From the ¶ Endocrine Laboratory, Royal Victoria Hospital,
Montreal, Quebec H3A 1A1, Gastroenterology Division,
Department of Pediatrics, Montreal Childrens Hospital Research
Institute, and Faculty of Medicine, McGill University, Montreal,
Quebec H3H 1P3, Canada
![]() |
ABSTRACT |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
We have used a sensitive bioassay of calcium-mediated volume changes in mammalian absorptive intestinal epithelial cells to screen extracts of the skin of the amphibian Xenopus laevis for the presence of factors affecting ion transport. A 66-residue peptide, purified using reversed-phase high performance liquid chromatography techniques, caused isotonic volume reduction of guinea pig jejunal villus cells in suspension. This volume reduction required extracellular Ca2+ and was prevented by the dihydropyridine-sensitive Ca2+ channel blocker niguldipine. Structural analysis demonstrated the presence of eight cysteines and a primary structure homologous to that of the neurotoxin/cytotoxin family found in the venom of certain poisonous snakes. The structure of the peptide was identical to that of xenoxin-1 purified from dorsal gland secretions of X. laevis (Kolbe, M., Huber A., Cordier, P., Rasmussen, U., Bouchon, B., Jaquinod, M., Blasak, R., Detot, E., and Kreil, G. (1993) J. Biol. Chem. 268, 16458-16464). Xenoxin-1 (10 nM) caused volume changes that required extracellular Ca2+ and were comparable in magnitude and direction to changes caused by BayK-8644 (100 nM), a dihydropyridine-sensitive Ca2+ channel agonist. The initial rate of dihydropyridine-sensitive 45Ca2+ influx was substantially increased by xenoxin-1. Staurosporine (10 nM) prevented volume changes caused by ATP (250 µM) but had no effect on volume changes caused by BayK-8644 or xenoxin-1. We conclude that xenoxin-1 directly activated dihydropyridine-sensitive Ca2+ channels in villus cells and that a mammalian homologue to xenoxin-1 may exist.
![]() |
INTRODUCTION |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
Frog skin, which is a multilayered epithelium, is a rich source of peptides with diverse biological functions (1-3). Originally used in tracer flux experiments (4), frog skin has recently been used as a model system for studying volume regulation (5). Frog skin peptides are similar or identical to hormones and neurotransmitters of mammalian origin. Numerous amphipathic antibacterial peptides have also been purified from amphibian skin exudates and tissue extracts (6). Since frog skin is an epithelium, it was originally speculated that some peptides could be regulators of electrolyte homeostasis (7).
The isotonic volume of mammalian intestinal epithelial cells is
regulated by salt transport (8). Increasing the rate of salt efflux
(i.e. K+ and Cl ions) results in a
volume reduction of these epithelial cells (9). Previously, we have
shown that members of the defensin family of peptides will
differentially activate isotonic volume changes in mammalian intestinal
epithelial cells (10). These 29-34-residue cationic peptides contain a
consensus distribution of six cysteine residues aligned in a highly
conserved fashion (11). Homogeneous populations of viable mature villus
epithelial cells can be isolated in suspension (8, 12, 13), and their volume can be accurately determined using electronic cell sizing (14).
We have used isotonic volume changes in this cell preparation as a
bioassay to facilitate the purification of peptides that activate
electrolyte efflux from extracts of amphibian skin.
In this report, we describe the isolation and characterization of a peptide from the dorsal skin of Xenopus laevis, which activates dihydropyridine-sensitive Ca2+ channels in guinea pig villus epithelial cells. This peptide shows structural similarity to the cytotoxin and neurotoxin family of peptides found previously only in the venom of poisonous snakes. While these studies were in progress, an identical peptide was characterized by other investigators as xenoxin-1 (15).
