Abstract
We report here the purification of glycerotoxin from the venom of Glycera convoluta, a novel 320 kDa protein capable of reversibly stimulating spontaneous and evoked neurotransmitter release at the frog neuromuscular junction. However, glycerotoxin is ineffective at the murine neuromuscular junction, which displays a different subtype of voltage- dependent Ca2+ channels. By sequential and selective inhibition of various types of Ca2+ channels, we found that glycerotoxin was acting via Cav2.2 (N-type). In neuroendocrine cells, it elicits a robust, albeit transient, influx of Ca2+ sensitive to the Cav2.2 blockers ω-conotoxin GVIA and MVIIA. Moreover, glycerotoxin triggers a Ca2+ transient in human embryonic kidney (HEK) cells over-expressing Cav2.2 but not Cav2.1 (P/Q-type). Whole-cell patch–clamp analysis of Cav2.2 expressing HEK cells revealed an up-regulation of Ca2+ currents due to a leftward shift of the activation peak upon glycerotoxin addition. A direct interaction between Cav2.2 and this neurotoxin was revealed by co-immunoprecipitation experiments. Therefore, glycerotoxin is a unique addition to the arsenal of tools available to unravel the mechanism controlling Ca2+-regulated exocytosis via the specific activation of Cav2.2.
Keywords: Ca2+ channels/exocytosis/glycerotoxin/neuromuscular junction/neurotoxin
Introduction
Milestones in our understanding of synaptic functions have been reached using naturally occurring neurotoxins. Fashioned by billions of years of evolution and struggle for life between competing species, neurotoxins have the ability to incapacitate prey by interfering with synaptic processes at strategic points. This arms race has had beneficial scientific outcomes. Indeed, neurotoxins directly affecting neurotransmitter release have been used as tools for deciphering several aspects of exo- and endocytosis and to characterize the role of many of the proteins involved in these processes (Schiavo et al., 2000).
The sea worms Glycera convoluta (Figure 1A) are polychaete annelids which live in burrows on the shoreline of coastal regions and are highly active carnivorous predators. They detect their prey, mostly crustaceans and other polychaetes, by sensing hydrostatic changes and attack by shooting out an eversible proboscis (Figure 1B). The latter unveils four chitinous copper-containing fangs (Lichtenegger et al., 2002) used to inject their prey with its deadly venom. In the early 1980s, this venom was studied because of its ability to stimulate spontaneous quantal acetylcholine (ACh) release at the frog neuromuscular junction (NMJ) (Manaranche et al., 1980). The venom produces a prolonged but fully reversible high-frequency discharge of miniature end-plate potentials (MEPPs) without altering the ultrastructural features of the NMJ. For these reasons, the active compound is expected to be an invaluable tool for studying the regulation of synaptic vesicle recycling. Early attempts to purify the active component of the venom suggested that the biological activity was linked to a high-molecular-weight glycoprotein (Morel et al., 1983). However, to date, no further attempts have been made to isolate the toxin, to identify its receptor or to decipher its mode of action.
Herein, the successful purification and characterization of an active 320 kDa glycoprotein called glycerotoxin (GLTx) is reported. Using a strategy based on the phar macology of voltage-dependent Ca2+ channels (VDCCs), Cav2.2 (N-type Ca2+ channel) has been identified as the presynaptic target of GLTx. Notably, Cav2.2 channels are one of the main presynaptic Ca2+ channels involved in fast neurotransmitter release. They are assembled by the association of the channel-forming subunit α1B with the auxiliary subunits β and α2–δ, which act as modulators. Cav2.2 interacts, via a region of α1B called synprint, with members of the exocytotic apparatus allowing a tight control of vesicular release (Catterall, 2000; Jarvis and Zamponi, 2001).
GLTx elicits a transient Ca2+ influx sensitive to selective blockers of Cav2.2 in chromaffin cells and in human embryonic kidney cells (HEK293) over-expressing Cav2.2. Patch–clamp analysis showed that, upon addition of GLTx, the current–voltage relationship was shifted towards more hyperpolarized potentials promoting an up-regulation of current activity. This prompted us to investigate the effect of GLTx on nerve-evoked synchronous transmitter release, which revealed a sustained potentiation of phasic secretion. Finally, co-immunoprecipitation experiments showed that Cav2.2 was selectively recovered from brain synaptosomes in a complex with GLTx.
By specifically interacting with Cav2.2, GLTx represents a novel major tool with great potential to elucidate the role of Cav2.2 in a wide range of neuronal processes in both the central nervous system (CNS) and the peripheral nervous system (PNS).
