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Papers In Press, published online ahead of print June 1, 2007
J. Lipid Res., doi:10.1194/jlr.M600485-JLR200

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Journal of Lipid Research, Vol. 48, 1325-1335, June 2007
Copyright © 2007 by American Society for Biochemistry and Molecular Biology

FcRI and Thy-1 domains have unique protein and lipid compositions

Zurab Surviladze^*, Kathleen A. Harrison, Robert C. Murphy and Bridget S. Wilson^1,*

^* Department of Pathology, University of New Mexico, Albuquerque, NM
Department of Pharmacology, University of Colorado at Denver and Health Sciences Center, Aurora, CO

The online version of this article (available at http://www.jlr.org) contains supplementary data in the form of three figures and two tables.

Published, JLR Papers in Press, March 26, 2007.

¹ To whom correspondence should be addressed. e-mail: bwilson{at}salud.unm.edu

	ABSTRACT

TOP ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
Receptor activation leads to the dynamic remodeling of the plasma membrane. Previous work using immunoelectron microscopy showed that aggregated high-affinity receptor for immunoglobulin E (FcRI) and aggregated Thy-1, a glycerophosphoinositol (GPI)-anchored protein, have distinct membrane distributions. We now report lipidomics analysis of FcRI- and Thy-1-enriched vesicles obtained by magnetic bead isolation in the absence of detergent. Protein analyses show that FcRI domains are enriched in receptors and associated signaling molecules, whereas Thy-1 domains are devoid of FcRI subunits. Positive and negative ion electrospray mass spectrometry demonstrated that both domains retained a complex mixture of phospholipid classes and molecular species, predominantly glycerophosphocholine, glycerophosphoethanolamine (GPE), and sphingomyelin as well as glycerophosphoserine and GPI lipids. Analysis of total acyl groups showed that <50% of fatty acids in these domains are fully saturated, inconsistent with the recruitment of aggregated receptors or GPI-anchored proteins to liquid ordered domains. However, further analysis showed that FcRI domains contain two times more sphingomyelin and a high ratio of cholesterol to total fatty acid content compared with Thy 1-enriched domains. Remarkably, plasmenyl glycerophosphoethanolamine phospholipids (plasmalogen GPE) were also 2.5–3 times more abundant in FcRI domains than in the Thy-1 microdomains, whereas most diacyl GPE molecular species were equally abundant in the two domains.

Supplementary key words lipidomics • membrane microdomains • lipid rafts • immunoglobulin E receptor • glycerophosphoinositol-anchored proteins

Abbreviations: DRM, detergent-resistant membrane; ESI, electrospray ionization; FcRI, high-affinity receptor for immunoglobulin E; GPC, glycerophosphocholine; GPE, glycerophosphoethanolamine; GPI, glycerophosphoinositol; GPS, glycerophosphoserine; MßCD, methyl-ß-cyclodextrin; MS/MS, tandem mass spectrometry

	INTRODUCTION

TOP ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
Receptor activation leads to the dynamic remodeling of the plasma membrane, facilitating the initiation, propagation, and termination of intracellular signaling. This remodeling of the membrane includes both the redistribution of membrane proteins and the activation of a host of enzymes that directly modify lipid substrates, including the phospholipases, inositol kinases, and phosphatases. Early insight into the importance of local lipid environments was provided by a series of studies using sucrose density centrifugation techniques to isolate detergent-resistant membranes (DRMs) from cell lysate preparations (1). The light fractions of these gradients are also often referred to as "lipid rafts," reflecting their enrichment in cholesterol, sphingomyelins, and gangliosides (2) and in proteins that are covalently attached to lipid. Classical examples of the latter group include the Src and G-protein family proteins that are anchored to the inner leaflet of the lipid bilayer by acylation with fully saturated fatty acids (palmitate and/or myristate) (3–7). Glycerophosphoinositol (GPI)-anchored proteins in the outer leaflet, such as alkaline phosphatase and Thy-1, also float to the light fractions of density gradients (8, 9). Importantly, ligand-dependent shifts in receptor distributions in lipid raft fractions have supported the notion that movement in and out of these specific membrane domains is key to the signaling process (10–14).

