A new sea anemone peptide, APETx2, inhibits ASIC3, a major acid‐sensitive channel in sensory neurons

Sylvie Diochot, Anne Baron, Lachlan D Rash, Emmanuel Deval, Pierre Escoubas, Sabine Scarzello, Miguel Salinas, Michel Lazdunski

Author Affiliations

  1. Sylvie Diochot1,
  2. Anne Baron1,
  3. Lachlan D Rash1,
  4. Emmanuel Deval1,
  5. Pierre Escoubas1,
  6. Sabine Scarzello1,
  7. Miguel Salinas1 and
  8. Michel Lazdunski*,1
  1. 1 Institut de Pharmacologie Moléculaire et Cellulaire, Centre National de la Recherche Scientifique, Institut Paul Hamel, Sophia Antipolis, Valbonne, France
  1. *Corresponding author. Institut de Pharmacologie Moléculaire et Cellulaire, Centre National de la Recherche Scientifique, UMR 6097, Institut Paul Hamel, 660, Route des Lucioles, Sophia Antipolis, 06560 Valbonne, France. Tel.: +33 493 957702 or 03; Fax: +33 493 957704; E-mail: ipmc{at}
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From a systematic screening of animal venoms, we isolated a new toxin (APETx2) from the sea anemone Anthopleura elegantissima, which inhibits ASIC3 homomeric channels and ASIC3‐containing heteromeric channels both in heterologous expression systems and in primary cultures of rat sensory neurons. APETx2 is a 42 amino‐acid peptide crosslinked by three disulfide bridges, with a structural organization similar to that of other sea anemone toxins that inhibit voltage‐sensitive Na+ and K+ channels. APETx2 reversibly inhibits rat ASIC3 (IC50=63 nM), without any effect on ASIC1a, ASIC1b, and ASIC2a. APETx2 directly inhibits the ASIC3 channel by acting at its external side, and it does not modify the channel unitary conductance. APETx2 also inhibits heteromeric ASIC2b+3 current (IC50=117 nM), while it has less affinity for ASIC1b+3 (IC50=0.9 μM), ASIC1a+3 (IC50=2 μM), and no effect on the ASIC2a+3 current. The ASIC3‐like current in primary cultured sensory neurons is partly and reversibly inhibited by APETx2 with an IC50 of 216 nM, probably due to the mixed inhibitions of various co‐expressed ASIC3‐containing channels.


Acid‐sensing ion channels (ASICs) are H+‐gated Na+‐permeable channels formed by the homo‐ or heteromeric association of six different subunits (Waldmann and Lazdunski, 1998): ASIC1a (Waldmann et al, 1997b), ASIC1b (Chen et al, 1998), ASIC2a (Price et al, 1996; Waldmann et al, 1996), ASIC2b (Lingueglia et al, 1997), ASIC3 (Waldmann et al, 1997a; de Weille et al, 1998; Babinski et al, 1999), and ASIC4 (Akopian et al, 2000; Grunder et al, 2000). Only ASIC1a, ASIC1b, ASIC2a, and ASIC3 are functionally activated by extracellular H+ when expressed alone. ASIC2b can modulate heteromeric ASIC currents by inducing a sustained nonselective cation current following the transient peak (Lingueglia et al, 1997; Coscoy et al, 1999).

In sensory neurons, ASIC currents have been implicated in pain transduction associated with acidosis in inflamed or ischemic tissues (Reeh and Steen, 1996; Waldmann and Lazdunski, 1998; Benson et al, 1999; Kress and Zeilhofer, 1999; Pan et al, 1999; Sutherland et al, 2001; Voilley et al, 2001; Mamet et al, 2002; Ugawa et al, 2002; Krishtal, 2003), particularly ASIC3, which is mainly expressed in sensory neurons (Waldmann et al, 1997a; Voilley et al, 2001). Recent studies in knockout mice confirm that ASIC3 plays a major role in high‐intensity pain stimuli (Price et al, 2001; Chen et al, 2002) and in acid‐induced hyperalgesia (Sluka et al, 2003). An involvement in the mechanosensitivity of large sensory neurons has also been proposed (Xie et al, 2002).

Further analysis of the involvement of ASIC3 in the electrical activity of nociceptors requires selective pharmacological tools. To date, the repertoire of active ligands on the ASIC3 channel is limited to amiloride, nonsteroidal anti‐inflammatory drugs, and Gd3+ (Waldmann et al, 1997a; Babinski et al, 2000; Voilley et al, 2001) that act as inhibitors, and to the mammalian neuropeptides NPFF and NPSF that activate ASIC3 (Askwith et al, 2000; Deval et al, 2003). However, none of these drugs is absolutely specific for ASIC channels.

In the past 25 years, animal venoms have yielded a great number of toxins that modulate specifically and with high affinity voltage‐gated Na+, K+, and Ca2+ currents (Moczydlowski et al, 1988; Norton, 1991; Harvey et al, 1994; Uchitel, 1997; Tytgat et al, 1999; Escoubas et al, 2000b), Ca2+‐gated K+ channels (Hugues et al, 1982; Shakkottai et al, 2001), and mechano‐sensitive K+ channels (Bode et al, 2001). Recently, Conus toxins have been shown to target neurotransmitter receptors at sensory synapses (England et al, 1998). The only toxin known to affect ASIC channels is Psalmotoxin 1 (PcTx1), a tarantula venom peptide that acts as a potent and specific inhibitor of homomeric ASIC1a channels (Escoubas et al, 2000a; Escoubas et al, 2003). We report here the identification of APETx2, a novel peptide toxin isolated from sea anemone venom, which selectively inhibits homomeric ASIC3 channels as well as the ASIC1a+3, ASIC1b+3, and ASIC2b+3 heteromers. A physico‐chemical characterization of APETx2 is presented, including its disulfide bridge arrangement, and a structural model based on its homology with the K+ channel sea anemone toxin BDS‐I. We show that APETx2 inhibits ASIC3‐like currents recorded from rat sensory neurons. APETx2 thus constitutes the first pharmacological tool to analyze the physiological involvement of ASIC3‐containing channels in neuronal excitability and pain coding.


