Large-scale fluid/fluid phase separation of proteins and lipids in giant plasma membrane vesicles.
ABSTRACT The membrane raft hypothesis postulates the existence of lipid bilayer membrane heterogeneities, or domains, supposed to be important for cellular function, including lateral sorting, signaling, and trafficking. Characterization of membrane lipid heterogeneities in live cells has been challenging in part because inhomogeneity has not usually been definable by optical microscopy. Model membrane systems, including giant unilamellar vesicles, allow optical fluorescence discrimination of coexisting lipid phase types, but thus far have focused on coexisting optically resolvable fluid phases in simple lipid mixtures. Here we demonstrate that giant plasma membrane vesicles (GPMVs) or blebs formed from the plasma membranes of cultured mammalian cells can also segregate into micrometer-scale fluid phase domains. Phase segregation temperatures are widely spread, with the vast majority of GPMVs found to form optically resolvable domains only at temperatures below approximately 25 degrees C. At 37 degrees C, these GPMV membranes are almost exclusively optically homogenous. At room temperature, we find diagnostic lipid phase fluorophore partitioning preferences in GPMVs analogous to the partitioning behavior now established in model membrane systems with liquid-ordered and liquid-disordered fluid phase coexistence. We image these GPMVs for direct visual characterization of protein partitioning between coexisting liquid-ordered-like and liquid-disordered-like membrane phases in the absence of detergent perturbation. For example, we find that the transmembrane IgE receptor FcepsilonRI preferentially segregates into liquid-disordered-like phases, and we report the partitioning of additional well known membrane associated proteins. Thus, GPMVs now provide an effective approach to characterize biological membrane heterogeneities.
- SourceAvailable from: Marion Jasnin[Show abstract] [Hide abstract]
ABSTRACT: Membrane pearling in live cells is observed when the plasma membrane is depleted of its support, the cortical actin network. Upon efficient depolymerization of actin, pearls of variable size are formed, which are connected by nanotubes of ∼40 nm diameter. We show that formation of the membrane tubes and their transition into chains of pearls do not require external tension, and that they neither depend on microtubule-based molecular motors nor pressure generated by myosin-II. Pearling thus differs from blebbing. The pearling state is stable as long as actin is prevented from polymerizing. When polymerization is restored, the pearls are retracted into the cell, indicating continuity of the membrane. Our data suggest that the alternation of pearls and strings is an energetically favored state of the unsupported plasma membrane, and that one of the functions of the actin cortex is to prevent the membrane from spontaneously assuming this configuration.Biophysical Journal 03/2014; 106(5):1079-1091. · 3.67 Impact Factor
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ABSTRACT: The influenza viral membrane protein hemagglutinin (HA) is required at high concentrations on virion and host-cell membranes for infectivity. Because the role of actin in membrane organization is not completely understood, we quantified the relationship between HA and host-cell actin at the nanoscale. Results obtained using superresolution fluorescence photoactivation localization microscopy (FPALM) in nonpolarized cells show that HA clusters colocalize with actin-rich membrane regions (ARMRs). Individual molecular trajectories in live cells indicate restricted HA mobility in ARMRs, and actin disruption caused specific changes to HA clustering. Surprisingly, the actin-binding protein cofilin was excluded from some regions within several hundred nanometers of HA clusters, suggesting that HA clusters or adjacent proteins within the same clusters influence local actin structure. Thus, with the use of imaging, we demonstrate a dynamic relationship between glycoprotein membrane organization and the actin cytoskeleton at the nanoscale.Biophysical Journal 05/2013; 104(10):2182-2192. · 3.67 Impact Factor