Although these analyses have advanced the field, there are several limitations to lipid raft analysis by fractionation (15, 16). Compartments that were previously separate in native membranes can merge during the extraction process with detergents (17). Fractionation results are known to be dramatically altered by varying the concentration of Triton X-100 (18, 19), by the use of alternative detergents (11, 20, 21), or by the omission of detergent altogether (4, 22, 23). During the past decade, new biophysical and microscopic methods have been needed to estimate the size of putative microdomains, which are below the resolution (>300 nm) of conventional fluorescence microscopy (reviewed in Ref. 24). Several groups have proposed that rafts in resting cells are small, <70 nm (25, 26). Quantitative measurements of protein and lipid diffusion, including applications of fluorescence resonance energy transfer and single-particle tracking, have demonstrated that membrane components move at significantly slower rates than predicted from experiments in artificial membranes (27, 28). Membrane components also often appear to rapidly hop past diffusional barriers set up by interactions of membrane proteins and lipids with the cortical cytoskeleton (29) or possibly by transient residency in microdomains via a process of "dynamic partitioning" (30). This work has collectively demanded a revision of the classic view of randomly distributed membrane species, based upon the Singer-Nicolson model, to a new paradigm that has been described as a "dynamically structured mosaic model" (31). In recognition that many factors govern membrane organization, the term "lipid raft" has been replaced by many in the field with the term "membrane raft" (32).

Our group has sought alternative, detergent-free methods to evaluate the native distributions of receptors and their signaling partners. One powerful technique uses transmission electron microscopy of fixed, immunogold-labeled plasma membrane sheets, or "rip-flips" (33). By direct labeling of sheets prepared from resting cells, we found that clusters of high-affinity receptors for immunoglobulin E (FcRI) and Thy-1 are very small (20–50 nm) in fixed membranes (34). Upon cross-linking, IgE receptors and a subset of their associated signaling proteins redistribute into large signaling patches (35, 36). Importantly, because the aggregation of IgE-bound receptors by polyvalent antigen is the physiological cue for FcRI activation, these signaling patches closely approximate normal signaling architecture. Immune complexes have also been used by us and others (25, 34, 37) to aggregate GPI-anchored proteins on the surfaces of living cells, coalescing these putative raft markers into large aggregates that can be visualized by conventional fluorescence microscopy techniques. Electron microscopy of labeled membrane sheets demonstrated that aggregates of FcRI and Thy-1 have distinct membrane distributions with little or no overlap (34).

In this work, magnetic beads were used to immunoisolate detergent-free membrane vesicles enriched in aggregated FcRI or Thy-1 membrane proteins and their associated lipid environment. Although both sets of vesicles contain complex mixtures of phospholipids, there are remarkable differences between them. Cholesterol, traditionally associated with lipid raft integrity, constitutes 50% of the lipid content of FcRI microdomains but <25% of the lipid associated with GPI-anchored aggregates. FcRI microdomains also contain greater than two times more glycerophosphoethanolamine (GPE) plasmalogen and sphingomyelin species. These data suggest that the local lipid environment of receptors is both richer and less dependent on acyl chain saturation than proposed by the lipid raft hypothesis. These results are discussed in relation to prior lipidomics studies (38, 39) that analyzed the lipid composition of vesicles floating in bulk to the sucrose density light fractions with and without the influence of detergent.

	MATERIALS AND METHODS

TOP ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
Reagents and cell culture
RBL-2H3 cells were grown as adherent cultures in MEM (Gibco Life Technologies, Inc., Grand Island, NY) supplemented with 10% Hybrimax serum substitute (Sigma), fresh L-glutamine, and antibiotics. Where specified, cells were incubated overnight with 1 µg/ml murine dinitrophenol-specific IgE to prime IgE receptors. The IgE was affinity-purified from ascites using a trinitrophenol-conjugated Sepharose column.

For magnetic bead isolation, we used rabbit anti-IgE antibodies that were affinity-purified on a column composed of Sepharose conjugated to mouse IgE. For Western blotting of subunits of the FcRI, mouse monoclonal anti-rat (ER14) antibodies were generously provided by Dr. Reuben Siraganian (National Institutes of Health), anti-rat ß monoclonal antibodies were a gift from Juan Rivera (National Institutes of Health), and rabbit polyclonal anti- antibodies were from Upstate Biological (Charlottesville, VA). Anti-OX7 antibodies were from BD Biosciences. Polyclonal anti-human FcRI was from US Biological (Swampscott, MA). Anti-Lyn and anti-Syk polyclonal antibodies were from Santa Cruz Biotechnology (Santa Cruz, CA). Colloidal gold secondary antibodies were from Amersham/GE Life Sciences (Piscataway, NJ). Rabbit anti-mouse IgG (Fc fragments) were from Jackson Laboratories. N-hydroxysuccinimide-biotin and avidin-HRP were from Sigma.