Purification of an ASIC3 inhibitory peptide from Anthopleura elegantissima

In order to find effectors of the ASIC3 channel, a large number of scorpion, bee, spider, snake, and sea anemone venoms (1/1000 dilution) or peptide fractions (0.1 mg/ml) were screened on ASIC3 channels expressed in Xenopus oocytes. A peptide fraction from the sea anemone Anthopleura elegantissima (Bruhn et al, 2001) was found to inhibit more than 80% of the rat ASIC3 current stimulated at pH6. The active peptide was purified to homogeneity by bioassay‐guided reversed‐phase and cation‐exchange chromatography (Supplementary Figure A), and was named APETx2.

Biochemical properties

APETx2 is a basic peptide (pI=9.59) of 42 amino acids, crosslinked by three disulfide bridges and has a calculated 280 nm molecular absorbance of ε280=11170. Its full sequence was established by N‐terminal Edman degradation, and its measured monoisotopic mass (4557.96 Da) was in perfect accordance with the mass calculated from sequence data (4557.88 Da, accuracy 17.5 ppm), indicating a free C‐terminal carboxylic acid. APETx2 displays 64% sequence identity (76% homology) with APETx1 (Diochot et al, 2003) (Figure 1A) and only 34% sequence identity (57 and 55% homology, respectively) with the BDS‐I and BDS‐II toxins from Anemonia sulcata, which inhibit the voltage‐dependent K+ (Kv) channel Kv3.4 (Diochot et al, 1998). Sequence identity with Na+ channel activators such as AP‐A, AP‐B, AP‐C, APE1‐1, and APE‐2 from Anthopleura sp (Bruhn et al, 2001) is only 25–29% (homology 41–47%). APETx2 does not display any sequence homologies with the ASIC1a inhibitor PcTx1 previously isolated from a tarantula venom (Escoubas et al, 2000a).

Figure 1.

Structural properties of APETx2. (A) Sequence alignments of APETx2, with K+ channel modulators from sea anemones. Black boxes indicate sequence identities and gray boxes sequence homologies with BDS‐I and BDS‐II (Anemonia sulcata), and APETx1 (Anthopleura elegantissima). The three disulfide bonds of APETx2, determined by the partial reduction/cyanylation method, are indicated. (B) Expected cleavage fragments of APETx2 and their calculated masses (average mass, M+H+) for singly reduced bonds according to the predicted disulfide bond arrangement. The masses in parenthesis were those observed after cleavage and reduction of peak 2a and peak 3b.

The determination of disulfide bridges in small peptide toxins is crucial to understand and confirm the three‐dimensional structure of the toxins. Partial reduction and cyanylation of APETx2 yielded five components separated by HPLC (Supplementary Figure B). MALDI‐TOF MS indicated that peaks 2 and 3 predominantly contained singly reduced/cyanylated isoforms (+52 Da). Based on its sequence homology and conserved cysteine spacing with BDS‐I, APETx2 was predicted to have similar disulfide pairing. Figure 1B shows the predicted fragments and calculated masses for each disulfide bond of APETx2 and the masses observed from the cleavage of singly reduced isoforms in HPLC peaks 2 and 3. Following cleavage and full reduction, MALDI‐TOF MS analysis revealed that peak 2 contained only one singly reduced isoform with the major ions (m/z 2025.53 and 2097.53), corresponding unambiguously to fragments expected for a Cys20–Cys38 (CysIII–CysVI) bond. Analysis of cleavage fragments from peak 3 suggested the presence of two isoforms of singly reduced toxin. The major ions (m/z 2741.71 and 1475.11) corresponded to cleavages at Cys6 and Cys30 (CysII–CysIV), while peptide 3772.86 indicated the reduction and cleavage of a Cys4–Cys37 (CysI–CysV) bond. See online Supplementary data for more details.

APETx2 has the same disulfide arrangement (CysI–CysV, CysII–CysIV, CysIII–CysVI) as BDS‐I, the only toxin with high homology to APETx2 for which the disulfides have been deduced (NMR data) (Driscoll et al, 1989b). Alternative disulfide bond pairings observed in other sea anemone toxins (HmK: I–VI, II–IV, III–V), or inhibitor cystine knot (ICK) toxins (I–IV, II–V, III–VI) were not supported by experimental data.