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ABSTRACT: There is growing recognition that lipid heterogeneities in cellular membranes play an important role in the distribution and functionality of membrane proteins. However, the detection and characterization of such heterogeneities at the cellular level remains challenging. Here we report on the poorly understood relationship between lipid bilayer asymmetry and membrane protein sequestering in raft-mimicking model membrane mixtures using a powerful experimental platform comprised of confocal spectroscopy XY-scan and photon-counting histogram analyses. This experimental approach is utilized to probe the domain-specific sequestering and oligomerization state of αvβ3 and α5β1 integrins in bilayers, which contain coexisting liquid-disordered/liquid-ordered (ld/lo) phase regions exclusively in the top leaflet of the bilayer (bottom leaflet contains ld phase). Comparison with previously reported integrin sequestering data in bilayer-spanning lo-ld phase separations demonstrates that bilayer asymmetry has a profound influence on αvβ3 and α5β1 sequestering behavior. For example, both integrins sequester preferentially to the lo phase in asymmetric bilayers, but to the ld phase in their symmetric counterparts. Furthermore, our data show that bilayer asymmetry significantly influences the role of native ligands in integrin sequestering.Biophysical Journal 05/2013; 104(10):2212-2221. · 3.67 Impact Factor
Large-scale fluid/fluid phase separation of proteins
and lipids in giant plasma membrane vesicles
Tobias Baumgart*, Adam T. Hammond†, Prabuddha Sengupta†, Samuel T. Hess‡, David A. Holowka†, Barbara A. Baird†,
and Watt W. Webb*§
*School of Applied and Engineering Physics and†Department of Chemistry and Chemical Biology, Cornell University, Ithaca, NY 14853; and
‡Department of Physics and Astronomy, University of Maine, Orono, ME 04469
Contributed by Watt W. Webb, December 26, 2006 (sent for review September 21, 2006)
The membrane raft hypothesis postulates the existence of lipid
bilayer membrane heterogeneities, or domains, supposed to be
important for cellular function, including lateral sorting, signaling,
and trafficking. Characterization of membrane lipid heterogene-
ities in live cells has been challenging in part because inhomoge-
neity has not usually been definable by optical microscopy. Model
membrane systems, including giant unilamellar vesicles, allow
optical fluorescence discrimination of coexisting lipid phase types,
but thus far have focused on coexisting optically resolvable fluid
phases in simple lipid mixtures. Here we demonstrate that giant
plasma membrane vesicles (GPMVs) or blebs formed from the
into micrometer-scale fluid phase domains. Phase segregation
temperatures are widely spread, with the vast majority of GPMVs
found to form optically resolvable domains only at temperatures
below ?25°C. At 37°C, these GPMV membranes are almost exclu-
sively optically homogenous. At room temperature, we find diag-
nostic lipid phase fluorophore partitioning preferences in GPMVs
analogous to the partitioning behavior now established in model
membrane systems with liquid-ordered and liquid-disordered fluid
phase coexistence. We image these GPMVs for direct visual char-
acterization of protein partitioning between coexisting liquid-
ordered-like and liquid-disordered-like membrane phases in the
absence of detergent perturbation. For example, we find that the
transmembrane IgE receptor Fc?RI preferentially segregates into
liquid-disordered-like phases, and we report the partitioning of
additional well known membrane associated proteins. Thus,
GPMVs now provide an effective approach to characterize biolog-
ical membrane heterogeneities.
liquid-disordered ? liquid-ordered ? membrane domains ?
membrane heterogeneity ? rafts
dynamic sorting and signaling platforms for membrane proteins
(1). Consensus data on the size, lifetime, and even existence of
lipid rafts in intact plasma membranes, however, have been
elusive (2, 3). Controversy arises due to current experimental
ambiguity and to operational definitions of membrane lipid
One common definition has relied on biochemical assessment
of membrane heterogeneity involving membrane lysis using
certain nonionic detergents, such as Triton X-100 at 4°C (4). A
second, operational definition for lipid rafts has been cellular
processes that are perturbed by either cholesterol or sphingo-
myelin depletion. Problems of these approaches have been
extensively discussed (2, 3).
The reports that membranes composed of lipids that are
resistant to detergent solubilization are apparently in a liquid-
ordered (Lo) state (5–7) have been the basis for proposing that
lipid rafts in plasma membranes represent the Lo phase of
coexisting Loand liquid-disordered (Ld) fluid/fluid phases (2, 8).
