JBC Oz Biosciences

HOME HELP FEEDBACK SUBSCRIPTIONS ARCHIVE SEARCH TABLE OF CONTENTS
QUICK SEARCH:   [advanced]


     

Originally published In Press as doi:10.1074/jbc.M504256200 on July 8, 2005

J. Biol. Chem., Vol. 280, Issue 35, 30705-30711, September 2, 2005
This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow All Versions of this Article:
280/35/30705    most recent
M504256200v1
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Right arrow Citation Map
Services
Right arrow Email this article to a friend
Right arrow Similar articles in this journal
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Right arrow reprints & permissions
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Vial, C.
Right arrow Articles by Evans, R. J.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Vial, C.
Right arrow Articles by Evans, R. J.
Social Bookmarking
Add to CiteULike   Add to Complore   Add to Connotea   Add to Del.icio.us   Add to Digg   Add to Reddit   Add to Technorati  
What's this?

Disruption of Lipid Rafts Inhibits P2X1 Receptor-mediated Currents and Arterial Vasoconstriction*

Catherine Vial and Richard J. Evans{ddagger}

From the Department of Cell Physiology & Pharmacology, University of Leicester, Leicester, LE1 9HN United Kingdom

Received for publication, April 19, 2005 , and in revised form, June 21, 2005.


   ABSTRACT
TOP
 ABSTRACT
INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
P2X1 receptors for ATP are ligand-gated cation channels expressed on a range of smooth muscle preparations and blood platelets. The receptors appear to be clustered close to sympathetic nerve varicosities and mediate the underlying membrane potential changes and constriction following nerve stimulation in a range of arteries and resistance arterioles. In this study we have used discontinuous sucrose density gradients, Western blot analysis, and cholesterol measurements to show that recombinant and smooth muscle (rat tail artery, vas deferens, and bladder) P2X1 receptors are present in cholesterol-rich lipid rafts and co-localize with the lipid raft markers flotillin-1 and -2. Lipid rafts are specialized lipid membrane microdomains involved in signaling and trafficking. To determine whether lipid raft association was essential for P2X1 receptor channel function we used the cholesterol-depleting agent methyl-{beta}-cyclodextrin (10 mM for 1 h). This led to a redistribution of the P2X1 receptor throughout the sucrose gradient and reduced P2X1 receptor-mediated ({alpha},{beta}-methylene ATP, 10 µM) currents in HEK293 cells by >90% and contractions of the rat tail artery by ~50%. However contractions evoked by potassium chloride (60 mM) were unaffected by methyl-{beta}-cyclodextrin and the inactive analogue {alpha}-cyclodextrin had no effect on P2X1 receptor-mediated currents or contractions. P2X1 receptors are subject to ongoing regulation by receptors and kinases, and the present results suggest that lipid rafts are an essential component in the maintenance of these localized signaling domains and play an important role in P2X1 receptor-mediated control of arteries.


   INTRODUCTION
TOP
 ABSTRACT
 INTRODUCTION
MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
ATP released from nerves following tissue damage or shear stress acts at P2 receptors to regulate cardiovascular function (1). P2 receptors are divided into ligand-gated P2X receptor channels and G-protein-coupled P2Y receptors. P2X receptor-mediated vasoconstriction has been described in a range of arteries in the periphery (1) and in the brain (2). Sympathetic nerves co-store and co-release ATP and noradrenaline, and the relative contribution of purinergic and noradrenergic mechanisms to vasoconstriction is dependent on the size of the vessel and the parameters of stimulation (3, 4). The P2X receptor-mediated component predominates in small diameter arteries (4, 5) and in submucosal resistance arterioles P2X receptor activation is solely responsible for sympathetic neurogenic vasoconstriction with noradrenaline acting through presynaptic mechanisms to regulate transmitter release (6). In addition P2X receptor channels in smooth muscle are permeant to calcium (~10% of current flowing through the channel under physiological conditions, Refs. 7 and 8), and a substantial component of the calcium required for contraction enters by this route (4, 9). P2X receptors therefore provide a mechanism for sympathetic nerve-mediated regulation of vascular tone that is resistant to {alpha}-adrenoreceptor and calcium channel antagonists.

Seven P2X receptor subunits have been identified (P2X1–7), and these can assemble as homo- and heterotrimeric receptors with a range of properties (10). The characteristic features of artery smooth muscle P2X receptors; (i) sensitivity to the ATP analogues: {alpha},{beta}-methylene and L-{beta},{gamma}-methylene ATP, and (ii) responses that desensitize during agonist application, are consistent with the expression of P2X1 receptor subunits. In arterial smooth muscle the P2X1 receptor is the dominant isoform, and P2X receptor-mediated responses are abolished in arteries from P2X1 receptor-deficient mice (11, 12). Studies with these P2X1 receptor-deficient mice have established a role for these receptors in sympathetic nerve-mediated vasoconstriction (11) and autoregulation of blood flow in the kidney (12, 13). The level of P2X1 receptors can be regulated by congestive heart failure (14), cardiomyopathy (15), and shear stress (16). In addition it has been shown recently that P2X receptors are involved in sensitizing responses following heart failure (17). P2X1 receptors are also expressed on blood cells, including platelets and P2X1 receptors contribute to platelet activation (18) and aggregation (19–21) and P2X1 receptor deficiency is protective against thromboembolism (22). Thus evidence is building that P2X1 receptors can play important roles in the cardiovascular system and regulation of blood flow.

In arteries P2X1 receptors do not appear to be randomly distributed throughout the plasma membrane as P2X1 receptor immunoreactivity appears in clusters (23). This clustering of receptors is supported by electrophysiological studies on dissociated artery muscle-excised membrane patches; some patches had multiple P2X receptor channels whereas channel activity was absent in others (24). Recent studies also indicate that the P2X1 receptors can be regulated by phosphorylation of interacting proteins (25), suggesting that the P2X1 receptor exists in an organized signaling domain. One possible explanation for the clustering of P2X1 receptors could be the inclusion in membrane lipid rafts (26). Lipid rafts are rich in cholesterol and glycosphingolipids that results in liquid-ordered microdomains within the liquid-disordered glycerophospholipid membrane bilayer (27, 28). Recent evidence suggests that there is heterogeneity in lipid rafts and that a range of different domains can be separated based on differences in detergent solubility (for a review see Ref. 27). A wide range of proteins, including many signaling molecules have been shown to be preferentially associated with rafts (29) including a range of ion channels (for a review see Ref. 30). In this study we have shown that P2X1 receptors are concentrated in lipid rafts and that disruption of rafts reduces P2X1 receptor signaling in arteries.