Toxin structure

Examination of the three‐dimensional structures of BDS‐I, APETx1, and APETx2 reveals that they share very similar features, comprising a triple antiparallel β‐sheet motif stabilized by three disulfide bridges. Although the orientation of the N‐terminal and connecting loops varies between BDS‐I and the APETx toxins, the main differences appear in the surface features. Comparison of BDS‐I and APETx1 (Figure 2A, boxed panel) shows that the differences in the primary sequence and therefore amino‐acid side chains are primarily reflected on the face of the toxin formed by the N‐terminal loop and the last two strands of the β‐sheet. APETx1 shows a higher abundance of aromatic residues. Comparison of the differences between APETx1 and APETx2 (Figure 2A) shows that differences in sequence result mostly in surface variations on the opposite side of the toxin and to a lesser extent in the C‐terminal area. Of particular significance are the replacements in APETx2 of Tyr5, Lys8, and Ileu10 by Ser5, Asn8, and Lys10, respectively, and the replacement of Gly16, Thr17, and Pro18 by Tyr16, Arg17, and Lys18. The latter induce a tighter turn of the loop connecting the first and second strands of the β‐sheets due to Pro18, and comprise a surface that is at the same time bulkier (Tyr16) and bears more positive charges (Figure 2B). The replacement of Gly31 by Arg 31 also contributes to the constitution of a strong basic patch on this side of the toxin. The modifications on the opposite side of the toxin result in a more negatively charged patch, surrounded by an area of hydrophobic or neutral residues. Comparison with BDS‐I (Figure 2B) shows that this area is significantly different, and thus may play a role in channel selectivity. The main differences between APETx1 and APETx2 appear to be located on two opposite sides of the molecule, with the β‐turn composed of Tyr16, Arg17, and Lys18, which could be hypothesized as a significant selectivity site for recognition of ASIC3.

Figure 2.

Molecular modeling of APETx2. (A) Ribbon representations of BDS‐I, APETx1, and APETx2. Peptide backbones and selected side chains are superimposed on the ribbon structure. To compare the models of BDS‐I and APETx1 (box), only side chains of nonconserved amino acids are apparent. The model of APETx2 shows side chains differing between APETx1 and APETx2, and Arg24, which could be part of the active site of the toxin. (B) Surface representation of the same toxins, mapped with the calculated electrostatic potential distribution (Blue=positive, red=negative, white=neutral) showing the charge distribution on the calculated toxin surface. All structures were generated with DeepView v3.7 and raytraced in PovRay.

APETx2 inhibits homomeric ASIC3 current

Rat homomeric ASIC3 currents induced every minute by a rapid step to pH 6 from pH 7.4 were recorded from Xenopus oocytes (Figure 3A, ▴) or COS cells (Figure 3A, •). Toxin‐containing solutions at pH 7.4 were perfused before the acidic step. Inhibition of the ASIC3 current started at 10 nM APETx2 and was maximal at 3 μM (Figure 3A and B). The inhibition of ASIC3 currents was rapid and saturated within 30 s of APETx2 perfusion. The concentration–response relationship indicates an IC50 of 63 nM (Figure 3A). Effects were totally reversible within 4 min (Figure 3C). The sustained component of ASIC3 current, easily measurable at pH 4, was insensitive to 3 μM APETx2, even though the transient peak component was totally inhibited (Figure 3D).

Figure 3.

Effect of APETx2 on homomeric ASIC3 current. (A) Concentration–response curve for APETx2 effects on ASIC3 channels expressed in Xenopus oocytes (▴) and in COS cells (•). Holding potential: −50 mV, pH drop from 7.4 to 6. APETx2 was perfused for 30 s before the pH drop. Data were fitted by the Hill equation (nH=1) giving an IC50 value of 63 nM. Each point is the mean±s.e.m. (3–6 cells). (B) APETx2 (3 μM) totally inhibits the ASIC3 current. (C) Effect of 100 nM APETx2 on ASIC3 currents, and reversibility. (D) Upon stimulation of ASIC3 at pH4, APETx2 (3 μM) inhibits the peak, but not the plateau phase of the current.

Human ASIC3 expressed in COS cells was also inhibited by APETx2 with an IC50 of 175 nM and nH of 1 (not shown).

APETx2 (3 μM) perfused for 30 s before the pH drop did not significantly inhibit ASIC1a, ASIC1b, or ASIC2a homomeric currents activated at pH 6 or 5 (n=5–6 cells under each condition, P>0.05, not shown) and expressed in COS cells.

APETx2 directly inhibits homomeric ASIC3 channels in outside‐out patches

Unitary ASIC3 currents triggered by an external pH drop from 7.4 to 6.6 were recorded at −50 mV from outside‐out patches of transfected COS cells. A high number of channels were usually simultaneously recorded even when submaximally activated at pH 6.6 (Figure 4A). When APETx2 (3 μM) was applied to the bath solution 30 s before the pH drop, it induced a 75±6% (n=4) inhibition of ASIC3 peak current and this effect was rapidly reversible. Amplitude histograms obtained from the analysis of ASIC3 unitary current recorded before (Figure 4Ba) and after (Figure 4Bb) application of APETx2 show that the unitary amplitude of ASIC3 currents was not modified by the toxin. The mean amplitude values are shown in Figure 4C. These results show that the ASIC3 channel is directly inhibited by the toxin, without any change in its unitary conductance. Similar results were obtained with 100 nM APETx2 producing a partial inhibition of the peak outside‐out current (58±7%).

Figure 4.

Effect of APETx2 on unitary ASIC3 currents recorded from outside‐out patches. ASIC3 currents were recorded from COS transfected cells. Holding potential: −50 mV, pH drop from 7.4 to 6.6. (A) Inhibitory effect of APETx2 (3 μM) on an ASIC3 current recorded from a single excised patch. The current was triggered every minute, and APETx2 was externally applied 30 s before the second pH drop. The inhibition of ASIC3 current was 75±6% (n=4), and reversible. (B) Time‐scale magnifications of parts of current trace shown in (A) (see a and b), and amplitude histograms of unitary current recorded before (a) and after (b) the application of APETx2. (C) Statistical analysis of ASIC3 unitary current amplitude measured at −50 mV in the presence and in the absence of APETx2 (4 excised patches, n.s., nonsignificant).