Results
Purification of a secretagogue component from the venomous glands of the sea worm Glycera convoluta
To follow the purification of the secretagogue component from the venomous glands of G.convoluta, we have tested the ability of the venom to elicit catecholamine release from primary monolayer cultures of bovine chromaffin cells by fluorimetry (Meunier et al., 2000). Following the homogenization of the venomous glands (Figure 1B), chromaffin cells were exposed to the extract (0.3 mg/ml), which induced the release of ∼20% of their total catecholamine content with maximal secretion reached after 20 min (Figure 1C). This response was Ca2+ dependent as no stimulatory effect was observed in the absence of external Ca2+ (Figure 1C). This activity was lost after heating the extract at 100°C for 5 min (Figure 1C, insert), suggesting that the secretagogue could be a protein. Having established that these primary neurosecretory cells were suitable for testing fractions from the venom, we undertook the purification of the active component using bovine chromaffin cells as a functional assay. Previous studies have reported the partial purification of an active fraction, devoid of lipolytic or proteolytic activities, containing, among several other contaminants, a protein with an apparent molecular weight of 300 kDa (Morel et al., 1983). Therefore, the initial purification step was to clear the crude extract from low-molecular-weight proteins using a 100 kDa cut-off dialysis membrane. As expected, the dialysed material was still stimulating catecholamine release from chromaffin cells (Figure 1E). The active component was further purified using ion-exchange chromatography (Figure 1D). Interestingly, a 320 kDa band could clearly be observed on a silver-stained gel of the eluted fractions, exhibiting an ∼10-fold increase in the specific activity (Figure 1E and F). The active pool was concentrated, desalted and further purified by gel filtration, which achieved a doubling in the specific activity of the partially purified extract (Figure 1E and F). Finally, the neurotoxin was affinity purified using the known ability of the active component of the venom to bind concanavalin A (Con A) (Morel et al., 1983). This last step reduced the complexity of the purified fraction to three proteins: a 320 kDa band, a 148 kDa band and a 74 kDa band which was not always detectable (Figure 1F). Henceforth, this final fraction will be referred to as purified glycerotoxin. Based on the comparison of several purifications using the same or similar protocols, the activity of the purified neurotoxin clearly followed the distribution pattern of the 320 kDa band. Moreover, treatment of glycerotoxin for 1 h at pH 8.0 at room temperature in Tris buffer (50 mM) causes the selective disappearance of the 320 kDa band (Figure 1G), which is paralleled by an abolition of the secretagogue activity (data not shown). In these conditions the 148 kDa band remained unaffected, indicating that the active component of the venom is the 320 kDa protein (Figure 1G). In the presence of 2-mercaptoethanol, the 320 and 148 kDa proteins exhibit a decrease in their mobility to 335 and 176 kDa, respectively, suggesting that one or more internal disulphide bridges might affect the overall shape and mobility of the protein (data not shown). Peptide mass fingerprinting analysis indicates that the 320 kDa component does not correspond to any entry present in the DDBJ/EMBL/GenBank protein database (http://www. ncbi.nlm.nih.gov/BankIt), suggesting that GLTx is a novel protein.
GLTx increases spontaneous quantal ACh release at frog but not mouse neuromuscular junctions
The activity of GLTx was subsequently tested at the frog NMJ using the cutaneous pectoris muscle upon which the venom enhances spontaneous quantal transmitter release (Manaranche et al., 1980). At the frog NMJ, 0.05– 0.3 µg/ml of purified GLTx markedly enhanced spontaneous quantal transmitter release after only a few minutes delay, as detected by a sustained increase in the frequency of MEPPs (Figure 2A). To determine whether GLTx has similar effects on a mammalian NMJ, we tested it on the mouse extensor digitorum longus (EDL) nerve– muscle preparation. Interestingly, in this preparation, GLTx (0.05–10 µg/ml) was totally ineffective in modifying quantal spontaneous transmitter release (Figure 2B).
Therefore, we investigated established differences between the murine and frog components of the motor nerve terminals that could underlie such a discrepancy. Frog motor nerve terminals mainly contain Cav2.2 (Robitaille et al., 1990), whereas murine endplates express mainly Cav2.1 (Day et al., 1997; Katz et al., 1997). As both Cav2.2 and Cav2.1 interact with the secretory apparatus in neurons, a plausible explanation for the stimulatory effect of GLTx at the frog versus the mouse NMJ is that GLTx selectively acts on Cav2.2.
To test this hypothesis, frog neuromuscular preparations were pre-treated with ω-conotoxin-GVIA (ω-CTx-GVIA), a selective inhibitor of Cav2.2 (Olivera et al., 1985, 1999). Notably, this procedure abolishes the increase in asynchronous quantal ACh release in response to GLTx application, strongly implicating Cav2.2 as a target for GLTx (Figure 2C).