   MATERIALS AND METHODS
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
RESULTS
 DISCUSSION
 REFERENCES
 
Reagents—{alpha},{beta}-meATP,1 cholesterol, filipin III, KCl, {alpha}-cyclodextrin ({alpha}-CD), {beta}-cyclodextrin ({beta}-CD), and methyl-{beta}-cyclodextrin (M{beta}-CD) were obtained from Sigma (Sigma-Aldrich).

Cell Culture and Transient Transfection—Native human embryonic kidney 293 (HEK293) cells and HEK293 cells subcloned after transfection with the human wild-type P2X1 receptor (P2X1cl-1 cells), were maintained in culture as previously described (25). For some studies native HEK293 cells were transiently transfected with plasmid cDNA encoding either the rat wild-type P2X1 receptor or human wild-type P2X1 receptor tagged with EGFP at its C terminus (P2X1-EGFP cells) using LipofectamineTM 2000 reagent (Invitrogen). Control and {beta}-CD-treated cells (10 mM for 1 h at 37 °C) were imaged live using a x60 oil immersion lens mounted on a Fluoview FV300 confocal microscope (excitation wavelength of 488 nm for EGFP and filters set to capture emission at wavelengths greater than 510 nm) (Olympus, Tokyo, Japan). Fluorescence was captured using Olympus Fluoviewer 4.2 software.

Rat Tissue Collection—Male Wistar rats (250–350 g) were killed by stunning and cervical dislocation. For membrane fractionation, tail artery, vas deferens, and bladder were excised and processed immediately or frozen in liquid nitrogen for later use. For contraction experiments, tail arteries were kept at 4 °C in physiological saline solution (150 mM NaCl, 2.5 mM KCl, 10 mM HEPES, 2.5 mM CaCl2,1mM MgCl2, pH to 7.3 with NaOH) for a maximum of 3 h before use.

Membrane Fractionation—Cells and rat tissues were fractionated using a detergent-free method adapted from Refs. 31 and 32. Two 80-cm2 tissue flasks of HEK293 P2X1cl-1 cells were washed three times with phosphate-buffered saline and scraped into 2 ml of 500 mM sodium carbonate, pH 11 and left on ice for 20 min. Either seven tail arteries, 3 vas deferens, or 3 bladders from rat were crushed in liquid nitrogen using a pestle and a mortar. When reduced to powder, the tissues were then homogenized into 2 ml of 500 mM Na2CO3, pH 11 using a tissue grinder and left on ice for 20 min. The lysed cells and rat tissues were then subjected to three 20-s bursts of sonication. Homogenates were brought to 45% sucrose by addition of an equal volume of 90% sucrose in MBS (25 mM MES and 150 mM NaCl, pH 6.5) and loaded in an ultracentrifuge tube. A discontinuous sucrose gradient was layered on top of the sample by placing 4 ml of 35% sucrose prepared in MBS with 250 mM Na2CO3 then 4 ml of 5% sucrose (also in MBS/Na2CO3). The gradient was centrifuged at 39,000 rpm on a TH-641 rotor in a Sorvall OTD65B ultracentrifuge (Kendro Laboratory Products Plc, Bishop's Stortford, UK) for 16 h at 4 °C. In some studies HEK293 P2X1c1-1cells were lysed in 2 ml of MBS containing either 0.1% Triton X-100 or 1% Triton X-100 and were homogenized using a tissue grinder and left for 20 min on ice. The homogenates were brought to 45% sucrose by addition of an equal volume of 90% sucrose in MBS and loaded in an ultracentrifuge tube. A discontinuous sucrose gradient (35 and 5% sucrose in MBS, lacking Triton X-100) was formed above the homogenate and centrifuged as described above for the detergent-free condition. After centrifugation, 11 fractions of 1 ml were collected from the top to the bottom of each tube. Cholesterol measurements were assessed with the Amplex Red cholesterol assay kit (Molecular Probes Europe BV, Leiden, The Netherlands). The cell volume or tissue quantities used for the sample preparations described above where each representative of one individual experiment. Each experimental condition was repeated three times.

Western Blots—The protein level of fraction 4 was used as a loading reference. To do so, the same volumes of samples (different fractions) were loaded for each gel after normalization for protein quantity in fraction 4 (0.04 µg for tail artery, vas deferens, or bladder and 0.1 µg for HEK293 P2X1cl-1 cells). After separation of the samples on 10–12% SDS-PAGE gels and transfer onto nitrocellulose, the membrane was processed with the primary antibody (anti-P2X1 receptor antibody (1:2000) (Alomone, Jerusalem, Israel) or anti-caveolin-1 (1:1000), anti-caveolin-2 (1:250), anti-flotillin-1 (1:250), anti-flotillin-2 (1:5000) (BD Biosciences Europe, Erembodegem, Belgium). Protein bands were visualized using an ECL+plus kit and Hyperfilm MP (Amersham Biosciences).

Surface Cell Expression and Immunoprecipitations—Cell surface proteins were biotinylated as previously described (33) and washed with phosphate-buffered saline. Cells from two 80-cm2 tissue flasks were processed for membrane fractionation as described above and blotted with Immunopure streptavidin/horseradish peroxidase-conjugated (0.5 µg/ml) (Pierce). Cells contained in a 35-mm Petri dish were processed for immunoprecipitation (33). The samples were resuspended in 15 µl of gel sample buffer before running on SDS-PAGE gels. In parallel an aliquot of total lysate (0.5 µg of total protein) was blotted with anti-p44/42 MAP kinase antibody (1:1000) (PerkinElmer Life Sciences). Each experimental condition was repeated three times.

Patch Clamp Recordings—Conventional whole cell and amphotericin-permeabilized patch-clamp experiments were performed at a holding potential of –60 mV at room temperature (21 °C) as described previously (11, 34). The agonist ({alpha},{beta}-meATP, 10 µM) was rapidly applied via a U-tube. When looking at the effect of cyclodextrins on the P2X1 receptor responses to {alpha},{beta}-meATP, the cells were incubated with the drugs at a concentration of 10 mM for 1 h at 37 °C, for cholesterol repletion cells were subsequently incubated for 1 h at 37 °C with 660 µg/ml cholesterol M{beta}-CD. Filipin (10 µM) was incubated with the cells for 30 min at 37 °C.

Contraction Studies—Rat tail artery rings were mounted in a Mulvany myograph and perfused with physiological saline solution at 34 °C and vasoconstrictions to applied drugs measured as described previously (35). Reproducible responses to 10 µM {alpha},{beta}-meATP could be recorded when the agonist was added at 30-min intervals. The superfusate was stopped when the arteries were incubated in the presence of cyclodextrin drugs (10 mM for 1 h at 34 °C). In the control condition, the superfusate was also stopped for 1 h. Before testing subsequent contraction responses to {alpha},{beta}-meATP and KCl (60 mM), the superfusion was reinitiated, and the arteries were washed with physiological saline solution.