![]() |
MATERIALS AND METHODS |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
Reagents-- The acetoxymethylester of 1,2-bis-(2-aminophenoxy)ethane-N,N,N1,N1-tetraacetic acid (BAPTA)1 was obtained from Molecular Probes (Eugene, OR). Niguldipine was from Research Biochemicals (Natick, MA) and N-methyl-D-glucamine from Aldrich. EGTA was from Sigma and RPMI 1640 (10×) medium from Life Technologies, Inc. (Burlington, Ontario). Dinonylpthalate was from Pfeltz and Bauer (Waterbury, CT), and 45CaCl2 was purchased from ICN Biomedicals (Montreal).
High Performance Liquid Chromatography (HPLC)-- Chromatography was undertaken using a Waters Associates (Milford, MA) HPLC system consisting of two 510 pumps and a gradient controller. Column eluates were monitored for UV absorbance at 210 and 280 nm using LDC (Riviera Beach, FL) and Beckman (Palo Alto, CA) detectors connected in series. HPLC solvents and reagents were prepared as described previously (16). Reversed-phase HPLC was undertaken using Waters C18 µBondapak and C18 Vydac TP201 (Cole Palmer, Chicago, IL) columns, which were eluted as described previously (16). Gel permeation HPLC was performed using two Waters I-125 columns connected in series, which were eluted as described previously (17).
Tissue Extraction and Peptide Purification-- A female X. laevis was purchased from Boreal (St. Catherines, Ontario) and sacrificed by decapitation. The dorsal skin was removed and homogenized in 50 ml of an acidic extraction medium consisting of 1 M hydrochloric acid containing 5% (v/v) formic acid, 1% (w/v) sodium chloride and 1% (v/v) trifluoroacetic acid (16). Following centrifugation, the supernatant was subjected to a reversed-phase extraction procedure using 10 Waters C18 Sep-Pak cartridges as described previously (16). The cartridge eluates consisting of 80% aqueous acetonitrile containing 0.1% (v/v) trifluoroacetic acid were combined and lyophilized. This material was homogenized in 5 ml of 0.1% trifluoroacetic acid. Following centrifugation the supernatant was loaded on the gel permeation HPLC columns using a trace enrichment procedure as described previously (18). The column was eluted isocratically using 40% aqueous acetonitrile containing 0.1% (v/v) trifluoroacetic acid (17). Biologically active fractions were pooled and subjected to two reversed-phase HPLC procedures using C18 µBondapak and Vydac columns each eluted with linear gradients of aqueous acetonitrile containing 0.1% (v/v) trifluoroacetic acid throughout.
Villus Enterocyte Isolation and Volume Determinations-- Villus cells were isolated from segments of adult male (200-300 g) guinea pig jejunum by mechanical vibration as described previously (8, 9). Isolated cells were resuspended at 0.8-1.5 × 106 cells/ml in RPMI 1640 medium (without HCO3) containing bovine serum albumin (Cohn fraction V) at 1 mg/ml and 20 mM sodium Hepes, pH 7.3 at 37 °C. Viability, assessed by trypan blue exclusion was 85%, 3 h after suspension in medium. Cell volume was measured using a Coulter Counter (ZM) with an attached Channelyzer (C-256) as described previously (8, 9). Villus cell volume measured electronically over a range of tonicities correlated positively (r = 0.967) with isotopic measurements of cell water (9). Relative cell volume was determined as the ratio of cell volume after agonist addition to the volume under basal conditions in isotonic medium immediately before challenge. Cell volume measurements were made using 30,000 cells/ml in Na+ medium, which contained (in mM): 140 NaCl, 3 KCl, 1 CaCl2, 1 MgCl2, 10 D-glucose, and 10 Hepes (pH 7.3, 295 mosM/kg H2O). Na+-free medium was prepared by iso-osmotically replacing NaCl with the chloride salt of N-methyl-D-glucamine. Nominally Ca2+-free Na+ medium contained 150 µM EGTA.
Uptake of 45Ca2+--
We measured the
initial rate of 45Ca influx into villus cells using a
modification of a procedure previously described for human lymphocytes
(19). We incubated the villus cells with 10 µM
acetoxymethylester of BAPTA (BAPTA-AM) for 30 min in RPMI medium, then
centrifuged the cells and resuspended them in BAPTA-AM-free medium.