GLTx stimulates catecholamine release from bovine chromaffin cells by causing a transient influx of Ca2+ sensitive to Cav2.2 selective inhibitors
Bovine chromaffin cells are known to express Cav1, Cav2.2 and Cav2.1 (Artalejo et al., 1994; Garcia et al., 1998) and therefore provide an excellent model to pinpoint the subtype of VDCC involved in GLTx action. Pre-treatment of chromaffin cells with D600, a Cav1 blocker, or Agatoxin TK (Aga TK), a Cav2.1 blocker, thereby sparing Cav2.2, was unable to prevent the secretagogue activity of GLTx (Figure 3). However, the specific inhibition of Cav2.2 using ω-CTx-GVIA or ω-CTx-MVIIA (Olivera et al., 1985, 1999) blocked catecholamine secretion evoked by GLTx (Figure 3). These results demonstrate that GLTx stimulates catecholamine-containing secretory granule exocytosis by targeting Cav2.2.
Since Ca2+ is a general trigger for regulated exocytosis and the secretagogue activity of GLTx is strictly dependent upon the presence of external Ca2+ in chrom affin cells, we tested whether GLTx stimulates secretion by increasing intracellular Ca2+ as a result of a functional interaction with Cav2.2. To test this hypothesis, chromaffin cells were loaded with the Ca2+-sensitive dyes fura-2 or fluo-3. In the presence of Ca2+ in the external medium, application of GLTx (0.1–1.0 µg/ml) transiently increased intracellular Ca2+ (Figure 4A and B). Importantly, in an external medium devoid of Ca2+, addition of GLTx did not trigger any detectable Ca2+ rise (Figure 4C). However, subsequent addition of Ca2+ (2 mM) in the GLTx-containing medium resulted in a transient increase in intracellular Ca2+ (Figure 4C). These results demonstrate that GLTx triggers an influx of Ca2+ able to trigger catecholamine secretion from chromaffin cells.
To verify that this rise in intracellular Ca2+ signal was initiated by a GLTx-dependent influx through Cav2.2, we used selective inhibitors to block the different types of VDCC present in chromaffin cells before applying GLTx. Blockade of Cav1 with D600 (100 µM) did not significantly affect the GLTx-induced Ca2+ transient (Figure 4D). Similarly, pre-treatment with Aga TK (1 µM), a Cav2.1 blocker, was unable to block this effect (Figure 4D).
In contrast, when chromaffin cells were monitored in the presence of ω-CTx-MVIIA (2 µM), a reversible Cav2.2 blocker, GLTx application did not result in any detectable increase in Ca2+ (Figure 4E). Interestingly, when the same cells were washed and monitored again, application of GLTx alone was capable of eliciting an increase in intracellular Ca2+ (Figure 4E). Altogether, these results demonstrated that Cav2.2 is necessary for GLTx to trigger an influx of Ca2+ and to stimulate catecholamine neurosecretion from chromaffin cells.
GLTx triggers an influx of Ca2+ in human embryonic kidney cells transiently transfected with Cav2.2 but not with Cav2.1
To examine whether the presence of Cav2.2 is sufficient for GLTx to trigger Ca2+ influx, we used the heterologous HEK cell system transiently transfected with either Cav2.2 or Cav2.1. The expression of Cav2.2 and Cav2.1 on the plasma membrane was checked by immunocytochemistry (data not shown). After establishing that the intracellular Ca2+ level in untransfected cells was not affected by GLTx (0.1–1.0 µg/ml) (not shown), we over-expressed various subunits encoding Cav2.2 or Cav2.1. Only cells over-expressing the Cav2.2 subunits α1B in the presence of β subunit (± α2–δ) responded to the application of GLTx with a robust transient intracellular Ca2+ signal (Figure 5, insert). Moreover, pre-incubation of HEK cells expressing Cav2.2 with ω-CTx-GVIA totally prevented this Ca2+ signal (Figure 5, grey bar and insert). To show that GLTx was acting on Cav2.2 exposed on the plasma membrane, HEK cells were transfected with α1B subunit only. β3 is required to overcome an endoplasmic reticulum (ER) retention signal present in the α1 subunit, and failure to co-express β subunit results in a lack of expression of the channel at the plasma membrane (Walker and De Waard, 1998; Bichet et al., 2000). These cells were insensitive to GLTx, clearly demonstrating that the toxin acts extracellularly on Cav2.2 present on the plasma membrane (Figure 5). Importantly, the level of Ca2+ in response to GLTx exposure remained unaffected in HEK cells transfected with α1A (± β3 ± α2–δ) encoding Cav2.1.
Anti-GLTx monoclonal antibodies co-immunoprecipitate Cav2.2
To investigate a possible direct interaction between GLTx and Cav2.2, GLTx-interacting proteins were co-immunoprecipitated from solubilized rat brain membranes (LP1) using a monoclonal antibody against purified GLTx. In the screening procedure, we selected a positive clone, named 4G9, which recognized purified GLTx on dot-blot (Figure 6A) and was able to immunoprecipitate GLTx from both the purified GLTx (Figure 6B) and crude extract (data not shown). In western blotting, 4G9 antibodies recognized not only the 320 kDa band specific for the active toxin (Figure 6B) but also the 148 kDa band, suggesting that the latter is a degradation product of the former (data not shown).