Effects of APETx2 on the heteromeric ASIC1a+3 current

As ASIC1a and ASIC3 channels are co‐localized in sensory neurons (Voilley et al, 2001; Alvarez de la Rosa et al, 2002), we studied the effects of APETx2 on the heteromeric ASIC1a+3 channel expressed in COS cells using the pBudCE4.1 vector designed for simultaneous expression of two genes under the control of two independent promoters. The current induced at pH 5 exhibits ASIC3‐like kinetics and a plateau phase (Figure 5Aa). The inactivation time constant, 258±136 ms (n=8), was comparable to that of the ASIC3 current (440±135 ms, n=15). As shown previously (Escoubas et al, 2000a), this current was insensitive to 10 nM PcTx1, a concentration that completely blocks the homomeric ASIC1a current (Figure 5Ab). The ASIC1a+3 current induced at pH 6 was only partly inhibited (63±10%, n=6) by high concentrations of APETx2 (3 μM). Moreover, the ASIC1a+3 current appears to be less sensitive than homomeric ASIC3 current, with an IC50 of 2 μM (nH=0.9; Figure 5D, ○).

Figure 5.

Effect of APETx2 on heteromeric ASIC1a+3, ASIC1b+3, and ASIC2b+3 channels. ASIC subunits were co‐expressed in COS cells. Drugs were perfused for 30 s before the pH drop, as indicated above each current trace. (A) ASIC1a+3 current stimulated at pH 5 exhibits a peak and a plateau phase (a). At pH 6, the current is insensitive to PcTx1 (10 nM), whereas partly inhibited by APETx2 (3 μM) (b). (B) The peak ASIC2b+3 current is inhibited by 300 nM of APETx2 (a) (HP=−50 mV). At +50 mV, the peak ASIC2b+3 current was also inhibited by the toxin (b), whereas the outward sustained phase was insensitive to APETx2 (300 nM). (C) The heteromeric ASIC1b+3 current was half‐inhibited by 1 μM APETx2 (HP=−50 mV). (D) Concentration–response relationship for APETx2 block of ASIC2b+3 (•), ASIC1b+3 (▪), and ASIC1a+3 (○) currents. The concentration–response curve was fitted by the Hill equation. The IC50 values are 117 nM, 0.9 μM, and 2 μM (nH of 1, 0.9, and 0.9) for ASIC2b+3, ASIC1b+3, and ASIC1a+3, respectively. Each point is the mean±s.e.m. of data from three to eight cells.

Effects of APETx2 on the heteromeric ASIC1b+3 current

The ASIC1b channel is expressed in small‐ and large‐diameter sensory neurons (Chen et al, 1998; Alvarez de la Rosa et al, 2002; Mamet et al, 2002). Co‐expression of ASIC1b+3 subunits in COS cells using the pBudCE4.1 vector resulted in channels carrying a rapidly activating and inactivating current at pH 6, with an inactivation time constant of 346±183 ms (n=20), comparable to that of the ASIC3 current (440±135 ms, n=15, Figure 5C). A plateau phase was recorded at pH 5 and pH 4. Similar to the ASIC1a+3 current, the ASIC1b+3 current was inhibited by APETx2, but with a lower affinity than the ASIC3 current (IC50=0.9 μM, nH=0.9) (Figure 5D, ▪).

Effects of APETx2 on the heteromeric ASIC2b+3 current

Both ASIC2b and ASIC3 are expressed in small‐ and large‐diameter sensory neurons (Lingueglia et al, 1997; Voilley et al, 2001; Alvarez de la Rosa et al, 2002). Their coexpression in heterologous systems results in channels activated at acidic pH with a transient Na+‐selective current, followed by a sustained nonselective cation current (Lingueglia et al, 1997). The ASIC2b+3 sustained current can be recorded as an inward plateau at −50 mV (Figure 5Ba), and as an outward steady‐state current at +30 mV and above (Figure 5Bb). Independently of the holding potential, only the peak ASIC2b+3 current was inhibited by increasing concentrations of APETx2 (Figure 5Ba and b), with an IC50 of 117 nM (nH=1, Figure 5D, •).

Effects of APETx2 on the heteromeric ASIC2a+3 current

ASIC2a has been shown to be mainly expressed in medium‐ and large‐diameter sensory neurons (Garcia‐Anoveros et al, 2001; Alvarez de la Rosa et al, 2002) and has not been shown to be involved in nociceptor function. However, its contribution to native currents cannot be excluded as low ASIC2a levels have been detected in rat sensory neurons (Voilley et al, 2001; Alvarez de la Rosa et al, 2002). The ASIC2a+3 current recorded in transfected COS cells shows a typical biphasic current with a transient phase, followed by a plateau (Babinski et al, 2000; Baron et al, 2001). APETx2 (3 μM) blocked neither the rapid nor the slow component of the ASIC2a+3 current (not shown, n=5).

Effects of APETx2 on K+ channels

Due to its sequence homology with the BDS toxins and APETx1, APETx2 was tested on various heterologously expressed Kv channels. None of them (Kv1.4, HERG, Kv2.2, Kv3.1, Kv4.1, Kv4.2, Kv4.3) was significantly inhibited by 300 nM APETx2. Only the Kv3.4 current was partially inhibited by much higher concentrations (3 μM) of APETx2 (38±2%, n=6, not shown).