Each villus cell preparation was divided in half and resuspended at a
final concentration of 5-6 mg of protein/ml in prewarmed uptake medium (Na+ medium supplemented) with bovine serum albumin at 1 mg/ml in a continuously stirred cuvette. For some experiments this
medium contained 0.1 µM niguldipine. Uptake was initiated
with the addition of 45Ca at a concentration of 10 µCi/ml, followed in some experiments by xenoxin-1 (10 nM). Immediately afterward, a 500-µl cell suspension was
removed and added to 500 µl of ice cold Ca2+-free (150 µM EGTA) uptake medium, which served as a "stop"
solution. This took less than 5 s and was taken to represent the
extracellular 45Ca associated with the cell pellet. Uptake
was terminated after 80 s by diluting 500 µl of cell suspension
in an equal volume of ice-cold stop solution, which was then gently
layered on a 100 µl layer of
di-n-butylpthalate:di-n-nonylphalate (3:2 by
volume) and centrifuged in an Eppendorf microcentrifuge for 20 s.
Aliquots of the supernatant were saved for counting and the cell pellet was processed as described previously (8). Prior to the addition of
45Ca, duplicate samples were taken and processed as above,
but following aspiration of the supernatant and oil, 100 µl of Triton
X-100 was added to the pellet. After vigorous shaking to induce cell lysis, protein content was determined using the Bio-Rad protein assay
reagent using bovine -globulin as a standard. Uptake experiments were first performed in the presence and absence of 0.1 µM niguldipine, then xenoxin-1 (10 nM) in the
presence and absence of niguldipine. In preliminary experiments, we
determined that 45Ca influx followed first order kinetics
in the BAPTA-loaded cells for 100 s. The extracellular
45Ca associated with the cell pellet was subtracted from
the 80-s values. Rates were expressed as picomoles /min/mg protein and are representative of five experiments performed in duplicate.
Amino Acid Analysis-- Purified peptide and cleavage fragments were hydrolyzed in the gas phase using a Waters Pico-Tag workstation as described previously (20) and subjected to amino acid analysis using a Beckman 6300 Series autoanalyzer.
Peptide Fragmentation-- Purified peptide was pyridylethylated according to a previously published method (20). The pyridylethyl cysteine derivative was purified by reversed-phase HPLC and subjected to both sequence analysis and endoprotease fragmentation. Arg-C endoprotease (Boehringer Mannheim) cleavage of the alkylated peptide was undertaken in 100 µl of 500 mM Tris (pH 8.5) at 37 °C for 5 h using a peptide to enzyme ratio of 20:1 (w/w). Arg-C protease fragments were purified by reversed-phase HPLC using a Waters C18 µBondapak column eluted with a linear gradient of 0-40% aqueous acetonitrile over 1 h containing 0.1% (v/v) trifluoroacetic acid throughout.
Gas-phase Sequencing-- Alkylated peptide and cleavage fragments were subjected to automated Edman degradation using a Porton Instruments gas-phase sequenator located at the Sheldon Biotechnology Center of McGill University.
Electrospray Ionization Mass Spectrometry-- Mass spectra of purified peptide were obtained as described previously using an API III triple-stage mass spectrometer with ion-spray interface (Sciex, Thornhill, Ontario, Canada) located at the Biotechnology Research Institute of the National Research Council of Canada in Montreal.
Statistics-- Data are reported as means ± S.E. of 4-10 experiments performed in duplicate. Differences in means were determined using Student's t test.
