodium channel subunits transcripts are expressed by odontoblasts. Degenerate homology-PCR was used to co-amplify SCN1A, SCN2A, and SCN3A genes. For this purpose, these sequences (SCN1A: S71446, SCN2A: M94055, SCN3A: AF035685, in GenBank™) were aligned using the MultAlin program (13Corpret F. Nucleic Acids Res. 1988; 16: 10881-10890Crossref PubMed Scopus (4347) Google Scholar). Two degenerate primers were designed to amplify a 277-bp fragment for SCN1A and SCN2A and a 268-bp fragment for SCN3A. RT-PCR realized on cultured odontoblast RNA amplified a single PCR product of about 277 bp. The gel did not allow us to discriminate between the 277 and 268 bp fragments. This product was submitted to four sets of digestion by restriction enzymes having specificity for each subtype. Fig. 3 shows that SCN1A, SCN2A, and SCN3A were expressed. For SCN2A and SCN3A, restriction produced two fragments of the expected size (Table 1). Digestion of the PCR product by TaqI gave rise to a fragment of 155 bp. The two other expected fragments (64 and 58 bp) were not detectable. A band of 399 bp was amplified from these RNA using the SCN2B primers. Restriction of the product gave rise to two fragments of 255 and 144 bp. In contrast, SCN5A coding for Nav1.5 (found in cardiac tissue) was not expressed in odontoblasts (data not shown). All these data confirm that the PCR products accurately represent the co-expression of the β2 subunit and the three isoforms SCN1A, SCN2A, and SCN3A (corresponding to Nav1.1, Nav1.2, and Nav1.3 α subunits, respectively, in another nomenclature) found in the central nervous system.TABLE 1Expected restriction endonuclease fragment sizes The 277-bp product expected for Na+ channels Nav1.1, 1.2, 1.3, or 1.7, was analyzed by cleavage with TaqI ((T/C)GA), AsnI (A(T/T)AAT), BspLU11 ((A/C)ATGT). The 399 bp product for β2 subunit was analyzed by cleavage with MaeIII (/GTNAC). The sizes of the expected fragments for each subunit (–) indicate that the restriction enzyme would not be expected to cut the product from the indicated subunit.Sodium channel subunitsSizeTaqIAsnIBspLU11MaeIIIbpSCN1A155–––64–58SCN2A–152–125––SCN3A––143–125–SCN2B–––255–144 Open table in a new tab In Situ Hybridization of SCN2A and SCN2B Transcripts— SCN2A and SCN2B transcripts were detected in cultured odontoblasts (Fig. 4, a and b). Experiments conducted in vivo on human dental pulp tissue clearly demonstrated that the highest density of transcripts was detected in odontoblasts as opposed to pulp cells (Fig. 4, c and d). Hybridization with sense SCN2A (data not shown) and SCN2B probes showed negligible signal in odontoblasts (Fig. 4f). On Fig. 4e, the location and spatial organization of odontoblast layer is clearly evidenced at the periphery of the pulp tissue. Co-culture Assays—Odontoblasts are known to be closely associated with nerves. To mimic the in vivo situation and to explore how Na+ channel subunits localize when nerves make contacts with odontoblasts, odontoblasts were co-cultivated with rat trigeminal ganglions. Analysis by confocal microscopy clearly showed a co-localization (yellow patches) of α2 and β2 subunits in the odontoblast cell membrane, whereas α2 subunits were often densely expressed at the apical pole of the cells (Fig. 5, a-c). When a single neurite ran close to the odontoblast cell membrane, α2 and β2 subunits clustered in the contact area (Fig. 5, d-f). Staining with antibodies raised against peripherin, a component of trigeminal axons (14Brody B.A. Ley C.A. Parysek L.M. J. Neurosci. 