Biological membrane heterogeneity, however, cannot be re-
duced to partitioning between coexisting lipid domains, because
he membrane raft hypothesis proposes that membrane lipid
domains enriched in cholesterol and sphingolipids form
reciprocal protein–lipid, as well as protein–protein interactions
necessarily modulate the thermodynamics of lipid heterogeneity
(2, 9, 10), emphasizing the need for examining membranes with
significant protein content, as suggested by protein segregation
measurements on living cells (11).
Several studies have suggested the existence of membrane
heterogeneities with size scales below optical resolution (?300
nanometers), but estimates of lipid raft sizes in the literature
range from several micrometers, as in cholesterol-depleted cells
(12), to just a few molecules (13). Fluid/fluid phase separation
in biological cell membranes has thus far not been unequivocally
demonstrated in live cells, perhaps because coupling of the
plasma membrane to the underlying cytoskeleton may prevent
fluid phase segregation into distinctive domains, as can be
observed in lipid-only model membranes with appropriate com-
positions. Differences from model membranes could arise from
the pinning of plasma membrane domains by cytoskeleton-
attached, membrane-associated proteins or from complex mem-
brane rugosities induced by protein–protein interactions. Fur-
thermore, the enormous complexity of cellular plasma
membrane protein and lipid compositions might preclude the
simple fluid/fluid phase separations observed in ternary lipid
To investigate fluid/fluid phase coexistence in systems with
realistic biological membrane compositions, we here use giant
plasma membrane vesicles (GPMVs) that are derived from
biological cells, RBL mast cells, and fibroblasts by chemically
induced plasma membrane vesiculation or ‘‘blebbing’’ (15–17).
These GPMVs show simple, low-curvature geometries of giant
unilamellar vesicles and appear free of cytoskeletal constraints.
By using fluorophores providing recently characterized mem-
brane fluid phase partitioning behavior (T.B., G. Hunt, E. R.
Farkas, W.W.W., and G. W. Feigenson, unpublished data) for
lipid phase characterization here, we find that these GPMVs can
segregate into multi-micrometer-scale coexisting fluid phases,
thereby enabling extension of early cell blebbing studies in our
laboratories in the 1980s (15, 18–20). These results are noted and
used throughout this paper.
In initial experiments to study phase separation in plasma
membrane-derived, micrometer-scale vesicles, mammalian cells
Author contributions: T.B., S.T.H., and W.W.W. initiated research; T.B. P.S., S.T.H., and
A.T.H. performed research; T.B., A.T.H., P.S., S.T.H., D.A.H., and B.A.B. analyzed data;
and T.B., D.A.H., B.A.B., and W.W.W. wrote the paper.
The authors declare no conflict of interest.
Abbreviations: CM, laser scanning confocal microscopy; CTB, cholera toxin subunit B;
GPMV, giant plasma membrane vesicle; GUV, giant unilamellar vesicle; Ld, liquid-disor-
dered; Lo, liquid-ordered; Nap, naphthopyrene; R-DOPE, rhodamine B sulfonyl dioleoyl
§To whom correspondence should be addressed at: Cornell University, 212 Clark Hall,
Ithaca, NY 14853. E-mail: email@example.com.
This article contains supporting information online at www.pnas.org/cgi/content/full/
© 2007 by The National Academy of Sciences of the USA
February 27, 2007 ?
vol. 104 ?
no. 9 ?
were treated with combinations of polar organic solvents to
induce GPMV formation and selected membrane dyes to label
lipid phases. Fig. 1 illustrates typical fluorescence-labeled cell-
attached GPMVs imaged by stacks of laser scanning confocal
microscopy (CM) or two-photon microscopy sections. The
GPMV in Fig. 1A was induced by addition of 4% (vol/vol)
ethanol to suspended RBL cells, and GPMV in Fig. 1B was
induced by addition of DMSO (1% vol/vol) to adherent fibro-
blasts. Under these conditions, substantial membrane dye is
rapidly internalized, delivering fluorescence to the cell body, as
illustrated in Fig. 1 A, C, and D. These GPMVs, having dimen-
sions comparable to cell sizes, occur in low fractions (?5%) of
treated cells and are possibly induced by transient, local high
solvent concentration during solvent injections into the sur-
rounding buffer. The cell-attached GPMV on an RBL cell in Fig.