![]() |
RESULTS |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
Peptide Isolation and Characterization-- A portion equivalent to 5% of the unfractionated X. laevis skin extract was tested in the bioassay and was found to cause a volume reduction (15%) of the suspended villus epithelial cell preparation (Fig. 1). The remaining skin extract was subjected to gel permeation HPLC (Fig. 1). Material causing volume reduction was localized to fractions 16 and 17, which corresponded to a molecular weight of approximately 6000. Material within these fractions was purified further using reversed-phase HPLC as shown in Fig. 2A. Upon testing these fractions in the villus enterocyte bioassay, one region of bioactivity was found which corresponded exactly with a large peak of UV absorbance. This material was subjected to further reversed-phase HPLC procedures until homogeneity was achieved (Fig. 2B). Amino acid analysis revealed that the active compound was a peptide rich in cysteine with the following composition: Asx (4.7), Thr (7.2), Ser (2.7), Glx (6.6), Pro (0.9), Gly (3.8), Ala (3.7), 1/2 Cys (6.0), Val (1.2), Met (3.7), Ile (2.5), Leu (6.5), Tyr (0), Phe (0.9), His (0), Lys (7.5), and Arg (2.2).
|
|
Xenoxin-1 Stimulates Ca2+-dependent Volume Changes-- The effect of xenoxin-1 (10 nM) on isotonic volume of villus epithelial cells is illustrated in Fig. 3A. Addition of the peptide to cells suspended in isotonic medium containing Na+ (140 mM) caused a volume reduction. The final relative volume of cells to which xenoxin-1 was added was less than untreated controls (0.95 ± 0.01 versus 0.99 ± 0.01, p < 0.001, Fig. 3A). In nominally Ca2+-free medium (150 µM EGTA), the volume reduction brought about by xenoxin-1 was prevented. The final relative volume of the cells in Ca2+-free medium with xenoxin-1 was greater than cells treated with xenoxin-1 in Ca2+-containing medium (1.00 ± 0.01 versus 0.95 ± 0.01, p < 0.001). In Na+-free medium, xenoxin-1 also stimulated rapid volume reduction (Fig. 3B). Within 2 min of xenoxin-1 addition, the cells were smaller than untreated controls (relative volume 0.90 ± 0.01 versus 0.95 ± 0.01, p < 0.001). At the conclusion of the experiment, the xenoxin-1-treated cells were substantially smaller than untreated cells (final relative volume 0.82 ± 0.01 versus 0.89 ± 0.1, p < 0.001). This volume reduction was also prevented in Ca2+-free medium. The final relative volume of cells treated in Ca2+-free medium with xenoxin-1 was greater than in Ca2+-containing medium (0.90 ± 0.01 versus 0.82 ± 0.01, p < 0.001). We assessed the effect of dihydropropyridine-sensitive Ca2+ channel blocker on the volume changes stimulated by xenoxin-1 in either Na+-containing or Na+-free medium (Fig. 3C). Niguldipine (0.1 µM), a potent inhibitor of dihydropyridine-sensitive Ca2+ channels (21, 22), prevented the xenoxin-1-stimulated volume reduction in Na+-containing medium (final relative volume: 1.00 ± 0.01, p < 0.001). In Na+-containing medium, niguldipine alone had no effect on cell volume over the course of the experiment. In Na+-free medium, niguldipine also blocked the xenoxin-1-stimulated volume reduction (final relative volume: 0.92 ± 0.01 versus 0.82 ± 0.01, p < 0.001). The data suggest that xenoxin-1 activates a dihydropyridine-sensitive Ca2+ channel, and subsequently with the Ca2+ influx from the extracellular Ca2+ compartment, osmolyte loss is activated leading to isotonic volume reduction of these epithelial cells.
|
Bay K-8644 and Xenoxin-1 Stimulate Ca2+-dependent Volume Changes-- To determine whether directly activating dihydropyridine-sensitive Ca2+ channels would generate volume changes, we used a well characterized (23) and selective agonist of these channels; 1-4-dihydro-2,6-dimethyl-5-nitro-4-(2-(trifluoromethyl)phenyl)-3-pyridine carboxylic acid methylester (BayK-8644). BayK-8644 (100 nM), added to villus cells suspended in isotonic Na+-containing medium, caused a volume reduction (Fig. 4). The final relative volume of these cells was less than untreated controls (0.93 ± 0.01 versus 1.00 ± 0.01, p < 0.001, n = 6). The BayK-8644 effect was dose-dependent with an EC50 of 40 nM (data not shown). In Ca2+-free medium (150 µM EGTA), the BayK-8644 volume reduction was prevented. The final relative volume of these cells was greater than in the presence of extracellular Ca2+ (0.99 ± 0.001 versus 0.93 ± 0.01, p < 0.001, n = 6).