Immunoprecipitation of GLTx followed by incubation with solubilized rat brain membranes led to the specific recovery of Cav2.2 as evidenced by probing for the α1B subunit in western blotting (Figure 6C). Moreover, co-immunoprecipitation revealed that GLTx could pull down up to 25% of the total [125I]ω-CTx-GVIA binding sites corresponding to α1B from detergent extracts of rat brain membranes (Figure 6D). These results confirm biochemically the specificity of the interaction between GLTx and Cav2.2.
Patch–clamp analysis of the action of GLTx
Whole-cell patch–clamp recordings were carried out on N-type Ca2+ channels (α1B + α2–δ + β2a) transiently expressed in HEK tsA-201 cells. At depolarized potentials, a small reduction in the maximum slope conductance could be observed, resulting in current inhibition at positive potentials (Figure 7A and C). Importantly, GLTx (0.03 µg/ml) significantly shifted the current– voltage relationship to more hyperpolarized potentials by about 10 mV. Hence, at hyperpolarized test potentials, GLTx promotes an up-regulation of current activity resulting in a large increase in peak current amplitude when test potential is stepped to –10 mV (Figure 7A, B and C). The enhanced inward current was slowly reversible and could be blocked by subsequent application of ω-CTx-MVIIA, indicating that it resulted from an up-regulation of N-type channel activity (Figure 7B, insert).
The 10 mV shift in half activation potential produced by GLTx is irrespective of the nature of the β subunit (Figure 7D). Moreover, as in the case of β2a (see Figure 7A), a small degree of inhibition was observed at more depolarized potentials when the other three β subunits were co-expressed (not shown). Given the similar shifts in half activation potential, a similar level of up-regulation of current activity could be predicted at negative test potentials, and was indeed observed (Figure 7E). GLTx did not significantly affect the voltage dependence of inactivation for channels containing the β1b or β2a subunit (n = 4, not shown). At higher concentrations (0.25 µg/ml), GLTx almost completely inhibited N-type channel activity (data not shown). This might indicate that GLTx has two separate sites of action on the N-type channel molecule: one high affinity linked to changes in gating properties, and a second low affinity that results in block of current activity.
Therefore, taken together, our data suggest that the size of the window current is increased in the presence of GLTx, thus leading to increased Ca2+ influx.
GLTx increases phasic neurotransmitter release at the frog neuromuscular junction by enhancing the quantal content of endplate potentials
Since GLTx was found to shift the current–voltage relationship of Cav2.2 channels towards more depolarized values, it was of interest to investigate whether the phasic quantal transmitter release was also modified. Therefore the pectoralis propius motor nerve, innervating the frog cutaneous pectoris muscle, was stimulated by single pulses at a low rate (0.2 Hz) and the evoked responses were recorded under conditions in which neurotransmitter release had been reduced by lowering external Ca2+ concentration and increasing Mg2+ concentration. Upon GLTx application, an increase in endplate potential (EPP) amplitude was detected, which depended on the dose (0.1–0.5 µg/ml) reaching up to 10 times control levels. The quantal content of the evoked responses (estimated by dividing EPP by MEPP amplitude) was clearly enhanced and this sustained effect was reversible by simple wash (Figure 8). At higher concentrations, GLTx induced a blockade of evoked release (data not shown) consistent with the blockade of Ca2+ currents observed in patch– clamp experiments at such concentrations. These results clearly demonstrate that GLTx acts presynaptically by modifying the biophysical properties of Cav2.2 channels, thereby promoting the synchronous recruitment of an increased number of synaptic vesicles for phasic release.
Discussion
In this study, the purification and characterization of GLTx, a 320 kDa protein stimulating exocytosis of large dense core vesicles in neuroendocrine cells and small synaptic vesicles from frog motor nerve terminals, is described. Involvement of Cav2.2 was first revealed using selective inhibitors of the various subtypes of VDCC. Moreover, GLTx was found to trigger Ca2+ influx in cells heterologously expressing Cav2.2 and to interact with this subtype of Ca2+ channel by co-immunoprecipitation from synaptosomes.
Previous attempts to isolate the active component responsible for the secretagogue activity of G.convoluta venom attributed the activity to a 300 kDa glycoprotein. However, the purity of the final fraction obtained by affinity chromatography using Con A–Sepharose was not refined enough as a number of contaminant proteins were detected (Morel et al., 1983). To overcome this problem, additional purification steps have been introduced in this study to eliminate the contaminating glycoproteins before proceeding with the Con A affinity chromatography. Since the active component had been reported to be around 300 kDa, the novel purification protocol was begun by dialysis using a membrane with a 100 kDa cut-off. Following this, ion-exchange and gel filtration steps were introduced prior to the final affinity chromatography. This protocol allowed the purification of three proteins with apparent molecular weights of 320, 148 and 74 kDa. The specific activity typically increased by a factor of more than 1000 during the purification procedure.