1A was prelabeled by the plasma membrane inner-leaflet-
targeted protein, geranylgeranyl-EGFP (21), and it shows a
homogenous membrane bilayer at optical resolution when im-
aged at room temperature. Fig. 1B shows a lipid phase-separated
GPMV from NIH 3T3 fibroblasts labeled with lissamine rhoda-
mine B sulfonyl dioleoyl phosphatidyl ethanolamine (R-DOPE)
to demonstrate that plasma membrane fluid/fluid phase sepa-
ration at room temperature is not a unique property of GPMVs
obtained from RBL mast cells.
At temperatures of 4–10°C, cell-attached GPMV membranes
often separate into two distinct phases, as shown by the con-
and R-DOPE in Fig. 1D. That these coexisting domains are in
fluid phase states at 4°C is indicated by frequent coalescence
activity and circular morphology. The fluid phase separations
shown in Fig. 1 C and D, as well as all other phase-separated
GPMVs examined here, show only two different fluorescence
intensities, suggesting that the lipid domains are coupled across
the bilayer, as previously observed for inner- and outer-leaflet-
labeled domain registration in phase-separated model mem-
brane giant unilamellar vesicles (GUVs) (22).
Nap preferentially labels the Lo phase in model membranes
containing ternary lipid mixtures of brain sphingomyelin, dioleoyl
phosphatidylcholine, and cholesterol, whereas R-DOPE strongly
of differing lipid compositions (T.B., G. Hunt, E. R. Farkas,
W.W.W., and G. W. Feigenson, unpublished data). Thus, GPMVs
from RBL cells appear to phase-separate into coexisting fluid
membrane phases with Lo-like and Ld-like phase states. Because
membrane phase behavior is likely to be modified in the presence
of organic solvents, we also developed alternative protocols for
GPMV formation and membrane staining.
Membrane blebbing induced by chemical methods that modify
amino and sulfhydryl groups (15, 17, 23) allows isolating large
numbers of GPMVs from adhering cells for characterization (15,
24). GPMVs isolated after treatment of RBL mast cells with 25
mM formaldehyde, together with 2 mM DTT, or by treatment
with 2 mM N-ethylmaleimide for 1 h at 37°C phase separate in
a temperature-dependent manner. Representative low-
magnification views of cell-free GPMVs isolated after formal-
dehyde/DTT treatment and labeled with the Ldphase-preferring
fluorescent phospholipid R-DOPE were imaged at three differ-
ent temperatures [supporting information (SI) Fig. 4]. At 5°C,
essentially all vesicles phase separate (SI Fig. 4A), but at room
temperature only ?10–25% of all vesicles show large-scale
fluid/fluid phase coexistence (SI Fig. 4B). At 37°C, fluid phase
coexistence is rare: ?1% of all imaged GPMVs show optically
resolvable domains. One of these exceptional cases is depicted in
SI Fig. 4C Inset. The large variation in phase separation observed
in different vesicles, especially at intermediate temperatures,
may indicate compositional variations among GPMVs in these
Fig. 2 compares the fluid-phase partitioning behavior of
several lipid analogues (Nap, R-DOPE, and DiI C16:0) and
lipid-binding proteins [cholera toxin subunit B (CTB) and
annexin V] in cell-free GPMVs imaged at room temperature
(Fig. 2 A–C) and at 12°C (Fig. 2D). Nap and R-DOPE show
contrasting partitioning in coexisting fluid phases, both at room
temperature as shown in Fig. 2A and at 5°C (Fig. 1 C and D). Fig.