Data Analysis—Data are expressed as mean ± S.E. throughout and n = number of cells, number of arteries. Differences between means were determined by Student's t test and a p value of < 0.05 was considered statistically significant.


   RESULTS
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
DISCUSSION
 REFERENCES
 
P2X1 Receptors Are Associated with Lipid Rafts—Membrane proteins can show a variable distribution relating to the lipid composition of the membrane, with a number of proteins being preferentially located in cholesterol-rich lipid rafts. Stable expression of P2X1 receptors in HEK293 cells provides an ideal model system to investigate the role of lipid rafts in receptor function. Cell lysates were extracted under detergent-free conditions and ultracentrifuged on a discontinuous sucrose gradient (31). P2X1 receptor protein was predominantly found colocalized with the lipid raft markers flotillin-1 and flotillin-2 in fractions 3 and 4 (36) (Fig. 1a) and was absent from nontransfected cells (Fig. 1d). Fractions 3 and 4 contain more than 75% of the total cellular cholesterol (and only ~10% of the total protein, Fig. 1b) confirming the presence of the P2X1 receptor protein in the cellular enriched-cholesterol fractions. As the P2X1 receptor is a transmembrane protein one possibility was that the fractionation concentrates the plasma membrane in fractions 3 and 4, and this could account for the predominant localization of the P2X1 receptors in these fractions and not lipid raft association. To test this we used membrane-impermeant sulfo-NHS-LC-biotin to label surface proteins and determine their distribution on the gradient. Biotinylated proteins were distributed throughout the gradient, demonstrating that the fractionation does not just concentrate membrane proteins. Moreover, the biotinylation process was specific for surface proteins as no trace of the cytosolic p44/42 MAP kinases was observed at the cell surface although present in the total lysate (Fig. 1e). Taken together these data demonstrate that P2X1 receptors are localized to enriched cholesterol lipid rafts.

P2X1 Receptors Remain in the Lipid Raft Fraction following Activation and Desensitization—Activation of some receptors, for example the {beta}2-adrenoreceptor leads to movement out of the lipid rafts and a reduction in signaling (37, 38). P2X1 receptors desensitize rapidly following agonist stimulation, and require several minutes for recovery, raising the possibility that the recovery process is dependent on movement between lipid rafts and the rest of bulk membrane. Activation of the P2X1 receptor with {alpha},{beta}-meATP (10 µM) for 10 min should fully desensitize the receptor; however it had no effect on the distribution of the receptor in the lipid raft fractions (Fig. 1f) indicating that movement out of the lipid rafts is not associated with desensitization of the P2X1 receptor channel.



View larger version (30K):
[in this window]
[in a new window]
  		FIG. 1.
Presence of the P2X1 receptor in the lipid raft-enriched fractions prepared from HEK293 cells. a, HEK293 cells stably expressing P2X1 receptor were lysed and separated on a density gradient (45, 35, and 5% sucrose). Eleven fractions (from top to bottom of gradient) were immunoblotted for P2X1 receptor, flotillin-1 and flotillin-2. b, fractions collected in a were also assayed for cholesterol and total protein. c, HEK293 cells stably expressing P2X1 receptor were treated with EZ-LinkTMSulfo-NHS-LC-Biotin and then processed as described in a. The fractions were then immunoblotted for streptavidin revealing the cell surface-expressed proteins. d, P2X1 receptor is not expressed in native HEK293 cells (Native lane) but is present in HEK293 cells stably expressing P2X1 receptor (P2X1 lane) as shown when immunoblotted for P2X1 receptor. Cells were lysed with 0.5% Triton X-100-containing buffer, and the total cell lysate was separated by SDS-PAGE. e, HEK293 cells stably expressing P2X1 receptor were treated with EZ-LinkTMSulfo-NHS-LC-Biotin, lysed with 0.5% Triton X-100-containing buffer and immunoprecipitated with streptavidin-agarose. After separation by SDS-PAGE, the sample was immunoblotted for p44/42 MAP kinase (Surface lane) and compared with an aliquot taken before immunoprecipitation (Total lane). Both p44/42 MAP kinases (which are known cytosolic proteins) are absent from the "surface" sample indicating that (i) the process of biotinylation is membrane protein-specific and that (ii) the surface-expressed protein fraction is not contaminated with cytosolic proteins. f, HEK293 cells stably expressing P2X1 receptor were treated or not with {alpha},{beta}-meATP (10 µM for 10 min), processed as described in a and immunoblotted for P2X1 receptor. All the gels shown in Fig. 1 are representative of three separate experiments as well as the cholesterol and protein assays.

 



View larger version (25K):
[in this window]
[in a new window]
  		FIG. 2.
Cholesterol depletion moves the P2X1 receptor out from the lipid raft fraction and inhibited agonist-evoked currents but had no effect on the surface localization of the receptor expressed in HEK293 cells. a, cholesterol depletion with M{beta}-CD (10 mM for 1 h) redistributed the P2X1 receptor from fractions 3 and 4 to a diffuse distribution throughout the sucrose gradient. A representative gel is shown of three separate experiments. b, representative traces of P2X1 receptor currents evoked in response to 10 µM {alpha},{beta}-meATP (application indicated by bar). The cholesterol-depleting agents M{beta}-CD and {beta}-CD (both 10 mM for 1 h) reduced the amplitude of the current with no obvious effect on the time course of responses. The inactive analogue {alpha}-CD (10 mM for 1 h) had no effect on P2X1 receptor currents. c, summary of the effects of cyclodextrins on P2X1 receptor current amplitude (n = 6–9). d, EGFP-tagged P2X1 receptors are localized to the surface membrane and are unaffected by M{beta}-CD treatment (10 mM for 1 h).

 
Lipid Raft Disruption Regulates P2X1 Receptor Properties— Depletion of cellular cholesterol leads to dissociation of lipid rafts. The cholesterol-depleting agent M{beta}-CD (10 mM for 1 h) reduced by 51 ± 28% the total cellular cholesterol content and induced a redistribution of the P2X1 receptor along the gradient (Fig. 2a). Following cholesterol depletion, the P2X1 receptor was now detected readily in fractions 5–11. M{beta}-CD is membrane impermeable and does not deplete cholesterol from intracellular membranes, this may in part account for the P2X1 receptor detected in fractions 3 and 4 that could correspond to receptors on intracellular membranes being trafficked.