Membrane isolation
RBL-2H3 cells (60 x 10⁶) were harvested with 1 mM EDTA in PBS. To aggregate surface GPI-anchored Thy-1 molecules, cells were washed, resuspended in Hanks' buffer, and incubated with OX-7 antibodies (1 µg/ml) at room temperature for 25 min. Cells were washed two times with Hanks' buffer and incubated with rabbit anti-mouse IgG (10 µg/ml) for 10 min at 37°C. To aggregate surface FcRI, IgE-primed RBL cells were harvested with EDTA-PBS, washed, resuspended in Hanks' buffer, and incubated with anti-IgE polyclonal antibodies (5 µg/ml) for 3 min at 37°C. In both cases, cells were transferred to an ice bath, followed by the addition of 10 ml of ice-cold Hanks' buffer. Cells were collected by centrifugation at 4°C, washed with cold Hanks' solution, and resuspended in 10 ml of cold hypotonic buffer (10 mM Tris, pH 7.5, 10 mM KCl, 5 mM MgCl₂, and 1 mM EGTA) supplemented with 1 mM vanadate and protease inhibitors. All tubes and pipette tips were rinsed with chloroform-methanol (2:1) solution to remove any lipid contaminants and other organic solvent-soluble contaminants that interfere with mass spectrometric analyses. Fatty acid-free BSA (Sigma) was used for the preparation of Hanks' buffer. For the preparation of negative controls, the same number of RBL cells were harvested, washed, and resuspended in hypotonic buffer.

Homogenization steps were performed on ice. Cells in hypotonic buffer were passed through a 26 g needle five times. Broken cells were then passed through a ball-bearing-style cell cracker (15–20 strokes), followed by 20 s of sonication. Unbroken cells were sedimented by centrifugation (600 g for 10 min at 4°C) and discarded. The supernatant was centrifuged at 16,000 g for 45 min at 4°C. The resulting membrane-enriched pellet fraction was resuspended in 3 ml of cold PBS and again sonicated for 15 s. Aggregated material was removed by low-speed centrifugation for 10 min. Combined supernatants were used for immunoisolation of microdomains. An equal amount of sheep anti-rabbit IgG-Dynabeads M-280 (Dynal Biotech) was added to each sample. Samples were diluted up to 4 ml with cold PBS and incubated overnight at 4°C on a wheel rotator. Magnetic beads were washed five times with 3 ml of cold PBS. For protein analysis, beads were resuspended in loading buffers appropriate for one-dimensional or two-dimensional electrophoresis. For lipid analysis, beads were transferred into the glass vials and treated with 100 µl of methanol-water (2:1). Vials were closed under nitrogen and stored at –20°C until lipid extraction.

Lipid extraction
Lipids were recovered from the magnetic beads by the addition of 400 µl of ethanol containing appropriate internal standard(s) for subsequent procedures. Ethanol was used rather than CH₂Cl₂/methanol because the polystyrene beads are not resistant to CH₂Cl₂. Ethanol extraction of phospholipids has been described (40). The beads and solvent were vortexed and centrifuged to pellet the beads, and the supernatant was drawn off with a pipette.

Cholesterol analysis
For cholesterol analysis, 50 ng of [²H₆]cholesterol internal standard (97 atom% excess; Cambridge Isotope Laboratories, Inc., Andover, MA) was added to the ethanol extraction. Aliquots (100 µl) were transferred to a screw-cap glass tube, dried under N₂, and resuspended in 50 µl of acetonitrile plus 50 µl of N,O-bis(trimethylsilyl)-trifluoroacetamide. The tubes were heated to 60°C for 20 min to convert the free hydroxy to the trimethylsilyl ether derivative for GC-MS analysis. Positive ion electron ionization mass spectrometry was used to monitor m/z 369 and 374 (corresponding to the [M-TMSOH]⁺ ions for endogenous cholesterol and deuterium-labeled [²H₆]cholesterol internal standard, respectively). Quantitation was performed by comparison of the chromatographic peak area ratio of m/z 369 to m/z 374 with a seven point standard curve (1.6–5,000 ng of cholesterol). Conditions for GC-MS were as follows: 30 m x 0.25 mm ZB-1 (Phenomenex, Torrance, CA); 0.1 µm film thickness; temperature programmed from 150°C to 300°C at 20°C/min, then held at 300°C for 2.5 min; quadrupole mass spectrometer (TRACE DSQ; Thermo-Finnigan, San Jose, CA); 70 eV electron ionization; source temperature of 200°C; and helium used as the carrier gas at 1.5 ml/min.