APETx2 inhibits ASIC3‐like currents in primary cultures of rat sensory neurons

ASIC3‐like currents were selected for their lack of sensitivity (less than 20% inhibition) to PcTx1 (Escoubas et al, 2000a), and for their typical kinetics and pH dependency (Mamet et al, 2002). Among the DRG neurons recorded, 26.5% expressed a PcTx1‐resistant ASIC3‐like current. This biphasic current could show either a Na+‐specific current as expected for homomeric ASIC3 channels, or a nonspecific sustained cation current, probably flowing through heteromeric ASIC2b+3 channels (Lingueglia et al, 1997) (Figure 6A). Neurons expressing a 10 μM capsaicin‐activated VR1 current were excluded. As shown by current traces in Figure 6B, APETx2 inhibited the ASIC3‐like current of sensory neurons in a concentration‐dependent manner when applied before the pH drop. However, the current was not fully inhibited by the toxin and 3 μM APETx2 reduced the ASIC3‐like current amplitude to 51±3% (n=11) of the control. The sigmoidal fit of the concentration‐dependent inhibition of the ASIC3‐like current by APETx2 shows an IC50 of 219 nM (Figure 6C). A mean IC50 of 216±49 nM (n=6) was calculated from IC50 values obtained from six different neurons. The effect of APETx2 was the same whether the ASIC3‐like current was activated at pH 6.3 or pH 5 (not shown).

Figure 6.

Effect of APETx2 on ASIC3‐like current in primary cultures of rat sensory neurons. (A) Original current traces of an ASIC2b+3‐like current showing typical ASIC3‐like kinetics at the holding potential of −50 mV and an outward sustained cation current at +30 mV. (B) Original current traces of ASIC3‐like current in the absence (control) and in the presence of increasing concentrations of APETx2 applied before the pH drop. This neuron expressed no VR1 current and the ASIC3‐like current showed a cation nonselective plateau phase (outward current at +30 mV, not shown). In this neuron, the ASIC3‐like current was maximally inhibited by 1–3 μM APETx2 to 47% of the control amplitude, and the fit of the concentration‐dependent block showed an IC50=203 nM. (C) Concentration–response curve of APETx2 inhibition of ASIC3‐like current. The amplitude of the current in the presence of toxin was expressed as a percentage of the amplitude of control current and plotted as a function of toxin concentration. Each point is the mean±s.e.m. of data from 5–17 cells. IC50=219 nM, nH=1. (D) Current‐clamp recordings of membrane potential variations induced by the same current pulses in control (top) and in the presence of 1 μM APETx2 (bottom) on the same neuron. Two potential traces are shown under each condition: one induced by an infraliminar current pulse and the other induced by a supraliminar current pulse inducing an action potential firing. APETx2 does not significantly modify action potential triggering or kinetics.

Experiments have been performed on ASIC‐like current recorded from sensory neurons of ASIC3 knockout adult mice (52 neurons, two primary cultures). These neurons do not express ASIC3‐like current. No ASIC2‐like current was recorded, consistent with previous observations that ASIC2a is essentially not expressed in DRG neurons (Lingueglia et al, 1997; Mamet et al, 2002). In 15% of recorded ASIC3/ DRG neurons, an ASIC1‐like current was recorded, which was blocked by the ASIC1a‐specific toxin PcTx1 (10 nM), but resistant to APETx2 (3 μM). This result is in agreement with the absence of inhibition of the recombinant ASIC1a current by APETx2.

APETx2 shares about 40% sequence homology with the Anthopleura sp. toxins, which are potent activators of voltage‐dependent Na+ channels (Romey et al, 1976; Kodama et al, 1981; Schweitz et al, 1981; Reimer et al, 1985). Therefore, we tested the effect of APETx2 on action potential triggering in sensory neurons. Figure 6D shows membrane potential variations induced by two current pulses, one infraliminar and the other reaching the action potential threshold, in the absence (top) and presence of 1 μM APETx2 (bottom) on the same neuron. APETx2 did not significantly modify the action potential triggering or its kinetics, eliminating the possible nonspecific effects on voltage‐dependent Na+ and K+ channels involved in the action potential of sensory neurons.

In vivo central injections of APETx2

Central injections of APETx2 in mice were administered to evaluate the toxicity and/or possible behavioral changes. Intracisternal injections of 5, 10, and 20 μg of APETx2 did not induce neurotoxic symptoms in mice even after 24 h. The behavior of injected mice was identical to that of control mice injected with physiological solution.


Animal venoms have provided a great variety of toxins, which have been successfully used as tools to characterize ion channels. The emergence of specific pharmacological tools for ASIC channels started with the discovery of Psalmotoxin 1 (PcTx1), a tarantula peptide that blocks with high specificity and affinity homomeric ASIC1a channels (Escoubas et al, 2000a, 2003). We have now isolated and characterized APETx2, the first toxin able to inhibit selectively ASIC3‐containing channels and ASIC3‐like currents in DRG neurons.

APETx2 reversibly inhibited the rat ASIC3 peak current with an IC50=63 nM, as well as the human ASIC3 peak current with an IC50=175 nM. Outside‐out patch recording demonstrated that APETx2 directly inhibits the ASIC3 channel, without any change in its unitary conductance. APETx2 also inhibits the heteromeric ASIC2b+3 channel with an IC50 of 117 nM and heteromeric ASIC1a+3 and ASIC1b+3 channels with lower affinities (IC50=2 and 0.9 μM, respectively).