In patch-clamp studies, the ATP analogue {alpha},{beta}-meATP (10 µM a maximal concentration) evokes transient inward currents through P2X1 receptors from HEK293 P2X1cl-1 cells (Fig. 2b). Depletion of cellular cholesterol with either M{beta}-CD or {beta}-CD (10 mM for 1 h) reduced the amplitude of agonist-evoked responses by >90% with no effect on either the rise time or rate of decay of the response (Fig. 2b). The reduced amplitude of response is unlikely to result from a decrease in agonist potency at the receptor, as suggested for the effects of cholesterol depletion on cyclic nucleotide-gated channels (39), as there was no effect on the time course of the response and a supramaximal concentration of ATP (1 mM, 1,000-fold greater than the EC50 concentration) was also reduced by >90% (data not shown). M{beta}-CD or {beta}-CD treatment also has no effect on the recovery of P2X1 receptors from the desensitized state as reproducible responses to {alpha},{beta}-meATP were evoked at 5-min intervals using the amphotericin-permeabilized patch technique (as shown previously, Ref. 34) from control cells and following M{beta}-CD or {beta}-CD treatment (data not shown). The inactive cyclodextrin stereoisomer {alpha}-CD (10 mM for 1 h) (40) had no effect on agonist-evoked responses (Fig. 2b). Following M{beta}-CD treatment responses to {alpha},{beta}-meATP (10 µM) were partially restored (~4-fold increase in amplitude compared with M{beta}-CD, p < 0.05) by cholesterol repletion (660 µg/ml for l h)(–3222 ± 549, –212 ± 130, and –818 ± 240 pA for control, M{beta}-CD and cholesterol repletion, respectively, n = >8). The reduction in current amplitude in response to M{beta}-CD is unlikely to result from a decrease in the number of P2X1 receptor channels at the cell surface as the localization of EGFP-tagged P2X1 receptors at the cell membrane (peak currents through these receptors are also reduced by ~85% by M{beta}-CD treatment; –5224 ± 1063 and –887 ± 200 pA for control and M{beta}-CD respectively, n>6) was unaffected by {beta}-CD treatment (observation of 17 and 14 cells, respectively, for control and {beta}-CD treatment) (Fig. 2d).



View larger version (17K):
[in this window]
[in a new window]
  		FIG. 3.
P2X1 receptor and flotillin-2 association with lipid rafts in HEK293 cells is sensitive to the concentration of Triton X-100 detergent. HEK293 cells stably expressing P2X1 receptors were lysed either in detergent-free condition (500 mM Na CO, pH 11) or in presence of 0.1 or 1% Triton X-100. Under detergent-free conditions, P2X1 receptors (left panels) and flotillin-2 (right panels) were detected in the buoyant membrane fractions. A different pattern of P2X1 and flotillin-2 protein distribution in the gradient was recorded following isolation with Triton X-100, and this was concentration-dependent; 0.1% Triton X-100 redistributed partially the P2X1 receptor along the sucrose gradient, whereas the P2X1 receptor was predominantly in the 45% sucrose bottom fractions following 1% Triton X-100 treatment. The inset shows that the P2X1 receptor was detected in the buoyant fractions on longer exposure of the blot. A similar distribution along the sucrose gradient was also observed for the lipid raft marker flotillin-2.

 
Lipid rafts may also be disrupted by filipin, which acts to form multimeric globular complexes with membrane cholesterol (41, 42). Filipin (10 µM for 30 min) reduced by >90% peak currents following P2X1 receptor activation with no effect on the time course of the response (–5809 ± 790 and 119 ± 70 pA for control and filipin treatment, respectively, n + 12.5). Taken together our results show that lipid raft disruption in HEK293 cells significantly depressed P2X1 channel function.

With What Type of Lipid Rafts Are P2X1 Receptors Associated?— Lipid rafts are thought to be heterogeneous with a range of different types of domain dependent on the protein and lipid content of the rafts (27). The only subtype of rafts that can be identified morphologically are caveolae. These are small plasma membrane invaginations associated with the expression of the caveolins (27). In this study caveolin-1 and -2 were below the limit of detection in HEK293 cell lines (data not shown; however caveolins were detected in arterial smooth muscle cells, see below) suggesting that P2X1 receptors are not associated with caveolae in lipid rafts.

The composition of lipid rafts appears to be dependent on the method of isolation and different types of lipid raft domain have been postulated based on differences in detergent solubility of individual raft proteins. Lipid rafts prepared by non-detergent methods are enriched in glycerophospholipids whereas, in contrast, detergent extraction with Triton X-100 leads to a depletion of these glycerophospholipids and in addition non-detergent methods lead to a greater retention of inner leaflet membrane lipids (for review, see Ref. 27). Thus comparing results from different isolation procedures may give an insight into which subpopulation of lipid rafts the P2X1 receptor associates with. We therefore compared rafts isolated by non-detergent methods with extraction with 0.1 and 1% Triton X-100 (Fig. 3). At 0.1% Triton X-100 P2X1 receptors were associated with the buoyant fraction, however in addition the P2X1 receptor was also significantly detected in bottom fractions. When 1% Triton X-100 was used the P2X1 receptor was detectable at low levels in the buoyant fractions and predominantly in the bottom fractions, this is consistent with a previous report on Triton X-100 (1%) extracted P2X1 receptors (43). The Triton X-100 concentration-dependent localization of the P2X1 receptor was mirrored by the fractions in which the lipid raft marker flotillin-2 was found. This suggests that the association of P2X1 receptors in lipid rafts, like for other proteins, for example the T cell receptor in Jurkat cells (Ref. 44 and for a more general review, see Ref. 27), are sensitive to Triton X-100 extraction. This raises the possibility that the association of P2X1 receptors with lipid rafts may be regulated by glycerophospholipids or inner leaflet membrane lipids as these are depleted by Triton X-100 treatment.