Fatty acid analysis
Total fatty acid analysis was performed after base hydrolysis of a 100 µl aliquot of the ethanol supernatant. Stable isotope-labeled palmitic acid ([¹³C₄]16:0) (97 atom% excess; Cambridge Isotope Laboratories), stearic acid ([²H₃]18:0) (98 atom% excess; Cambridge Isotope Laboratories), oleic acid ([²H₂]18:1) (97 atom% excess; Cambridge Isotope Laboratories), and arachidonic acid ([²H₈]20:4) (96 atom% excess; Cayman Chemical, Ann Arbor, MI) served as internal standards. Base hydrolysis was accomplished by the addition of 100 µl of 1 N NaOH and saponification for 30 min. Acidification of the reaction with HCl followed by extraction with isooctane recovered the total fatty acids in the lipid extract. Fatty acids were converted to pentafluorobenzyl esters (1% pentafluorobenzyl bromide, 1% diisopropylethylamine in acetonitrile, 20 min, room temperature) for analysis by negative ion chemical ionization GC-MS with selected ion monitoring of the [M-PFB] ions (41). Procedural blanks were obtained by ethanol extraction of magnetic beads that had not been exposed to cells and were used alongside the samples to correct for background levels of fatty acids. Quantitation of the fatty acids was determined by comparisons of the peak area ratios of the fatty acid [M-PFB] ions with the [M-PFB] ions of their internal standards on a seven point standard curve constructed for each fatty acid (0.32–1,000 ng range). The GC-MS conditions were the same as those used for cholesterol analysis except that negative ions were monitored and methane was used as the reagent gas.

Phospholipid analysis
Lipid extracts were first treated by adding 200 ng of 17:0a/17:0 GPE internal standard (Avanti%20Polar%20Lipids">Avanti Polar Lipids, Alabaster, AL), then analyzed using normal-phase HPLC-electrospray ionization (ESI)-MS and tandem mass spectrometry (MS/MS) phospholipid polar head group scans, with 90% split to a fraction collector for further analyses (42). Separation of the phospholipid classes was achieved using a 4.6 mm x 250 mm silica column (Ultremex 5u; Phenomenex) with a gradient of hexane-isopropanol-water containing 1 mM NH₄OAc. Gradient elution proceeded from 47% B applied to the column for 6 min, then increased to 100% B over 20 min and held for 30 min, where solvent A = 3:4 hexane-isopropanol and solvent B = 3:4:0.7 hexane-isopropanol-water and 1 mM NH₄OAc. The flow rate was maintained at 1 ml/min throughout. Under these conditions, neutral lipids (including cholesterol) elute first, followed by GPI, GPE, glycerophosphoserine (GPS), glycerophosphocholine (GPC), and sphingomyelin. Multiple scans were performed throughout the analyses. GPI was detected using negative ESI. GPE was detected by positive ion ESI as well as the neutral loss of 141u (NL 141). In the NL 141 scan, the phosphoethanolamine polar head group left as a neutral fragment, leaving the charge on the remainder of the molecule. This procedure selectively detected the diacyl glycerol ions and severely discriminated against plasmalogens and alkyl ether molecular species of GPE (43). GPS was detected by the neutral loss of 185u, which corresponded to the loss of phosphoserine from the protonated molecular ions of GPS species. GPC and sphingomyelin were detected by monitoring the precursors of m/z 184, the phosphocholine ion. Analyses were performed on an Applied Biosystems (Framingham, MA) API 3000 triple quadrupole mass spectrometer. The ion spray voltage was 4,600 V, declustering potential was 70 V, collision energy was 30 eV, and collisional gas setting was 8.