|
|
Xenoxin-1 Stimulates Dihydropyridine-sensitive 45Ca2+ Influx-- To determine whether xenoxin-1-stimulated 45Ca influx that was sensitive to a dihydropyridine, we directly measured the initial rate of 45Ca influx after addition of xenoxin-1 in the absence or presence of niguldipine (Fig. 6). Niguldipine (0.1 µM) inhibited the initial rate of 45Ca2+ influx in control cells (40 ± 9 versus 155 ± 38 pmol of 45Ca2+/min/mg of protein, p < 0.05, n = 5). Xenoxin-1 (10 nM) substantially increased the rate of influx in comparison with control cells (848 ± 117 pmol of 45Ca2+/min/mg protein, p < 0.05, n = 5). Niguldipine (0.1 µM) abolished the increase in rate stimulated by xenoxin-1 (73 ± 24 pmol of /min/mg of protein, p < 0.01, n = 5). Thus, xenoxin-1 stimulated a 6-fold increase in dihydropyridine-sensitive 45Ca2+ influx into villus cells.
|
Staurosporine Blocks ATP but Not Xenoxin-1-stimulated Volume
Reduction--
In remaining experiments, we assessed whether protein
kinase C (PKC) was required for the xenoxin-1-stimulated volume
reduction. We first assumed that ATP would interact with a purinergic
receptor coupled to phospholipase C hydrolysis, which would release
diacylglycerol and mobilize PKC, which would in turn activate
Cl conductance causing volume reduction. Addition of ATP
(250 µM) to villus cells in Na+ medium caused
a volume reduction that peaked at 10 min and remained stable for an
additional 20 min. The final relative volume of cells treated with ATP
was less than untreated controls (0.92 ± 0.01, p < 0.001, n = 6). The PKC inhibitor staurosporine (10 nM) prevented the ATP-stimulated volume reduction (final
relative volume: 0.99 ± 0.01, p < 0.001, n = 6). Staurosporine (10 nM) had no effect
on volume reduction caused by xenoxin-1 (10 nM, 0.95 ± 0.01, n = 6) or BayK-8644 (100 nM,
0.93 ± 0.01, n = 6).
![]() |
DISCUSSION |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
In this report, we have shown that xenoxin-1, a peptide belonging to the neurotoxin/cytotoxin family of peptides (1, 15), isolated from the skin of X. laevis, stimulates dihydropyridine-sensitive 45Ca influx and dihydropyridine-sensitive volume changes in Na+-absorbing epithelial cells isolated from guinea pig jejunum. We conclude that a biological activity of xenoxin-1 is its ability to activate dihydropyridine-sensitive Ca2+ channels in mammalian epithelium.