P2X1 Receptors in Rafts in Smooth Muscle Cells—We have shown that recombinant P2X1 receptors are associated with lipid rafts and disruption of these leads to an inhibition of P2X1 receptor-mediated currents. In this series of studies we determined whether native P2X1 receptors are expressed in lipid rafts in smooth muscle preparations and whether disruption of the rafts can regulate the functional properties of native P2X1 receptors. Rat tail arteries were lysed under detergent-free conditions and ultracentrifuged on a discontinuous sucrose gradient. The P2X1 receptor protein was identified in the fractions 4 and 5 of the gradient just as the lipid raft markers, flotillin-1 and flotillin-2. P2X1 receptor protein also co-localized with caveolae (specialized subtype of lipid rafts) proteins caveolin-1 and caveolin-2 (Fig. 4a). The enriched cholesterol fractions represented by fractions 3, 4, and 5, contain more than 70% of the total cellular cholesterol (with a peak ~30% for fraction 4) but less than 10% of the total cellular protein (Fig. 4b). Taken together, these results confirm that P2X1 receptor protein is present in the cellular-enriched cholesterol fractions of rat tail arteries. P2X1 receptor protein and the lipid raft marker caveolin-1 were similarly distributed along rat vas deferens and bladder gradients in fractions 4 and 5 (Fig. 4c). It is interesting to note that there were slight differences in the distribution of lipid rafts between HEK293 cells and smooth muscle cells; P2X1 receptor and lipid raft-associated proteins were present in fractions 3 and 4 of HEK293 cells whereas in fractions 4 and 5 of smooth muscle cells. This localization reflected the distribution of cholesterol (for comparison see Figs. 1b and 4b). Because HEK293 cells and smooth muscles are distinct cell types, the membrane fractionation divergences are likely to be caused by cell membrane composition differences.



View larger version (23K):
[in this window]
[in a new window]
  		FIG. 4.
Presence of the P2X1 receptor in the lipid raft-enriched fractions prepared from rat smooth muscles (rat tail artery, vas deferens, and bladder). a, rat tail arteries were lysed and separated on a density gradient (45, 35, and 5% sucrose). Eleven fractions (from top to bottom of gradient) were separated on SDS-PAGE gels and blotted for the P2X1 receptor, caveolin-1, caveolin-2, flotillin-1, and flotillin-2. b, fractions collected in a were also assayed for cholesterol and total protein. Rat vas deferens (c) and bladder (d) were processed as described in a and immunoblotted for P2X1 receptor and caveolin-1. All the gels shown in Fig. 3 were representative of three separate experiments as well as for the cholesterol and protein assays.

 
Raft Disruption Reduces P2X1 Receptor-mediated Arterial Constriction—The treatment of rat tail arteries with the cholesterol depleting agent M{beta}-CD (10 mM for 1 h) disrupts lipid rafts and resulted in a redistribution of the P2X1 receptor along the gradient (Fig. 5a) similar to its effects observed previously on HEK293 P2X1cl-1 cells. Tail artery constriction amplitudes to {alpha},{beta}-meATP (10 µM for 10 min) were dramatically reduced by half after M{beta}-CD treatment (10 mM for 1 h), whereas the inactive analogue {alpha}-CD (10 mM for 1 h) had no effect (110.5 ± 5.8%, 52.5 ± 4.1%, and 115.4 ± 6.9% of the initial control response, respectively for control, M{beta}-CD and {alpha}-CD, n = 4–7 from three and four different animals) (Fig. 5, b and c). In contrast, vasoconstrictions induced by 60 mM KCl were unaffected either by treatment with M{beta}-CD or {alpha}-CD (97.3 ± 4.2%, 104.2 ± 10.9%, and 96.1 ± 2.5% of the initial control response, respectively for control, M{beta}-CD and {alpha}-CD, n = 4–8 from three and five different animals) demonstrating that the cyclodextrins do not interfere with the ability of the smooth muscle to contract. Taken together these data suggest that P2X1 receptors are associated with lipid rafts in arteries and that disruption of these rafts inhibits responses through the channel.



View larger version (24K):
[in this window]
[in a new window]
  		FIG. 5.
Lipid raft disruption and inhibition of P2X receptor-mediated contractions of the rat tail artery. a, cholesterol depletion with M{beta}-CD (10 mM for 1 h) redistributed the P2X1 receptor from the lipid raft fractions to a diffuse distribution throughout the sucrose gradient (representative gel shown of three separate experiments). b, {alpha},{beta}-meATP (10 µM) applied for 10 min (indicated by bar)-mediated transient contractions of the rat tail artery, these were reduced following treatment with M{beta}-CD (10 mM, 1 h) but were unaffected by the inactive analogue {alpha}-CD (10 mM, 1 h). c, summary of the effects of M{beta}-CD and {alpha}-CD on rat tail artery contractions evoked by potassium chloride or {alpha},{beta}-meATP (n = 4–8; p < 0.001).

 

   DISCUSSION
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
REFERENCES
 
The localization of the P2X1 receptor to the buoyant cholesterol-rich fractions and the co-localization with lipid raft markers (flotillins 1 and 2, and in addition for the smooth muscle preparations caveolin-1 and -2), combined with the reduction of functional P2X1 receptor mediated responses following interference with lipid raft cholesterol, provides strong evidence that P2X1 receptors are present in lipid rafts in HEK293 cells as well as smooth muscles (arteries, vas deferens, and bladder).

Lipid rafts are characterized as cholesterol- and sphingolipid-rich regions of membrane. Density fractionation of cholesterol-rich lipid rafts has shown that there is heterogeneity in the rafts (45) and demonstrates that there are likely to be different populations of microdomains that vary in lipid and protein composition. The only clearly identifiable subtype of lipid rafts are the caveolae (46), these membrane invaginations are characterized by the presence of caveolins. Many proteins are associated with caveolae through interaction with these caveolins; for example the ATP-sensitive potassium channel pore-forming subunit Kir6.1 co-immunoprecipitates with caveolin in arterial smooth muscle (47). We were unable to co-immunoprecipitate the P2X1 receptor with anti-caveolin antibodies2 suggesting that caveolin is not directly associated with the localization of the P2X1 receptor to lipid rafts. This is further supported by our work in HEK293 cells where levels of caveolin-1 and -2 were below the limit of detection (data not shown). A similar lack of caveolins has been reported in other HEK293 cell lines and used to suggest that {beta}-adrenoreceptor raft localization is not caveolin-dependent (37). However caveolins have been described in some HEK293 cell lines (39) and it seems likely that their expression may vary between different subclones of these cells. Myristylation and palmitylation of proteins may be involved in associations with caveolae (48, 49); however, the lack of motifs for such forms of protein modification suggests that this is unlikely for the P2X1 receptor. Additional support that caveolin-1 is unlikely to be involved in P2X1 receptor function comes from studies with knock-out mice; P2X1 receptor mice show male infertility because of a reduced contractile responses of the vas deferens (50), and in this study we show that disruption of lipid rafts with {beta}-CD reduced P2X1 receptor currents by >90%; however caveolin-1 knock-out mice show normal levels of fertility (51). Finally as P2X1 receptors are associated with rapid nerve-mediated depolarization of smooth muscle it seems counterintuitive that the receptor would be localized to membrane invaginations (caveolae), because the ATP would have to diffuse into the caveolae before activating the channel. It therefore seems likely that the P2X1 receptor is associated with non-caveolar lipid rafts.