Analysis of GPE species using isotope-tagged derivative
Precise determination of differences in GPE molecular species composition was carried out using a stable isotope dilution strategy after isolation of this class of phospholipids from the original ethanol extract. For these experiments, the remainder of the GPE fractions collected during LC-MS were derivatized with the isotope-tagged N-methylpiperazine N-hydroxy succinimide ester reagent (iTRAQ derivative; Applied Biosystems) as described (44) The GPE from the control (no primary antibody added) was derivatized with the 115-isotope-tagged reagent, the Thy-1 GPE was derivatized with the 117-isotope-tagged reagent, and the FcRI GPE was derivatized with the 114-isotope-tagged reagent. The isotope-tagged samples were then combined and analyzed by nanoflow ESI-MS/MS/MS. The MH⁺ ions were chosen from a survey scan of the precursors of m/z 286. These MH⁺ ions were decomposed in the collision cell (Q2), and their common product ion (m/z 286, which contains the isotope tags) was stored in the linear ion trap (Q3-linear ion trap) and collisionally decomposed to produce reporter ions, which were mass analyzed and detected. The peak areas for each reporter ion (m/z 114 for FcR1, m/z 115 for the control, and m/z 117 for Thy-1) were divided by the peak area of the reporter ion for the 17:0a/17:0 GPE internal standard to correct for sample losses. Analyses were performed on an Applied Biosystems API 4000 triple quadrupole-linear ion trap mass spectrometer equipped with the Advion Nanomate (Ithaca, NY) for nanospray ionization sample introduction. The lipids were dissolved in methanol:AcCN:10 mM NH₄OAc (60:20:20) and diluted so that the internal standard concentration was 20 pg/µl. The API 4000 was operated with declustering potential of 80 V, high collisional gas setting, collision energy of 40 eV, and ion trapping time of 300 ms. The Nanomate was operated with a voltage of 1.33 kV and gas pressure of 0.13 p.s.i.

	RESULTS

TOP ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
Harder and Kunh (45) previously described a novel approach to the isolation of plasma membrane fragments. Working with Jurkat T-cells, they incubated cells with anti-CD3-coated magnetic beads, followed by mechanical disruption. Membrane recovered on the magnetic beads was 50-fold enriched for T cell receptor compared with the bulk membrane. We modified this technique to isolate very small patches of RBL membranes representative of domains surrounding aggregates of either FcRI or the GPI-anchored protein Thy-1. This detergent-free strategy yielded a highly enriched preparation of right side out membrane vesicles. The protocol was initiated by incubating live RBL cells with rabbit polyclonal antibodies to IgE (which cross-link IgE-primed FcRI) or a combination of mouse monoclonal anti-Thy-1 antibodies and polyclonal anti-mouse secondary antibodies (which aggregate GPI-anchored surface Thy-1 molecules). After incubation, cells were lysed at 4°C by a combination of mechanical disruption and sonication. Vesicles enriched in FcRI or Thy-1 aggregates were then immunoisolated on magnetic beads. Dynal beads were chosen for their relatively smooth surface, as characterized previously by Saucan and Palade (46). The size and specificity of bound vesicles was determined by labeling immunoisolated FcRI vesicles with anti-IgE immune complexes conjugated to 10 nm colloidal gold, glutaraldehyde fixation, dehydration, and embedding in Epon. Ultrathin sections were prepared and examined by transmission electron microscopy. Figure 1A shows a cross-sectional view of a magnetic bead whose surface was coated with many small vesicles (diameter < 100 nm) that label specifically with gold directed at IgE bound to surface receptors (arrows). Vesicles of similar size and purity were isolated using anti-Thy1 reagents (data not shown). Figure 1B shows a cross-sectional view of a magnetic bead that was incubated with lysates in the absence of primary antibodies. These control beads are clean of bound vesicles. A diagram of the isolation strategy is provided in supplementary Fig. I.

View larger version (56K): [in this window] [in a new window]   Fig. 1. A: Cross-sectional view of a magnetic bead coated with anti-IgE antibodies and bound to vesicles containing IgE-bound receptors. Images were acquired by transmission electron microscopy of ultrathin sections. Arrows point to anti-IgE gold used to confirm the presence of high-affinity receptor for immunoglobulin E (FcRI) in bound vesicles. B: Control bead that was incubated with membrane fractions, but no primary antibody, is clean. C: After isolation using anti-IgE or anti-Thy1 antibodies, vesicles were lysed in Laemmli buffer, and proteins were separated by SDS-PAGE, transferred to nitrocellulose, and blotted to demonstrate unique subsets of proteins in the two vesicle populations. Results are representative of three separate experiments.