Although the ratio of the upper to the lower band differed from preparation to preparation, the level of secretagogue activity exclusively correlated with the abundance of the 320 kDa protein. This was further substantiated by the discovery that mild alkalization caused the selective disappearance of the 320 kDa band and concomitant abolition of the secretagogue activity. As both the 320 and 148 kDa bands were recognized by a monoclonal antibody raised against the active toxin, it is likely that the 148 kDa species is a degradation product of the 320 kDa protein.
The high specific activity of the purified fraction makes GLTx one of the most active toxins yet discovered, working in the picomolar range at the frog NMJ, similar to α-latrotoxin (LTX) from the black widow spider Latrodectus mactans tredecimguttatus (Davletov et al., 1998; Südhof, 2001) and trachynilysin from the stonefish Synanceia trachynis (Meunier et al., 2001). The stimulatory activity of LTX mainly depends on the cation-conducting pore formed by LTX, which has been shown to exploit the extracellular domains of two presynaptic proteins to promote its insertion into the plasma membrane (Davletov et al., 1998; Volynski et al., 2000; Südhof, 2001). An important consequence of this insertion is that LTX effect is irreversible, which is in striking contrast with the equally potent but easily reversible stimulatory effect of GLTx. This strongly suggests that the strategy employed by the two toxins to stimulate neurotransmitter release is different.
Insight into the mode of action of GLTx was provided by the discovery that it had no effect at the mouse EDL nerve–muscle preparation. In fact, GLTx proved to be non-toxic when injected in mice intraperitoneally, even at the high doses used for immunization. In sharp contrast, GLTx potently enhanced spontaneous and evoked quantal transmitter release at the frog NMJ. Despite being widely expressed in the mammalian CNS (Jones et al., 1997), Cav2.2 channels are absent from the adult peripheral motor nerve terminals (Day et al., 1997; Katz et al., 1997). Thus Cav2.2 became an obvious candidate for mediating GLTx action. This hypothesis was confirmed by pre-treatment of frog NMJ preparation by ω-CTx-GVIA, which completely prevented GLTx stimulatory effect. The unique involvement of Cav2.2 was gathered using chromaffin cells, which are known to express three major types of VDCC: Cav1, Cav2.1 and Cav2.2 (Artalejo et al., 1994; Garcia et al., 1998). By sequentially inhibiting each of the subtypes, it became clear that only Cav2.2 was responsible for mediating the toxin’s effect.
Attention was then turned to elucidating the mechanism by which GLTx stimulates exocytosis via Cav2.2 channels. An increase in synaptosomal Ca2+ level in response to G.convoluta venom has previously been reported (Madeddu et al., 1984). Our study suggests that GLTx triggered Ca2+ influx through Cav2.2 channels, which in turn is believed to initiate exocytosis. GLTx triggers an influx of Ca2+ sensitive to ω-CTx-GVIA in neuroendocrine cells and transient expression of Cav2.2 rendered HEK cells responsive to GLTx.
This evidence points to an interaction between GLTx and presynaptic Cav2.2. Cav2.2 is comprised of three subunits: α1B, β and α2–δ. The channel subunit α1B is known to be retained in the ER when not co-expressed with a β auxiliary subunit, the latter being responsible for the targeting of α1B to the plasma membrane by binding to its ER retention signal (Walker and De Waard, 1998; Bichet et al., 2000). HEK cells transfected solely with cDNA encoding the α1B subunit of Cav2.2 were insensitive to GLTx action and sensitivity was conferred only upon co-expression of β3. This result, together with the reversibility of GLTx stimulatory effect by simple wash, clearly demonstrates that GLTx acts on Cav2.2 only when expressed at the plasma membrane.
The interaction between Cav2.2 and GLTx, demonstrated by co-immunoprecipitation using antibodies against GLTx, is particularly interesting in light of the central role played by Cav2.2 in coordinating several proteins of the secretory apparatus. Indeed, Cav2.2 has been shown to interact directly with SNARE family members and synaptic vesicle proteins, ensuring that synaptic vesicles are tightly bound to a source of Ca2+. Syntaxin, SNAP-25 and synaptotagmin bind to the synprint region of Cav2.2, altering the gating properties of Cav2.2 channel (Catterall, 2000; Jarvis and Zamponi, 2001). Recently, RIM binding proteins were shown to interact with several subtypes of Ca2+ channels including Cav2.2 and to functionally control the strength of secretion (Hibino et al., 2002). Future work will address whether GLTx can perturb this equilibrium.