Xenoxin-1 was purified in this study because of its ability to
stimulate isotonic volume changes in jejunal villus epithelial cells. A
well characterized dihydropyridine-sensitive Ca2+ channel
agonist, BayK-8644, caused comparable volume changes when added to
these cells. In general, isotonic epithelial cell volume is maintained
because the rate of salt influx is equivalent to the rate of efflux (8,
9, 14). Accordingly, volume reduction occurs because salt efflux is
greater than salt influx. Previously, we have shown that both the
calcium ionophore A23187 and certain members of the defensin peptide
family cause an isotonic volume reduction, which was blocked by either
a Cl channel or K+ channel blocker (10). This
was consistent with osmolyte loss as being responsible for the volume
reduction. However, the volume reductions stimulated by either the
ionophore or defensin peptide were prevented in the absence of
extracellular calcium, suggesting that Ca2+ influx was
proximal to the activation of the K+ and C1
channels. In the current experiments, the volume reduction stimulated by xenoxin-1 or BayK-8644 were prevented in the absence of
extracellular calcium. In other systems, BayK-8644 has been shown to
increase Ca2+ influx by increasing the mean open time of
dihydropyridine-sensitive Ca2+ channels (23). The volume
reduction of villus cells caused by BayK-8644 suggests that activating
dihydropyridine-sensitive Ca2+ channels in these cells
results in the activation of K+ and Cl
channels, which cause the volume reduction. Consequently, the loss of
volume reduction brought about by BayK-8644 in the absence of
extracellular calcium is consistent with calcium influx being required
for volume changes initiated by BayK-8644. Because all the volume
changes stimulated by xenoxin-1 also required calcium, we conclude that
calcium influx was the stimulus for the volume altering effects of
xenoxin-1.
Xenoxin-1 stimulated dihydropyridine-sensitive 45Ca influx into the villus cells. Our earlier studies have shown that both dihydropyridines and benzothiazapines will prevent volume regulation following hypotonic dilution of the cells (24). Binding studies of basolateral membrane vesicles derived from rabbit villus epithelial cells have characterized both phenylalkylamine- and dihydropyridine-sensitive Ca2+ channels in these cells (25). Furthermore, addition of the dihydropyridine agonist BayK-8644 in the current studies caused both isotonic volume reduction, and when cells were permeabilized to sodium by gramicidin, a Ca2+-dependent volume increase. The latter volume change has been characterized as rate-limited by anion permeability (9, 12). Because xenoxin-1 caused Ca2+-dependent volume changes that were comparable in both magnitude and direction as those caused by the specific agonist BayK-8644, and no greater effects were observed when both agonists were added together, our data strongly suggest that xenoxin-1 stimulates dihydropyridine-sensitive Ca2+ channels in these epithelial cells.
We considered three models to explain the volume reduction caused by
xenoxin-1. They are as follows: xenoxin-1 causing direct activation of
Cl channels, xenoxin-1 activating a receptor that is
coupled to phospholipase C hydrolysis, and xenoxin-1 directly
activating dihydropyridine-sensitive Ca2+ channels. In the
first model, Cl
channel activation would depolarize the
cell thus activating voltage-sensitive K+ channels so that
the net effect is K+ and Cl
efflux resulting
in volume reduction. However, mobilization of extracellular
Ca2+ would not be required to activate this osmolyte
efflux. In the second model, xenoxin-1, activating a receptor coupled
to phospholipase C hydrolysis, would liberate intracellular
Ca2+ and generate diacylglycerol, which would in turn
activate protein kinase C. In villus cells, as we have previously
determined (12), PKC activation of Cl
conductance may be
inhibited by staurosporine. Again, the net effect would be
K+ and Cl
efflux, which would lead to a
volume reduction. In the current experiments, activation of a
purinergic receptor by ATP-stimulated volume reduction, which was
prevented by the PKC inhibitor staurosporine, suggesting that this
pathway was operative in the volume reduction. Neither the xenoxin-1-
nor the BayK-8644-stimulated volume reduction were influenced by the
PKC inhibitor, suggesting that PKC activation was not required for
these volume changes. Because xenoxin-1 and BayK-8644 both stimulated
volume changes that required extracellular Ca2+ and
xenoxin-1 substantially increased dihydropyridine-sensitive 45Ca2+ influx, we conclude that our data are
most compatible with the third model, that xenoxin-1 directly activates
dihyropyridine-sensitive Ca2+ channels in villus cells.