Pike (27) has recently suggested a model where lipid rafts can be divided into three classes based on their sensitivity to extraction by a variety of methods: (i) Triton X-100- and CHAPS-resistant, (ii) Brij96, Brij98, and non-detergent isolation-resistant, and (iii) lubrol and Tween-resistant fractions. The findings that the P2X1 receptor is found in the buoyant lipid raft fraction when non-detergent methods are used and is sensitive to the concentration of Triton X-100 used suggests that the P2X1 receptor is associated with class (ii) lipid rafts; however, the motif/region of the receptor associated with raft localization, either directly or through an interacting protein remains to be determined.

Cholesterol depletion with M{beta}-CD resulted in a re-distribution of P2X1 receptors throughout the membrane fractions consistent with a disruption of the lipid rafts. Similar movements have been described for a range of ion channels and raft-associated proteins (e.g. 28, 39, 52). In addition M{beta}-CD treatment or the use of filipin to sequester cholesterol in the membrane to disrupt the lipid rafts (41, 42) reduced P2X1 receptor-mediated responses. Recombinant human P2X1 receptor currents recorded in HEK293 cells were reduced by >90% (also for recombinant rat P2X1 receptors, control 799 ± 137 pA and 31 ± 7 following M{beta}-CD treatment, p < 0.001, n = 10, 5) and contractions of arteries were reduced by ~50% (this difference most likely results from the reduced access of M{beta}-CD in whole artery studies compared with patch clamp studies on isolated single cells). It is unlikely that these effects of M{beta}-CD result from nonspecific effects or a block of the ability of the muscle to contract as responses evoked by depolarization with 60 mM KCl were unaffected by M{beta}-CD treatment (this study), and M{beta}-CD has previously been shown to have no effect on L-type calcium currents expressed in HEK293 cells (53). Similarly P2X1 receptor currents or contractions were unaffected by {alpha}-CD, the stereoisomer that has no effect on membrane cholesterol (40). In addition cholesterol repletion following M{beta}-CD treatment resulted in a significant restoration of P2X1 receptor-mediated responses. Taken together these data strongly suggest that the reduction in P2X1 receptor responsiveness is caused by depletion of cholesterol and disruption of the lipid rafts. Similar reductions in function following lipid raft disruption have been described for a number of other ion channels for example voltage-dependent potassium channel Kv2.1 (28) and cyclic nucleotide-gated channels (39).

Lipid raft association of the P2X1 receptor may be a method for bringing the receptor into an organized signaling domain. We have previously shown that P2X1 receptors are basally phosphorylated, P2X1 receptor currents are reduced following treatment with the tyrosine kinase inhibitor genistein and can be potentiated by kinase activation or stimulation of G{alpha}q-coupled receptors e.g. mGlur1{alpha} (54). M{beta}-CD treatment dissociates proteins from rafts and inactivates signaling cascades (26), for example the Src family of tyrosine kinases are present in rafts (30). Therefore disruption of the localized signaling pathways could result in disruption of ongoing regulatory mechanisms and account for the decrease in P2X1 responses following cholesterol depletion.

The association of P2X1 receptors in lipid rafts may not only be important in maintaining the responsiveness of the receptor but may also be a mechanism to achieve clustering of the receptor. Immunohistochemical and single channel recording studies have indicated that the P2X1 receptor is not randomly distributed in the membrane but forms clusters (23, 24) and that in smooth muscle preparations these clusters are often seen close to sympathetic nerve varicosities; the site of transmitter release. Thus lipid rafts may be a way of concentrating the P2X1 receptor at signaling hot spots. Calcium imaging studies on the rat tail artery showed the initial transient rise in calcium was caused by purinergic receptor stimulation, and this was quickly followed by the noradrenergic component that oscillates and propagates as a wave through the vessel (55). Subsequent, higher resolution studies from vas deferens (56), mesenteric arteries (9, 57), and bladder (58) showed discrete, localized, P2X receptor-mediated calcium rises in the smooth muscle cells following nerve stimulation. The sympathetic nerves that innervate arteries and the vas deferens release the co-transmitters ATP and noradrenaline. It is interesting that nerve evoked P2X receptor, but not {alpha}-adrenoreceptor mediated rises in calcium are recorded in response to short trains of stimulation from the vas deferens (56) and mesenteric arteries (9). A similar finding was reported in contractile studies on submucosal arterioles where following sympathetic nerve stimulation the vasoconstriction is mediated solely by P2X receptors, noradrenaline is released from the nerves but acts prejunctionally through {alpha}2-adrenoceptors to regulate transmitter release (6). These data suggest that although sympathetic nerves release both ATP and noradrenaline under certain conditions P2X receptors appear to be preferentially activated. One possible reason for this could be the differential membrane localization of P2X and {alpha}-adrenoceptors. This seems likely because in this study we have shown that the P2X1 receptor is localized in lipid rafts, and in previous work it has been shown that {alpha}1-adrenoceptors are not present in the lipid raft fractions, and noradrenaline-mediated contractions are not affected by cholesterol depletion with M{beta}-CD (59). This would provide a mechanism where P2X1 receptors in lipid rafts could be concentrated close to the site of transmitter release while {alpha}-adrenoceptors would be excluded from these domains and thus be less responsive and require longer periods of nerve stimulation to be activated (57).

In summary the present study shows for the first time that P2X1 receptors are associated with lipid rafts and that disruption of these rafts compromises P2X1 receptor responsiveness probably through interference with organized signaling microdomains. This has significant implications for cardiovascular function where P2X1 receptors have been shown to have important signaling roles, for example in the control of resistance artery vasoconstriction following sympathetic nerve stimulation (6, 11), pressure-induced autoregulation in the kidney (12), and platelet regulation (18–22).


   FOOTNOTES
 
* This work was supported by the Wellcome Trust. The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact. Back

{ddagger} To whom correspondence should be addressed. Tel.: 44-116-252-3032; Fax: 44-116-252-5045; E-mail: rje6{at}le.ac.uk.

1 The abbreviations used are: {alpha},{beta}-meATP, adenosine 5'-[{alpha},{beta}-methylene]triphosphate; HEK, human embryonic kidney; MES, 4-morpholineethanesulfonic acid; MAP, mitogen-activated protein; CHAPS, 3-[(3-cholamidopropyl)dimethylammonio]-1-propanesulfonic acid; EGFP, enhanced green fluorescent protein; CD, cyclodextrin. Back

2 C. Vial and R. Evans, unpublished observations. Back


   ACKNOWLEDGMENTS
 
We thank Drs. C. Dart and L. J. Sampson for discussions and help with raft protocols and Dr. B. D. Grubb for help with the confocal microscopy.