Two-dimensional gel electrophoresis was next used to more fully characterize the protein composition of the two vesicle preparations. Results in Fig. 2 show blots stained for overall protein by incubating membranes in borate buffer containing N-hydroxysuccinimide-biotin, which labels free amine groups. Protein spots on the membranes were visualized by sequential incubation with avidin-HRP and chemiluminescence solution, followed by film development. Figure 2A represents total proteins in FcRI-enriched domains and Fig. 2B represents total proteins in Thy-1-enriched domains. Spots representing unique proteins in each preparation are circled, illustrating that although there is some overlap in protein composition, there are also significant differences in overall protein contents.

View larger version (41K): [in this window] [in a new window]   Fig. 2. Two-dimensional (2-D) gel electrophoresis analysis of proteins in the FcRI microdomains (A) or Thy-1 microdomains (B). After electrophoresis and transfer of proteins to nitrocellulose, blots were stained for total protein. Circles highlight unique protein spots in each of the two membranes. Results are representative of two separate experiments.

View larger version (33K): [in this window] [in a new window]   Fig. 3. Two-dimensional gel electrophoresis analysis of tyrosine-phosphorylated proteins in the FcRI microdomains (A) or Thy-1 microdomains (B). After electrophoresis and transfer of proteins to nitrocellulose, membranes were probed with HRP-conjugated anti-phosphotyrosine antibodies followed by ECL development. Circles in A highlight unique phosphoproteins in the FcRI microdomains. Stripped membranes were also probed with specific antibodies to the FcRI ß and subunits (side boxes), demonstrating that only FcRI micodomains contain IgE receptor subunits. Results are representative of two separate experiments.

Having established the complexity of the phospholipids isolated in the immunoisolated vesicles, we next performed normal-phase HPLC-MS/MS analyses to evaluate the relative abundances of the phospholipids in the two different microdomains (Fig. 4 ). There were no major differences in relative abundances of the GPC, GPS, or GPI molecular species between the FcRI and Thy-1 microdomains (data not shown). However, the HPLC-MS/MS analyses of GPE phospholipid species indicated significant differences between the two microdomains, particularly for the plasmenyl (plasmalogen) GPE species (Fig. 5 ). We used an isotope-tagged derivative to precisely determine relative differences in the molecular species between microdomain samples.

View larger version (20K): [in this window] [in a new window]   Fig. 4. Normal-phase HPLC-MS analysis of a sample of lipids from the IgE receptor microdomain, demonstrating sequential elution of cholesterol (and other neutral lipids) and glycerophosphoinositol (GPI), glycerophosphoethanolamine (GPE), glycerophosphoserine (GPS), and glycerophosphocholine (GPC) with sphingomyelin (SM). ESI, electrospray ionization.

View larger version (28K): [in this window] [in a new window]   Fig. 5. Positive ion ESI mass spectra from GPE of the FcRI microdomain (A) and the Thy-1 microdomain (B). m/z 720 corresponds to the 17:0/17:0 GPE internal standard (I.S.).

FcRI domains are enriched in GPE plasmalogens

View larger version (13K): [in this window] [in a new window]   Fig. 6. Use of iTRAQ reagent to compare the levels of diacyl and vinyl ether (plasmalogen) phospholipids in the FcRI and Thy-1 microdomains. GPEs in each of the sample preparations were isolated and modified with a distinct iTRAQ isotope tag, as described in Materials and Methods and outlined in supplementary Fig. II. Control samples were modified with the 115.1 tag, FcRI microdomains were modified with the 114.1 tag, and Thy-1 micodomains were modified with the 117.1 tag. Representative results of these analyses are shown for the relative abundance of the 36:2 diacyl species, the 38:4 diacyl species, the 34:1 plasmalogen species, and the 38:4 plasmalogen species. Rel. Int., relative intensity.

Analysis of all GPE molecular species measured using the isotope-tagging method revealed that plasmalogen GPE molecular species on average were 2.7 ± 0.8 times more abundant in the IgE receptor microdomains than in the Thy-1 microdomains (Fig. 7 ). Conversely, the diacyl GPE species were somewhat more abundant in the Thy-1 microdomains than in the IgE receptor microdomains.