The xenoxin-1-stimulated volume reduction and increased rate of
45Ca2+ influx were sensitive to a
dihydropyridine antagonist, niguldipine. This antagonist, originally
shown to block "L" type Ca2+ channels (21) has also
been shown to inhibit T-type Ca2+ currents (26), inhibit
drug transport by P-glycoprotein (27, 28) as well as inhibit adenosine
(29) and 1-adrenergic (30) receptors. Previously we have shown that
under isotonic conditions in both villus (8, 9) and crypt (14)
epithelial cells that if either the constitutively active
K+ or Cl
channels of these cells were
inhibited by the appropriate blockers, the cells began to swell because
of continued influx of Na+ and Cl
.
Niguldipine had no effect on the isotonic volume of the cells suggesting that neither the K+ nor Cl
conductances were inhibited. Niguldipine did block the increased rate
of 45Ca2+ influx stimulated by xenoxin-1,
consistent with the capacity of such compounds to increase closure
intervals of dihydropyridine-sensitive Ca2+ channels (31).
Therefore, we conclude that xenoxin-1 activated dihydropyridine-sensitive Ca2+ channels in villus
epithelial cells.
Xenoxin-1 has been shown to be negative for -neurotoxin activity, as
well as anti-protease and anti-bacterial activity (15). Frog skin is an
epithelium, and it was speculated earlier that peptides isolated from
frog skin might regulate water and electrolyte homeostasis (7). Our
results suggesting that xenoxin-1 activates dihydropyridine-sensitive
Ca2+ channels in intestinal epithelial cells allow us to
speculate on a physiological role for a mammalian homologue of
xenoxin-1 in the gut. In the mammalian small intestine, transepithelial Na+ and Cl
flux in the mucosal to serosal
direction is exquisitely sensitive to intracellular calcium
concentrations. Lowering [Ca2+]i will increase
this sodium flux while elevating it inhibits the flux (32). These
effects are thought to be mediated through protein kinase C or
Ca2+/calmodulin kinase II (32, 33). Most peptides
identified from X. laevis skin or skin secretions are
homologous to vertebrate hormones and neurotransmitters, providing
evidence for the evolutionary relationship of the amphibian
skin/gut/brain axis. Indeed, it is now appreciated that the
neurotoxin/cytotoxin peptides are members of a protein superfamily that
includes the glycosyl phosphotidylinositol-anchored membrane proteins
CD59, the Ly-6 family, and the urokinase receptor (34). We speculate
that a mammalian homologue of xenoxin-1, if present in the gut, would
participate in electrolyte homeostasis by dihydropyridine-sensitive
Ca2+ channel activation. Transient increases in villus
epithelial cell [Ca2+]i would inhibit sodium and
chloride influx in these cells.
In conclusion, using a sensitive bio-assay of calcium-mediated volume changes in intestinal epithelial cells, we have purified to homogeneity xenoxin-1 from the skin of X. laevis. This peptide, which is a member of the cytotoxin/neurotoxin family of peptides, activates dihydropyridine-sensitive Ca2+ channels in mammalian gut epithelial cells.
![]() |
ACKNOWLEDGEMENTS |
---|
We thank Bernard Gibbs for undertaking mass spectrometry and Sheryl Mann and Dawn Williams for preparing the manuscript. The continuing interest, advice, and support of Dr. S. Solomon and Dr. R. Hamilton is gratefully acknowledged.
![]() |
FOOTNOTES |
---|
* This work was supported by Medical Research Council of Canada Grants MT-6733 and MT-6708.The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.
§ Present address: Endocrine-Hypertension Div., Brigham and Women's Hospital, Dept. of Medicine, Harvard Medical School, Boston, MA 02115.
To whom correspondence should be addressed: Endocrine
Laboratory, L2.05, Royal Victoria Hospital, 687 Pine Ave. West,
Montreal, Quebec H3A 1A1, Canada. Tel.: 514-842-1231 (ext. 6731); Fax:
514-843-1709; E-mail: bennett{at}pathology.lan.mcgill.ca.
The abbreviations used are: BAPTA, 1,2-bis-(2-aminophenoxy)ethane-N,N,N1,N1-tetraacetic acid HPLC, high performance liquid chromatographyPKC, protein kinase C.
![]() |
REFERENCES |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|