Electrophysiological analysis was performed on transiently transfected HEK tsA-201 cells using patch whole-cell recordings. GLTx induces a leftward shift in the current–voltage relationship in Cav2.2-expressing cells. As a consequence of this increase in window current, the amplitudes of the elicited Ba2+ current increased more than threefold (340 ± 60%) compared with untreated cells upon depolarization from –80 mV to –10 mV. The fact that channels containing the β3 subunit could undergo a GLTx-evoked increase in the current is consistent with the Ca2+ influx detected upon GLTx addition in HEK cells co-expressing α1B and the β3 rabbit orthologue (Figure 5).
Since GLTx induced an up-regulation of Ca2+ currents, we investigated the effect of GLTx on nerve-evoked synchronous quantal transmitter release. We found that the size of the EPPs was greatly enhanced upon addition of GLTx and remained higher for as long as our experiment lasted. Interestingly, this effect was fully reversible by simple wash. To ascertain that this was a presynaptic effect the quantal content was measured using the ratio method, which confirmed that the number of quanta entering into the composition of EPPs was enhanced by as much as 10 times (Figure 8). In contrast with several neurotoxins that only stimulate spontaneous neurotransmitter release (Schiavo et al., 2000), GLTx also enhanced evoked phasic quantal ACh release. This clearly indicates that upon arrival of an action potential, the enhanced elicited Ca2+ influx through Cav2.2 increases the number of synaptic vesicles recruited to build up an EPP.
To date, most compounds found to act selectively upon Ca2+ channels are inhibitory (Garcia et al., 1998). To the best of our knowledge, only a dihydropyridine derivative (Bay k 8644) has been shown to activate Cav1 by favouring the open state of this channel (Hess et al., 1984). Cav1 is found in skeletal, smooth and cardiac muscles and in neuroendocrine cells (Catterall, 2000; Fisher and Bourques, 2001). In contrast, Cav2.2 is mostly present in neurons of the CNS and in neurons involved in digestive functions in the PNS (Garcia et al., 1998) and is functionally coupled with the exocytic machinery controlling secretion. In this context, GLTx provides a novel and unique tool to study secretion in these neurons and to investigate the functional interaction between Cav2.2 and the exocytotic machinery at the molecular level.
Materials and methods
Gland dissection
Glycera convoluta specimens were obtained from the Marine Biological Station, Roscoff (France) and the glands were isolated as previously described (Manaranche et al., 1980) and stored at –80°C.
Scanning electron microscopy
Glycera convoluta were fixed in 4% paraformaldehyde in Sorensen’s phosphate buffer. Fixed animals were dehydrated in ascending ethanol concentrations, washed twice in acetone before critical point drying, mounted and coated with platinum. Samples were examined with a JEOL 5600 field emission scanning electron microscope.
Purification of GLTx
Two hundred glands were thawed, homogenized in 10 mM sodium phosphate buffer (pH 7.2) on ice using a glass–Teflon homogenizer and centrifuged for 5 min at 16 000g. The supernatant was kept on ice and the pellet extracted again as above. Supernatants were pooled, clarified by centrifugation (20 min at 16 000g) and dialysed for 24 h in a Float A Lyser™ with a 100 kDa molecular weight cut-off (Spectrum, Perbio Science, UK). The dialysed extract was then fractionated by ion-exchange chromatography on a Resource Q column (Amersham Pharmacia Biotech, UK). Bound material was eluted using a linear NaCl concentration gradient (0–1 M in 10 mM sodium phosphate buffer pH 7.2).
Fractions were tested for their ability to stimulate catecholamine release from cultured bovine adrenal chromaffin cells. Active fractions were pooled and concentrated (3 h dialysis 15% (w/v) addition polyethylene glycol (PEG) 20 000 15% (w/v) in a 10 mM sodium phosphate buffer (pH 7.2) before fractionation on a Superdex™ 200 column (Amersham Pharmacia Biotech, UK). Active fractions were pooled and further purified by affinity chromatography on Con A– Sepharose™ (Amersham Pharmacia Biotech, UK). Bound material was eluted with 0.25 M α-methyl-d-mannoside (Sigma, UK) and concentrated by dialysis against 15% PEG as described above. Protein concentration was determined using Bradford protein assay (Biorad, UK). The specific activity was calculated as the percentage of total catecholamine release per milligram of protein (Figure 1E).