View larger version (17K): [in this window] [in a new window]   Fig. 7. Summary of the levels of ester and vinyl ether phospholipids measured in two replicate experiments, expressed as a ratio of relative abundances normalized to the GPE internal standard (I.S.) in FcRI microdomains to those in Thy-1 microdomains.

View larger version (15K): [in this window] [in a new window]   Fig. 8. Measurements of total cholesterol/fatty acid content in FcRI and Thy-1 microdomains as well as in control samples. Results of four independent experiments are reported. Ab, antibody.

FcRI domains are enriched in sphingomyelin
The relative abundance of sphingomyelin lipids was also measured in the Thy-1 and FcRI samples (see supplementary Table II). All samples were normalized to internal standards, and values for three GPC molecular species are shown for comparison. As shown, all three major sphingomyelin molecular species were >2-fold more abundant in FcRI domains compared with Thy-1 domains. The 32:0e GPC was also enriched in FcRI microdomains. In contrast, the 34:1a and 32:1e GPC species were slightly more abundant in the Thy-1 microdomains.

	DISCUSSION

TOP ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
The rapidly advancing field of cellular lipidomics promises to shed light on the complexity and organization of the lipid bilayer (47). Here, sophisticated mass spectrometry techniques were used to analyze the lipid composition of immunoisolated membrane microdomains prepared in the absence of detergent. This is an important distinction, because previous attempts to further analyze the composition of the lipid environment of FcRI during the signaling process have been limited to the DRMs of RBL cells (38). The extent to which isolated DRMs reflect the composition of native membrane domains is debatable (15).

Protein analyses showed that membrane vesicles isolated using anti-IgE or anti-Thy1 were highly enriched in constituents that preferentially associate with each of these distinct signaling proteins. It is particularly remarkable to have such good separation of FcRI and Thy-1, because they are both exceptionally abundant constituents of RBL-2H3 membranes. There are 200,000 FcRI molecules and 1 million Thy-1 molecules per cell. Conditions were carefully chosen for cross-linking that favored the formation of very large rafts (300–500 nm in diameter) and minimized the presence of contaminating lipids in the much smaller (100 nm) vesicle preparations.

Cholesterol was found as the major lipid constituent of FcRI domains. On a molar ratio, it was roughly equivalent to the combined total of all of the fatty acids extracted from immunoisolated FcRI vesicles. In contrast, the relative concentrations of cholesterol to fatty acid in the Thy-1 domains were only 0.3–0.5. This may explain previous evidence for greater sensitivity of Thy-1-mediated mast cell activation to cholesterol depletion compared with that of FcRI activation (22). With lower starting levels of cholesterol, the Thy-1 domains might be expected to deplete faster and more completely during the initial exposure to methyl-ß-cyclodextrin (MßCD). An attractive alternative explanation is that the higher levels of sphingolipids, known to bind cholesterol, render FcRI domains partially resistant to cholesterol depletion. One role for cholesterol is likely to be its ability to promote the close packing of sphingolipid molecules (48), also found to be enriched in the FcRI domains. Intimate associations between FcRI and cell surface glycosphingolipids were suggested previously by the work of Pecht and colleagues (49) based upon monoclonal antibodies to mast cell glycosphingolipids that inhibit FcRI-mediated signaling. An early report by Rivnay and Fischer (50) also reported 2- to 5-fold enrichment of sphingomyelin in lipids bound tightly to receptor-IgE complexes.

Treatment of cells with agents that extract cholesterol, such as MßCD, reduces the recovery of raft components, disrupts caveolae, and prevents the formation of functional coated pits (reviewed in Ref. 51). In our experience, the total cholesterol in plasma membranes of cultured cells varies considerably. Fibroblast cell lines, for example, require significantly longer intervals and higher concentrations of MßCD for the depletion of cells loaded with [³H]cholesterol than do RBL cells (data not shown). Thus, it would be difficult to predict how well the exact ratios measured here would translate to receptors in other cell types. Nevertheless, the much higher concentration of cholesterol in FcRI domains provides unequivocal support for the hypothesis that the IgE receptor and Thy-1 occupy distinct lipid environments in native RBL membranes. A previous study in neuronal membranes found significant differences in lipid composition in immunoprecipitated DRMs of Thy-1 or the GPI-anchored prion protein (52). Compared with Thy-1, that study also found prion protein DRM preparations to have a higher concentration of cholesterol, slightly more unsaturated, longer chain lipids, and 5-fold higher levels of glycosylated hexosylceramide. Morris and colleagues (52) proposed that hydrogen bonding between carbohydrate moieties of glycolipids such as hexosylceramide might affect interactions with prion protein. This theory can obviously apply to many membrane glycoproteins that transiently associate with each other and with glycolipids through weak, noncovalent interactions. Interactions between transmembrane domains likely also influence lipid raft association. Thus, it seems clear that there are a number of mechanisms to explain the considerable heterogeneity in the lipids surrounding specific membrane proteins, regardless of their anchor.