Similar to amiloride, which has been shown to inhibit ASIC3 with an IC50=63 μM (Waldmann et al, 1997a), APETx2 blocks the peak ASIC3 current without affecting the sustained plateau. Analysis of structure–function relationships of the FaNaC channel, another member of the ENaC/ASIC family (Lingueglia et al, 1995), has previously shown that amiloride blocks the channel by entering into the pore structure (Poet et al, 2001).

Although APETx2 has sequence homologies with the Anthopleura sp. toxins (AP‐A, AP‐B, AP‐C), which are potent activators of voltage‐dependent Na+ channels (Romey et al, 1976; Kodama et al, 1981; Schweitz et al, 1981; Reimer et al, 1985), it does not modify the triggering or kinetics of the action potential in rat sensory neurons, thus showing no nonspecific effect on voltage‐dependent Na+ channels. This is not surprising as APETx2 was purified from a sea anemone peptide fraction devoid of paralytic activity (Bruhn et al, 2001). APETx2 was also non‐toxic to mice after i.c. injection using doses 100–1000‐fold higher than the known LD50 for AP‐A (AxI) or AP‐B (AxII) administered under the same conditions (Schweitz, 1984). Furthermore, the basic residues (Arg 12, Arg14, Lys 48, or Lys49 in AP‐A or AP‐B), which have been implicated in the toxin interaction with Nav channels (Barhanin et al, 1981; Gallagher and Blumenthal, 1994; Khera and Blumenthal, 1994; Loret et al, 1994), are absent in the APETx2 primary sequence. Similarly, hydrophobic (Trp 33 in AP‐B) or acidic residues (Asp7, Asp9 in AP‐B), also implicated in toxin binding to the Nav channel (Dias‐Kadambi et al, 1996; Khera and Blumenthal, 1996), are absent in APETx2.

The structure of APETx2 is more closely related to that of the K+ channel modulators BDS‐I, BDS‐II, and APETx1, purified, respectively, from Anemonia sulcata and Anthopleura elegantissima (Driscoll et al, 1989a, 1989b; Diochot et al, 1998, 2003). These short polypeptides are folded into three‐stranded antiparallel β‐sheets connected by three disulfide bonds whose location is similar to that of the long sea anemone Nav toxins (Norton, 1991; Loret et al, 1994). Although APETx2 shares 57, 55, and 76% sequence homologies with BDS‐I, BDS‐II, and APETx1, and has the same structural fold, its biological target is different. BDS‐I and BDS‐II are specific inhibitors of Kv3.4 channels, while APETx1 is a specific blocker of HERG K+ channels. Despite sequence homology with APETx1, the inhibitory effect of APETx2 appears to be specific for ASIC3‐containing channels. Toxin structure comparison reveals a highly conserved three‐dimensional scaffold, and also two toxin areas that are significantly altered by amino‐acid substitutions, probably leading to the different pharmacological profiles. As previously observed for other animal toxins, a similar scaffold is used as a basis for ‘combinatorial chemistry’, and slight alterations of toxin structure guide the selectivity toward different cellular receptors.

In vivo, ASIC‐like currents are the result of both homomeric and heteromeric associations of ASIC subunits (Bassilana et al, 1997; Babinski et al, 2000; Alvarez de la Rosa et al, 2002). In order to determine their respective contribution, tools are required that block heteromeric as well as homomeric channels. To this end, APETx2 is the first toxin known to inhibit homomeric ASIC3 channels in addition to several ASIC3‐containing heteromers, and thus represents a major pharmacological step in dissecting the molecular basis of acid‐induced currents in sensory neurons.

ASIC1a, ASIC1b, ASIC2b, and ASIC3 are often co‐expressed in sensory neurons (Lingueglia et al, 1997; Waldmann and Lazdunski, 1998; Alvarez de la Rosa et al, 2002; Mamet et al, 2002), and the inhibition of ASIC3‐like current by APETx2 could result from a combination of the various effects of APETx2 on the different ASIC3‐containing channels. The existence of ASIC2b+3 channels is identified by the nonspecific sustained cation current that can often be recorded following the transient ASIC3‐like peak (Figure 6A). ASIC1a+3 and ASIC1b+3 channels could also participate in the ASIC3‐like current, because their electrophysiological properties (activation and inactivation kinetics, plateau phase) cannot distinguish them from the ASIC3 homomeric channel. The presence of ASIC2a+3 channels is also possible as ASIC2a has now been identified in rat sensory neurons (Voilley et al, 2001; Alvarez de la Rosa et al, 2002), but the participation of homomeric ASIC2a channels can be ruled out in these experiments due to the low pH sensitivity of these channels (pH0.5=4.4, (Lingueglia et al, 1997; Baron et al, 2001)). As neurons expressing capsaicin‐sensitive VR1 current were excluded and homomeric ASIC1a current were blocked by PcTx1, the partial inhibitory effect of APETx2 on ASIC3‐like current in sensory neurons could then result from an inhibition of ASIC3 and ASIC2b+3 channels, in addition to a very partial inhibition of ASIC1a+3 and ASIC1b+3 channels.