Neuromuscular junction preparations
Cutaneous pectoris nerve–muscle preparations were removed from frog (Rana esculenta; 25–30 g) and pinned in a Rhodorsil-lined Plexiglas chamber containing a standard frog Ringer solution (115.0 mM NaCl, 2.1 mM KCl, 1.8 mM CaCl2 and 5 mM HEPES–NaOH pH 7.25). To avoid spontaneous contraction, some preparations were pre-treated with tetrodotoxin (TTX, 1 µM). Studies on nerve-evoked quantal transmitter release were performed in solutions containing low Ca2+ (1 mM) and high Mg2+ (6 mM) concentrations. The EDL muscle was removed from adult Swiss-Webster mice (25–30 g) and pinned in a similar Rhodorsil-lined chamber containing continuously oxygenated Krebs–Ringer solution (151 mM NaCl, 5 mM KCl, 1 mM MgCl2, 2 mM CaCl2, 11 mM glucose and 5 mM HEPES–NaOH pH 7.4).
Cell culture and transfection
Exponentially growing human embryonic kidney (HEK 296 or HEK tsa-201) cells, seeded at 2 × 106 cells/10 cm dish, were transfected by calcium phosphate (Feng et al., 2001a) for patch–clamp experiments and electroporation for monitoring Ca2+ variations (400 V; infinity resistance, 125 µF) using a Gene Electropulser II (BioRad, CA) with 10 µg of total DNA using equimolar ratios of expression constructs encoding the following subunits of VDCC: α1A (Mori et al., 1991), α1B (Fujita et al., 1993), α2–δ (Kim et al., 1992), β3 (Witcher et al., 1993), β1b, β2a and β4 (Feng et al., 2001b).
Electrophysiological recordings
MEPPs and EPPs were recorded at room temperature (22°C) with an intracellular glass capillary microelectrode filled with 3 M KCl (8–12 Ω) using conventional techniques. The motor nerve of the isolated NMJ preparation was stimulated via a suction microelectrode. After amplification, electrical signals were digitized, displayed on an oscilloscope and simultaneously recorded on videotape with the aid of a modified digital audio processor (Sony PCM 701 ES) and a videocassette recorder (Sony SLC 9F). Data were collected and analysed with scan, software kindly provided by Dr John Dempster (University of Strathclyde, UK) running on a PC equipped with an analogue–digital converter (Model DT2821, Data Translation, MA).
Whole-cell patch–clamp recordings were performed as described previously (Feng et al., 2001b). GLTx dissolved in the recording solution [5 mM BaCl2, 1 mM MgCl2, 10 mM HEPES, 40 mM TEA-Cl, 10 mM glucose, 97.5 mM CsCl (pH 7.2 adjusted with TEA-OH)] was perfused onto the cells using a gravity-driven perfusion system. Current–voltage relations exported from Clampfit (Axon Instruments, CA) were fitted with Sigmaplot 4.0 (Jandel Scientific, CA) using the Boltzmann relation
I = {1/(1 + exp(–(Vm – Va)/k))}{G(Vm – Erev)}
where Vm is the test potential, Va is the potential at which half of the channels are activated, G is the maximal slope conductance, Erev is the reversal potential and k is the slope of the activation curve.
Culture of bovine adrenal chromaffin cells, and stimulation and quantification of catecholamine secretion
Chromaffin cells were prepared from bovine adrenal glands and maintained as primary cultures in 24-well plates (Nunc, UK) as previously described (Meunier et al., 2000). Chromaffin cells were briefly washed once with buffer A (145 mM NaCl, 5 mM KCl, 1.2 mM Na2HPO4, 10 mM glucose and 20 mM HEPES–NaOH pH 7.4), and processed as stated in the figure legends. Aliquots of the medium were taken at the end of each experiment and cells were lysed with 1% (v/v) Triton X-100 (Sigma, UK). Both sets of samples were assayed fluorimetrically for catecholamine content, and the amounts released were expressed as a percentage of the total amount of catecholamine present in the cells. Plotted data are representative of at least four independent experiments, each carried out in quadruplicate.
Intracellular Ca2+ imaging
Chromaffin and HEK cells cultured on glass bottom (no. 1.5) dishes (MatTek Corporation, MA) coated with poly-l-lysine (0.1 mg/ml; Sigma, UK) were loaded with the acetoxymethyl ester form of fura-2 or fluo-3 [5 µM with 0.02% pluronic acid (w/v) for 45 min at 37°C in the dark] in Buffer A or Hanks’ buffer (136 mM NaCl, 5.36 mM KCl, 0.81 mM MgCl2, 1.26 mM CaCl2, 0.44 mM KH2PO4, 0.81 mM MgSO4, 0.42 mM Na2HPO4, 11 mM glucose and 20 mM HEPES–NaOH pH 7.4), respectively. After washing and incubation at 37°C for 15 min, the dishes were placed in an environmental chamber (37°C) on the stage of a confocal (LSM510, Zeiss, Germany) or epifluorescent microscope (Diaphot 300, Nikon, UK) equipped with Plan Fluor 40×, 60× or 100×, N.A. 1.3 oil-immersion lenses. For confocal Ca2+ imaging, fluo-3-loaded cells were processed as previously described but using the above-mentioned objectives (Meunier et al., 2000).