Our analysis of GPE molecular species using isotope-tagged derivatization and nanospray MS³ detection revealed that FcRI microdomains were also enriched in GPE plasmalogen molecular species relative to the Thy-1 microdomains. Intriguingly, Pike, Han, and Gross (39) also found a relative enrichment in plasmalogens in lipid raft fractions, prepared with and without detergent, compared with postnuclear supernatants. It is worth noting that the vinyl ether linkage at the sn-1 position of GPE phospholipids introduces a double bond into the structure that is very near the lipid head group. It is tempting to speculate that this unique feature is preferentially favorable for association with some transmembrane receptors and/or their signaling partners. It is also interesting that the double bonds in GPE plasmalogens, sphingomyelins, and cholesterol are consistent with transmission electron microscopy images of dark patches surrounding aggregated IgE receptors. Sophisticated electron spectroscopy techniques demonstrated that dark patches concentrate osmium, which binds specifically to double bonds in lipids (34). These data suggest that sphingolipids, plasmalogens, and cholesterol are good candidates for the putative lipid shell that may surround some transmembrane receptors (53). Further work is needed to rigorously test this possibility.

Both domains isolated by immunoaffinity chromatography, rather than by sucrose density centrifugation, contain significant amounts of phosphatidylinositols. This is a notable distinction, because Pike, Han, and Gross (39) concluded that phosphatidylinositol appeared to be specifically excluded from raft preparations. Fridriksson et al. (38) did detect phosphatidylinositol in DRM fractions but failed to detect any polyphosphoinositol lipids. Our own study did not extend to the characterization of polyphosphoinositol species within FcRI domains. We expect that PtdIns(4,5)P₂ and PtdIns(3,4,5)P₃ are present, because our previous electron microscopy studies showed that receptor signaling patches specifically recruit phospholipase C , phosphatidylinositol 3-kinase, and phosphatase with tensin homology on chromosome 10 (36, 54). In addition to its role as substrate for PLC and phosphatidylinositol 3-kinase, PtdIns(4,5)P₂ is a critical factor for the recruitment and function of adaptor molecules involved in receptor endocytosis (5), which is initiated in FcRI signaling domains (36).

The method of purification used here does have an important limitation: it tracks the lipid environment surrounding activated FcRI receptors, because cross-linking and formation of large signaling patches was an essential feature of the protocol. Thus, evaluation of the local lipid environment for the resting receptor, where receptor clusters are limited to a few receptors and typically have diameters of <20–30 nm (35), remains a technically challenging prospect. It is clear from the work of Brown and colleagues (55, 56) that significant remodeling of lipids occurs during signal transduction. For example, B-cell receptor stimulation leads to significant decreases in overall phosphocholine, phosphatidylinositol, and phosphoethanolamine species and concomitant increases in lysophosphocholine, lysophosphatidylinositol, lysophosphoserine, and glycerophosphatidic acid compounds (56). Similar increases in lysophosphocholine were seen in RBL-2H3 cells within 5 min of antigen stimulation. Future work will explore the nanoscale compartmentalization of lipid components in membranes of both resting and activated cells and the dynamic events associated with localized lipid remodeling during the signaling process.

	ACKNOWLEDGMENTS

 
The authors thank Dr. Janet Oliver for valuable discussion and Janet Pfeiffer for technical assistance. This work was supported by National Institutes of Health Grants R01 AI-051575 (to B.S.W.) and U54 GM-069338 (to R.C.M.). The University of New Mexico Health Sciences Center Electron Microscopy Facility is gratefully acknowledged.

Manuscript received November 13, 2006 and in revised form March 15, 2007.

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