The discovery of a toxin with ASIC3‐blocking activity is of major significance given the substantial amount of evidence now implicating this channel in the transduction of acid‐induced pain and hyperalgesia. ASIC3 channel activity is dramatically increased in the presence of lactate (produced under ischemic conditions), and is responsible for sensing and transmitting pain associated with myocardial ischemia (Immke and McCleskey, 2001). ASIC channel expression, particularly ASIC3, is upregulated by proinflammatory mediators including NGF, and has been implicated in sensory neuron hyperexcitability and hyperalgesia (Mamet et al, 2002, 2003). In addition, ASIC3 and ASIC3‐like currents are potentiated by neuropeptides that are overexpressed under inflammatory conditions (Deval et al, 2003).

Two independent groups reported that ASIC3 channels play a role in the modulation of pain sensation (Price et al, 2001; Chen et al, 2002), and it was recently shown that ASIC3, but not ASIC1, is involved in the development of acid‐induced mechanical hyperalgesia in skeletal muscle and central sensitization (Sluka et al, 2003). This finding is important for understanding the development of chronic musculoskeletal pain syndromes, and identifies ASIC3 as a potential therapeutic target for treatment or prevention of chronic hyperalgesia. In addition to studies in rat and mouse models, ASIC channels have been shown to be the primary acid sensors in human nociceptors in vivo (Ugawa et al, 2002). APETx2 is the first and so far the unique peptide toxin inhibitor of ASIC3‐containing channels. Along with PcTx1, APETx2 will be an important component of the pharmacological toolbox needed to determine the physiological involvement of ASIC channels in neuronal excitability and pain coding.

Materials and methods

Purification of APETx2 from Anthopleura elegantissima

A pool of polypeptides was isolated from a crude water–methanol extract of the sea anemone Anthopleura elegantissima (Bruhn et al, 2001) by anion exchange chromatography on QAE Sephadex A‐25 (4.5 × 400 mm) eluted with ammonium acetate (pH8.3), followed by gel filtration on Sephadex G50 (12 × 140 cm) in acetic acid 1 M. Six fractions were tested on ASIC3 channels expressed in Xenopus oocytes. One fraction, which inhibited 90% of the ASIC3 current, was further purified by reversed‐phase HPLC (Waters Symmetry C18, 4.6 × 250 mm), with a linear gradient from 10 to 40% of solvent B (10% acetonitrile/TFA 0.1%) in 30 min, at 1 ml/min. The separation was carried out on a HP1100 system (Hewlett Packard, USA) coupled to a diode‐array detector with UV absorbance monitoring at 220 and 280 nm. The active fraction was then purified on a TSK‐SP5PW (7.5 × 75 mm) cation exchange column (Tosoh, Japan) equilibrated in water/acetic acid 1% using a linear gradient from 0 to 100% ammonium acetate 1 M in 50 min at 1 ml/min. Final purification of APETx2 was carried out on the same reversed‐phase HPLC column, using a linear gradient from 20 to 30% in 10 min, followed by 30–40% solvent B in 20 min.

Peptide sequencing and mass determination

APETx2 was reduced with 2‐mercaptoethanol and alkylated with 4‐vinylpyridine prior to N‐terminal automated Edman sequencing (477A, Applied Biosystems, USA). The C‐terminal sequence of the peptide was confirmed by citraconylation of the arginine residues, followed by trypsin digestion. Tryptic fragments were separated by HPLC (Waters C18, 2 × 150 mm) using a 40 min linear gradient from 5 to 50% of acetonitrile/TFA 0.1% in water/TFA 0.1% at 200 μl/min. Sequence homologies were determined from a BLAST search ( Molecular mass determination was carried out by MALDI‐TOF Mass Spectrometry on a Voyager DE‐PRO system (Applied Biosystems, USA) in reflector mode, with α‐cyano‐4‐hydroxycinnamic acid matrix (Sigma‐Aldrich, USA) and internal calibration. Mass spectra were analyzed with Data Explorer software, and theoretical molecular masses were calculated from sequence data using GPMAW (

Disulfide bridge determination

The disulfide bond arrangement of APETx2 was determined using the partial reduction and cyanylation‐induced cleavage method (Wu et al, 1996; Qi et al, 2001). Briefly, 5 nmol of toxin was dissolved in 5 μl of citrate buffer (0.1 M, pH 3, 6 M guanidine HCl). Partial reduction was carried out by adding 150 nmol of tris(2carboxyethyl)‐phosphine hydrochloride (TCEP) and incubating for 20 min at 40°C. Cyanylation was achieved by adding a large excess (4000 nmol, pH 3) of 1‐cyano‐4‐(dimethylamino)pyridinium tetrafluoroborate (CDAP) and incubating for 15 min at room temperature. The mixture was diluted to 200 μl with water/0.1% TFA and separated by reversed‐phase HPLC using a linear gradient of 20–40% acetonitrile in water/TFA 0.1% over 40 min (Merck Purospher STAR C18 55 × 4.6 mm, 3 μm). After analysis by MALDI‐TOF mass spectrometry, fractions containing singly and doubly reduced isoforms were vacuum‐dried and dissolved in 2 μl of 1 M NH4OH (pH 8, 6 M guanidine HCl), to which was added another 8 μl of 1 M NH4OH for cleavage (1 h, room temperature). The NH4OH was removed under vacuum before complete reduction with 2 μl of 0.1 M TCEP (200 nmol, citrate buffer, pH 3) for 30 min at 37°C. Samples were desalted on reversed‐phase microcolumns (ZipTips C18, Millipore, USA) prior to MALDI‐TOF MS analysis.