For ratiometric measurement of intracellular Ca2+, fura-2-loaded cells were alternatively excited through 340 and 380 nm filters and images were acquired using a cooled CCD camera (Orca I, Hamamatsu, Japan) controlled by AQM2000 software (Kinetic Imaging, UK). Images were taken at 5 s intervals and ratios obtained using Lucida (v.4.0; Kinetic Imaging, UK).
The index of the fluorescence variations ΔF/F0 used to quantify the relative changes of intracellular Ca2+ was calculated as follows:
ΔF/F0 = [(f340/f380)i – (f340/f380)max] / (f340/f380)i
where (f340/f380)i is the initial fluorescence ratio measured before application of the relevant drug or toxin and (f340/f380)max is the maximal fluorescence ratio taken at the peak of the effect.
Preparation of anti-GLTx monoclonal antibodies
Balb/c mice were immunized by intraperitoneal injections (every 4 weeks) of 50 µg of purified GLTx. Serum and hybridoma supernatants were tested for their ability to inhibit GLTx secretagogue activity in chromaffin cells. The clone 4G9 was singled out for its ability to partially inhibit the stimulatory activity of both the venom and purified GLTx and to recognize purified GLTx in dot-blots and western blotting.
Immunoprecipitation and western blotting
Crude synaptosomes were prepared from rat brain cortex following the method of Huttner et al. (1983) with minor variations. Seventy milligrams of synaptic plasma membranes (LP1) were solubilized in 10 mM HEPES–NaOH pH 7.4 containing protease inhibitors (Pefabloc, Roche Boehringer Mannheim, Germany) and 4% octyl-β-d-glucopyranoside (OG) for 1 h. In some experiments, 5 mg of LP1 were pre-incubated for 1–2 h with [125I]ω-CTx-GVIA (0.5 µCi; NEN, UK), washed twice by ultracentrifugation and solubilized as described above. Detergent-free buffer was added to dilute the OG to a final concentration of 1.2% and the insoluble material was removed by centrifugation. The extract was pre-incubated for 2–4 h at 4°C with Protein G–Sepharose (Roche Boehringer Mannheim, Germany) coupled or not with 4G9 monoclonal antibodies with or without pre-binding of GLTx for 2 h (at concentrations indicated in Figure 6).
Protein samples were heated at 100°C for 3 min in 2% SDS sample buffer, and proteins were resolved in 8% or 12% SDS–polyacrylamide gels. Proteins were transferred (200 mM glycine, 25 mM Tris–OH, 10% methanol) to nitrocellulose membrane (0.2 µm; Schleicher and Schuell, UK), blocked in TBST (20 mM Tris–HCl pH 7.6, 137 mM NaCl, 0.05% Tween 20) containing 1% ovalbumine (w/v) and 1% polyvinylpyrrolidone (w/v) and probed for 2 h with indicated antibodies diluted in blocking solution (mouse anti-GLTx, 0.1 µg/ml; rabbit anti-α1B, 8 µg/ml; Cambridge Bioscience, UK). After washing three times with TBST, the membranes were incubated with the appropriate HRP-conjugated secondary antibody in blocking solution (1:2000) for 1 h, washed and revealed by enhanced chemoluminescence (ECL; Amersham Pharmacia Biotech, UK).
Drugs and toxins
Aga TK (Alomone, Israel); ω-CTx-GVIA (Calbiochem, UK); ω-CTx-MVIIA (Alomone, Israel); Verapamil (D600) (Sigma, UK); TTX (Sigma, UK); fluo-3/AM and fura-2/AM (Molecular Probes, The Netherlands).
Statistical analysis
Statistical analysis was performed using Student’s t-test (two-tailed, paired or unpaired depending on the experimental protocol). Values are expressed as mean ± SEM and data were considered significant (*) at P < 0.01.
Acknowledgments
Acknowledgements
We thank S.L.Osborne for LP1 preparation and excellent suggestions, S.Tooze, D.Shima and M.Seagar for critical reading of the manuscript, S.Gschmeissner for electron microscopy and B.Adams for the kind gift of the plasmids encoding Ca2+ channels. This work was supported by Cancer Research UK (F.A.M. and G.S.), by the Direction des Systemes de Forces et de la Prospective (J.M.), by an operating grant from the Heart and Stroke Foundation of Alberta and the Northwest Territories (G.W.Z.) and by travel grant BC 00156SE from the British Council (F.A.M., J.M. and G.S.). Z.P.F. holds postdoctoral awards from the Canadian Institutes of Health Research (CIHR) and the Heart and Stroke Foundation of Canada. G.W.Z. is a CIHR Investigator and a Senior Scholar of the Alberta Heritage Foundation for Medical Research.
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