   REFERENCES
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 

  1. Ralevic, V., and Burnstock, G. (1998) Pharmacol. Rev. 50, 413–492[Abstract/Free Full Text]
  2. Lewis, C. J., Ennion, S. J., and Evans, R. J. (2000) J. Physiol. 527, 315–324[Abstract/Free Full Text]
  3. Evans, R. J., and Cunnane, T. C. (1992) Naunyn Schmiedeberg's Arch. Pharmacol. 345, 424–430[Medline] [Order article via Infotrieve]
  4. Gitterman, D. P., and Evans, R. J. (2001) Br. J. Pharmacol. 132, 1201–1208[CrossRef][Medline] [Order article via Infotrieve]
  5. Ramme, D., Regenold, J. T., Starke, K., Busse, R., and Illes, P. (1987) Naunyn Schmiedeberg's Arch. Pharmacol. 336, 267–273[Medline] [Order article via Infotrieve]
  6. Evans, R. J., and Surprenant, A. (1992) Br. J. Pharmacol. 106, 242–249[Medline] [Order article via Infotrieve]
  7. Benham, C. D., and Tsien, R. W. (1987) Nature 328, 275–278[CrossRef][Medline] [Order article via Infotrieve]
  8. Benham, C. D. (1989) J. Physiol. 419, 689–701[Abstract/Free Full Text]
  9. Lamont, C., and Wier, W. G. (2002) Circ. Res. 91, 454–456[Abstract/Free Full Text]
  10. North, R. A. (2002) Physiol. Rev. 82, 1013–1067[Abstract/Free Full Text]
  11. Vial, C., and Evans, R. J. (2002) Mol. Pharmacol. 62, 1438–1445[Abstract/Free Full Text]
  12. Inscho, E. W., Cook, A. K., Imig, J. D., Vial, C., and Evans, R. J. (2003) J. Clin. Investig. 112, 1895–1905[CrossRef][Medline] [Order article via Infotrieve]
  13. Inscho, E. W., Cook, A. K., Imig, J. D., Vial, C., and Evans, R. J. (2004) Acta. Physiol. Scand. 181, 445–453[CrossRef][Medline] [Order article via Infotrieve]
  14. Malmsjo, M., Bergdahl, A., Moller, S., Zhao, X.-H., Sun, X.-Y., Hedner, T., Edvinsson, L., and Erlinge, D. (1999) Cardiovasc. Res. 43, 219–227[CrossRef][Medline] [Order article via Infotrieve]
  15. Berry, D. A., Barden, J. A., Balcar, V. J., Keogh, A., and dos Remedios, C. G. (1999) Electrophoresis 20, 2059–2064[CrossRef][Medline] [Order article via Infotrieve]
  16. Wang, L., Andersson, M., Karlsson, L., Watson, M. A., Cousens, D. J., Jern, S., and Erlinge, D. (2003) Arterioscler. Thromb. Vasc. Biol. 23, 1370–1376[Abstract/Free Full Text]
  17. Li, J., Sinoway, A. N., Gao, Z., Maile, M. D., Pu, M., and Sinoway, L. I. (2004) Circulation 110, 3049–3054[Abstract/Free Full Text]
  18. Vial, C., Rolf, M. G., Mahaut-Smith, M. P., and Evans, R. J. (2002) Br. J. Pharmacol. 135, 363–372[CrossRef][Medline] [Order article via Infotrieve]
  19. Toth-Zsamboki, E., Oury, C., Cornelissen, H., De Vos, R., Vermylen, J., and Hoylaerts, M. F. (2003) J. Biol. Chem. 278, 46661–46667[Abstract/Free Full Text]
  20. Oury, C., Sticker, E., Cornelissen, H., De Vos, R., Vermylen, J., and Hoylaerts, M. F. (2004) J. Biol. Chem. 279, 26266–26273[Abstract/Free Full Text]
  21. Oury, C., Kuijpers, M. J., Toth-Zsamboki, E., Bonnefoy, A., Danloy, S., Vreys, I., Feijge, M. A., De Vos, R., Vermylen, J., Heemskerk, J. W., and Hoylaerts, M. F. (2003) Blood 101, 3969–3976[Abstract/Free Full Text]
  22. Hechler, B., Lenain, N., Marchese, P., Vial, C., Heim, V., Freund, M., Cazenave, J.-P., Cattaneo, M., Ruggeri, Z. M., Evans, R. J., and Gachet, C. (2003) J. Exp. Med. 198, 661–667[Abstract/Free Full Text]
  23. Hansen, M. A., Dutton, J. L., Balcar, V. J., Barden, J. A., and Bennett, M. R. (1999) J. Auton. Nervous Sys. 75, 147–155
  24. Lewis, C. J., Davies, N. W., and Evans, R. J. (2001) Drug. Dev. Res. 52, 164–169[CrossRef]
  25. Vial, C., Tobin, A. B., and Evans, R. J. (2004) Biochem. J. 382, 101–110[CrossRef][Medline] [Order article via Infotrieve]
  26. Simons, K., and Toomre, D. (2000) Nat. Rev. Mol. Cell. Biol. 1, 31–39[CrossRef][Medline] [Order article via Infotrieve]
  27. Pike, L. J. (2004) Biochem. J. 378, 281–292[CrossRef][Medline] [Order article via Infotrieve]
  28. Xia, F., Gao, X., Kwan, E., Lam, P. P., Chan, L., Sy, K., Sheu, L., Wheeler, M. B., Gaisano, H. Y., and Tsushima, R. G. (2004) J. Biol. Chem. 279, 24685–24691[Abstract/Free Full Text]
  29. Foster, L. J., De Hoog, C. L., and Mann, M. (2003) Proc. Natl. Acad. Sci. U. S. A. 100, 5813–5818[Abstract/Free Full Text]
  30. Martens, J. R., O'Connell, K., and Tamkun, M. (2004) Trends Pharmacol. Sci. 25, 16–21[CrossRef][Medline] [Order article via Infotrieve]
  31. Ostrom, R. S., Liu, X., Head, B. P., Gregorian, C., Seasholtz, T. M., and Insel, P. A. (2002) Mol. Pharmacol. 62, 983–992[Abstract/Free Full Text]
  32. Ostrom, R. S. (2002) Mol. Pharmacol. 61, 473–476[Free Full Text]
  33. Ennion, S. J., and Evans, R. J. (2001) FEBS Lett. 489, 154–158[CrossRef][Medline] [Order article via Infotrieve]
  34. Lewis, C. J., and Evans, R. J. (2000) Br. J. Pharmacol. 131, 1659–1666[CrossRef][Medline] [Order article via Infotrieve]