Molecular modeling

A model of APETx2 was calculated from the previously described coordinates of APETx1 (Diochot et al, 2003), using the DeepView Swiss‐PDB viewer software v3.7 ( The model was optimized via the Swiss‐Model server ( BDS‐I coordinates (1BDS) were obtained from the PDB database (

Xenopus oocytes preparation, cRNA injections, and electrophysiological measurements

Oocytes preparation and cRNA injections have been previously described (Diochot et al, 1998) (see online Supplementary data). Rat ASIC3 cRNA was synthesized with the mCAP RNA capping kit (Stratagene). A rapid perfusion system allowed local and rapid changes of extracellular solutions. Depending on the pH range, solutions were buffered with HEPES (pH>6), MES (pH between 6 and 5) or acetate (pH<5).

COS cell transfections

COS‐7 cells were transfected with pCI‐rASIC1a, pCI‐rASIC1b, pCI‐rASIC2a, pCI‐rASIC2b, pCI‐rASIC3, and pCI‐hASIC3 as previously described (Lingueglia et al, 1997; Anzai et al, 2002). For heteromeric expression, cells were co‐transfected with pCI‐rASIC2a and pCI‐rASIC3 (1:1 ratio) or pCI‐rASIC2b and pCI‐rASIC3 (1:1 ratio), and with an expression vector containing the CD8 receptor cDNA, using the DEAE‐dextran method. The heteromeric expressions of ASIC1a+3 and ASIC1b+3 were achieved using the pBudCE4.1 vector (Invitrogen), which contains the human cytomegalovirus (CMV) immediate‐early promoter and the human elongation factor 1α‐subunit (EF‐1α) promoter for high‐level, constitutive, independent expression of two recombinant proteins. Rat ASIC3 (Accession Number # AAB69328) was subcloned under the control of the EF‐1α promoter, whereas rat ASIC1a (Accession Number # U94403) or rat ASIC1b (Accession Number # AJ309926) was subcloned under the control of the CMV promoter. K+ channels were expressed using 0.01 μg of pCI‐rKv1.4, pCI‐rKv2.2, pRc/CMV rKv3.4, 0.05 μg of pCI‐rKv4.1, pCI‐rKv4.2, pCI‐rKv4.3, and pSI‐rHERG per dish. Currents in COS‐7 cells were recorded at room temperature (22°C) within 1–2 days of transfection.

Primary culture of sensory neurons

Dorsal root ganglia were dissected from Wistar rats (5–7 weeks) and enzymatically dissociated with 0.1% collagenase. Cells were then plated on collagen‐coated 35 mm Petri dishes and maintained in culture at 37°C (95% air/5% CO2) in DMEM containing 5% fetal calf serum. Electrophysiological experiments were carried out 1 or 2 days after plating (Mamet et al, 2002).

Patch‐clamp recording

Currents were sampled at 3.3 or at 20 kHz for whole‐cell and outside‐out patch‐clamp recordings (Hamill et al, 1981), and low‐pass filtered at 3 kHz using pClamp8 software (Axon Instruments). Off‐line analysis of currents was performed using pClamp and Bio‐Patch (Bio‐Logic Science Instruments). The pipette solution contained (in mM): KCl 140, NaCl 5, MgCl2 2, EGTA 5, HEPES‐KOH 10 (pH 7.4) and the bath solution contained (in mM): NaCl 140, KCl 5, MgCl2 2, CaCl2 2, BSA 0.1%, HEPES‐NaOH 10 (pH 7.4). Depending on the pH range, solutions were buffered with HEPES (pH>6), MES (pH between 6 and 5) or acetate (pH<5). Solutions were applied locally by a rapid perfusion system. For experiments with sensory neurons, glucose 10 mM, CNQX 20 μM, and kynurenic acid 10 μM (to inhibit glutamate‐activated ionotropic currents) were added to the bath solution, and the pipette solution contained (in mM): KCl 140, ATP‐Na2 2.5, MgCl2 2, CaCl2 2, EGTA 5, and HEPES 10 (pH 7.3, pCa estimated to 7).


Concentration–response curves were fitted by the Hill equation:

Embedded Image

where I is the amplitude of relative current, Imax is the maximum current amplitude, Imin is the minimum current amplitude, C is the toxin concentration, IC50 is the toxin concentration that half‐maximally inhibited the current, and nH is the Hill coefficient. The results are expressed as mean±standard error of the mean (s.e.m.). Statistical significance was determined using the Student's t‐test (P<0.05*, P<0.01**, P<0.005***).

Mouse intracisternal injections

Anesthetized 5‐week‐old outbred OF1 (Charles River) mice were injected intracisternally with 1–5 μl APETx2 diluted in sterile NaCl solution (0.9% NaCl, 0.1% BSA). Symptoms were observed during the first hour after injection and at regular intervals over 24 h. Control mice were injected with 5 μl of NaCl solution.

Supplementary data

Supplementary data are available at The EMBO Journal Online.

Supplementary Information

Supplementary Figure [emboj7600177-sup-0001.pdf]

Supplementary Material [emboj7600177-sup-0002.pdf]


We thank D Moinier, M Jodar, and V Briet for technical assistance, and Dr L Beress for generously and kindly providing sea anemone extracts. This work was supported by the Centre National de la Recherche Scientifique (CNRS), the Ministère de la Recherche et de la Technologie, the Association pour la Recherche contre le Cancer (ARC), Astra Zeneca AB Research Area CNS/Pain, and the Association Française contre les Myopathies (AFM). LD Rash is supported by an INSERM/NH&MRC fellowship (ID 194470).


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