1989; 9: 2391-2401Crossref PubMed Google Scholar), clearly identified the nerves from the trigeminal ganglion, and the double labeling with β2 subunits showed a dot-like co-localization where a close contact was evidenced between odontoblasts and neurites (Fig. 5, g-i). To explore the possibility that electric signals may propagate from odontoblasts to nerve cells via gap junctions, we injected Lucifer yellow into odontoblasts, a reported freely diffusible dye tracer through gap junctions (15Ushiyama J. Cell Tissue Res. 1989; 258: 611-616Crossref PubMed Scopus (33) Google Scholar). Microinjection was preferentially performed in odontoblasts making apparent close contact with nerves. Fig. 5j shows an intense fluorescence in a microinjected cell that spread after 30 min to adjacent odontoblast (Fig. 5k). However, in the 10 cells tested, the dye failed to migrate to axons located in the close vicinity of the injected cell. Immunohistochemistry in Odontoblasts in Vivo—Double staining of α2 and β2 subunits in odontoblasts demonstrated a strong fluorescence for the two subunits at the apical pole of the cells (Fig. 6, a and b). In addition, α2 subunits labeling clearly underlined the membranes of the basal pole of the odontoblasts (Fig. 6b). Confocal analysis showed co-localizations of α2 and β2 subunits on the cell membrane and at the apical pole corresponding to the terminal web connecting odontoblasts in this region (Fig. 6c). In mature odontoblasts, β2 subunits decorated as dots profiled the cell membrane and labeled thin axons (Fig. 6d). Peripherin immunoreactivity revealed nerves running to the odontoblast layer (Fig. 6e). Confocal microscopy clearly showed co-localizations of peripherin positive nerves with β2 at the apical pole of the cells without co-localization of β2 and peripherin in the nerve fibers (Fig. 6f). β2 subunits were also shown to co-localize with ankyrinG (an intracellular anchoring protein directly linked to β2 subunit intracellular domains) (Fig. 6g) at the apical pole of the odontoblast layer and along the cell bodies only as cell processes did not show any ankyrin immunoreactivity (Fig. 6, h and i). Finally, β-tubulin, a major brain component of microtubules suspected to bind ankyrinG (16Kobayashi N. Mundel P. Cell Tissue Res. 1998; 291: 163-174Crossref PubMed Scopus (87) Google Scholar), was mainly associated with the odontoblast cell membrane (Fig. 6j) and co-localized with ankyrinG particularly at the base of the cell processes (Fig. 6, k and l). On in vitro and in vivo control experiments, negligible staining could be detected (data not shown). Intracellular staining was observed in some experiments (Fig. 6g); it might correspond to β2 subunits in the progress of synthesis related to the secretory stage of odontoblasts. In this study, we present evidence that voltage-gated TTX-sensitive sodium channels are functional in cultured odontoblasts originating from human dental pulp. In response to depolarization, odontoblasts exhibited a fast sodium current that inactivated rapidly. This sodium current displayed biophysical characteristics comparable with those classically reported for the voltage-gated sodium current in axons (17Armstrong C.M. Bezanilla F. Rojas E. J. Gen. Physiol. 1973; 62: 375-391Crossref PubMed Scopus (365) Google Scholar, 18Oxford G.S. Wu C.H. Narahashi T. J. Gen. Physiol. 1978; 71: 227-247Crossref PubMed Scopus (98) Google Scholar). Although less sensitive to TTX than voltage-gated Na+ channels present in nervous cells, Na+ currents in odontoblasts were found to be as sensitive as cloned brain channels expressed in host systems (19Noda M. Suzuki H. Numa S. Stuhmer W.A. FEBS Lett. 1989; 259: 213-216Crossref PubMed Scopus (271) Google Scholar). In agreement with our electrophysiological data, PCR experiments and in situ hybridization performed in cultured odontoblasts demonstrated expression of the transcripts of four genes (SCN1A, SCN2A, SCN3A, and SCN2B) encoding, respectively, the pore-forming α subunit isoforms Nav1.1, Nav1.2, and Nav1.3 and β2 subunits of voltage-gated Na+ channels broadly expressed in neurons of the centra