  35. Lewis, C. J., Gitterman, D. P., Schluter, H., and Evans, R. J. (2000) Br. J. Pharmacol. 129, 124–130[CrossRef][Medline] [Order article via Infotrieve]
  36. Bickel, P. E., Scherer, P. E., Schnitzer, J. E., Oh, P., Lisanti, M. P., and Lodish, H. F. (1997) J. Biol. Chem. 272, 13793–13802[Abstract/Free Full Text]
  37. Rybin, V. O., Xu, X., Lisanti, M. P., and Steinberg, S. F. (2000) J. Biol. Chem. 275, 41447–41457[Abstract/Free Full Text]
  38. Ostrom, R. S., Gregorian, C., Drenan, R. M., Xiang, Y., Regan, J. W., and Insel, P. A. (2001) J. Biol. Chem. 276, 42063–42069[Abstract/Free Full Text]
  39. Brady, J. D., Rich, T. C., Le, X., Stafford, K., Fowler, C. J., Lynch, L., Karpen, J. W., Brown, R. L., and Martens, J. R. (2004) Mol. Pharmacol. 65, 503–511[Abstract/Free Full Text]
  40. Grassme, H., Jekle, A., Riehle, A., Schwarz, H., Berger, J., Sandhoff, K., Kolesnick, R., and Gulbins, E. (2001) J. Biol. Chem. 276, 20589–20596[Abstract/Free Full Text]
  41. Reungpatthanaphong, P., Marbeuf-Gueye, C., Le Moyec, L., Salerno, M., and Garnier-Suillerot, A. (2004) J. Bioenerg. Biomembr. 36, 533–543[CrossRef][Medline] [Order article via Infotrieve]
  42. Bang, B., Gniadecki, R., and Gajkowska, B. (2005) Exp. Dermatol. 14, 266–272[CrossRef][Medline] [Order article via Infotrieve]
  43. Vacca, F., Amadio, S., Sancesario, G., Bernardi, G., and Volonte, C. (2004) J. Neurosci. Res. 76, 653–661[CrossRef][Medline] [Order article via Infotrieve]
  44. Janes, P. W., Ley, S. C., and Magee, A. I. (1999) J. Cell Biol. 147, 447–461[Abstract/Free Full Text]
  45. Hering, H., Lin, C. C., and Sheng, M. (2003) J. Neurosci. 23, 3262–3271[Abstract/Free Full Text]
  46. Lai, E. C. (2003) J. Cell Biol. 162, 365–370[Abstract/Free Full Text]
  47. Sampson, L. J., Hayabuchi, Y., Standen, N. B., and Dart, C. (2004) Circ. Res. 95, 1012–1018[Abstract/Free Full Text]
  48. Lee, H., Woodman, S. E., Engelman, J. A., Volonte, D., Galbiati, F., Kaufman, H. L., Lublin, D. M., and Lisanti, M. P. (2001) J. Biol. Chem. 276, 35150–35158[Abstract/Free Full Text]
  49. Galbiati, F., Volonte, D., Meani, D., Milligan, G., Lublin, D. M., Lisanti, M. P., and Parenti, M. (1999) J. Biol. Chem. 274, 5843–5850[Abstract/Free Full Text]
  50. Mulryan, K., Gitterman, D. P., Lewis, C. J., Vial, C., Leckie, B. J., Cobb, A. L., Brown, J. E., Conley, E. C., Buell, G., Pritchard, C. A., and Evans, R. J. (2000) Nature 403, 86–89[CrossRef][Medline] [Order article via Infotrieve]
  51. Drab, M., Verkade, P., Elger, M., Kasper, M., Lohn, M., Lauterbach, B., Menne, J., Lindschau, C., Mende, F., Luft, F. C., Schedl, A., Haller, H., and Kurzchalia, T. V. (2001) Science 293, 2449–2452[Abstract/Free Full Text]
  52. Martens, J. R., Navarro-Polanco, R., Coppock, E. A., Nishiyama, A., Parshley, L., Grobaski, T. D., and Tamkun, M. M. (2000) J. Biol. Chem. 275, 7443–7446[Abstract/Free Full Text]
  53. Lohn, M., Furstenau, M., Sagach, V., Elger, M., Schulze, W., Luft, F. C., Haller, H., and Gollasch, M. (2000) Circ. Res. 87, 1034–1039[Abstract/Free Full Text]
  54. Vial, C., Tobin, A. B., and Evans, R. J. (2004) Biochem. J. 382, 101–110[CrossRef][Medline] [Order article via Infotrieve]
  55. Iino, M., Kasai, H., and Yamazawa, T. (1994) EMBO J. 13, 5026–5031[Medline] [Order article via Infotrieve]
  56. Brain, K. L., Jackson, V. M., Trout, S. J., and Cunnane, T. C. (2002) J. Physiol. 541, 849–862[Abstract/Free Full Text]
  57. Lamont, C., Vainorius, E., and Wier, W. G. (2003) J. Physiol. 549, 801–808[Abstract/Free Full Text]
  58. Heppner, T. J., Bonev, A. D., and Nelson, M. T. (2005) J. Physiol. 564, 201–212[Abstract/Free Full Text]
  59. Dreja, K., Voldstedlund, M., Vinten, J., Tranum-Jensen, J., Hellstrand, P., and Sward, K. (2002) Arterioscler. Thromb. Vasc. Biol. 22, 1267–1272[Abstract/Free Full Text]

Add to CiteULike CiteULike   Add to Complore Complore   Add to Connotea Connotea   Add to Del.icio.us Del.icio.us   Add to Digg Digg   Add to Reddit Reddit   Add to Technorati Technorati    What's this?


This article has been cited by other articles:


Home page
 Mol. Pharmacol.Home page
L.-P. Bernier, A. R. Ase, X. Tong, E. Hamel, D. Blais, Q. Zhao, D. E. Logothetis, and P. Seguela
Direct Modulation of P2X1 Receptor-Channels by the Lipid Phosphatidylinositol 4,5-Bisphosphate
Mol. Pharmacol., September 1, 2008; 74(3): 785 - 792.
[Abstract] [Full Text] [PDF]

Home page
 J. Biol. Chem.Home page
A. K. Weaver, M. L. Olsen, M. B. McFerrin, and H. Sontheimer
BK Channels Are Linked to Inositol 1,4,5-Triphosphate Receptors via Lipid Rafts: A NOVEL MECHANISM FOR COUPLING [Ca2+]i TO ION CHANNEL ACTIVATION
J. Biol. Chem., October 26, 2007; 282(43): 31558 - 31568.
[Abstract] [Full Text] [PDF]