2B shows that CTB bound to the ganglioside GM1partitions into
membrane regions complementary to those labeled with Ld-
preferring R-DOPE. CTB is frequently used as a marker for
cellular lipid rafts and caveolae based on sucrose gradient
fractionation experiments (25), and GUV model membrane
studies have shown that fluorescent CTB bound to GM1pref-
erentially labels Lophases that are coexisting with Ldphases (26,
27). Partitioning of CTB bound to GM1, in contrast to DiI C16:0,
indicates that DiI preferentially partitions into the Ld-like phase
(Fig. 2C). Although DiI C16:0 is deemed a marker for lipid rafts
on cells (12, 28, 29), it has been observed to partition preferen-
tially into Ld phases in selected ternary mixtures of brain
sphingomyelin/dioleoyl phosphatidylcholine/cholesterol and in
mixtures of distearoyl phosphatidylcholine/dioleoyl phosphati-
dylcholine/cholesterol (data not shown).
We compared the partitioning of CTB bound to GM1with
fluorescent annexin V, which binds phosphatidylserine (PS) in a
calcium-dependent manner (30). Annexin V is an indicator of
transbilayer flipping of the negatively charged PS that is a
hallmark of cellular apoptosis (31). In phase-separated GPMVs,
annexin V labeling is in contrast to Lo-like domains that are
preferentially labeled with fluorescent CTB (Fig. 2D). This
indicates that PS, and possibly other negatively charged phos-
pholipids, partition preferentially into more disordered regions
with fluorescent CTB and annexin V derivatives is similar to
lipid-bound fluorophores (R-DOPE, DiIC16:0, and Nap) ex-
cludes the possibility that the fluid phase segregation we detect
is due to membrane insertion of fluorescent lipids or to photo-
decomposition products of membrane-embedded fluorophores.
phases. (A, C, and D) RBL cells treated with 4% (vol/vol) ethanol. Cells con-
taining fluorescent membrane probes show formation of large GMPVs at-
tached to the cell bodies by superposition of CM or two-photon microscopy
image z-stacks. (A) Cell expressing geranylgeranyl-EGFP (GG-GFP) with at-
tached GPMV measured by CM-imaged stack at ?23°C. Note the absence of
internal membranes within the GPMV and significant partitioning of GG-GFP
into the GPMV compared with the cell body structures. (B) CM images of an
NIH 3T3 GPMV incubated at room temperature with 1% (vol/vol) DMSO and
R-DOPE, showing large-scale fluid/fluid phase coexistence similar to the RBL
cells. (C and D) Two-photon microscopy images of a cell-attached GPMV
Note their contrasting wavelength-selected labeling of the separated phases.
Cell bodies show large fluorescence (attenuated here) due to internalized
membrane probes. (Scale bars, 5 ?m.)
Cell-attached GPMVs can laterally segregate into coexisting fluid
www.pnas.org?cgi?doi?10.1073?pnas.0611357104Baumgart et al.
Photoinduced lipid oxidation, which can interfere with mem-
brane phase behavior (32), was minimized by the antioxidant
As seen by CM, soluble fluorescently labeled proteins, such as
CTB and annexin V, are mostly excluded from the interior of
GPMVs, suggesting that their membranes are sufficiently sealed
to prevent internalization of protein-sized solutes. However,
some GPMVs are slightly leaky to these proteins, as judged by
the occasional observation of slow internal labeling of GPMVs
(data not shown). Nevertheless, determining whether fluores-
to the outer leaflet or on the inner leaflet of these GPMVs is
uncertain. Earlier experiments on formaldehyde induced plasma
membrane vesicles of neuroblastoma cells indicated partial
retention of lipid asymmetry for as long as 3 days after blebbing
that GPMVs may retain significant leaflet asymmetry during our
imaging, but it remains for future studies to determine the extent
of lipid asymmetry preservation in GPMVs.
An advantage of GPMVs is that membrane protein partition-
ing can be reliably studied by optical microscopy in vesicles with
clearly identified fluid/fluid phase coexistence. Fig. 3 demon-
strates selective partitioning of lipid-anchored proteins from
outer and inner leaflets of cellular plasma membranes, as well as
phatidylinositol-anchored proteins, including Thy-1, are com-
mon markers for outer leaflets of lipid rafts, based on detergent
fractionation, (34, 35), intact cell membrane (36, 37), and model
membrane studies (38). Fig. 3A shows Thy-1 labeled with
Cy3-conjugated Ox7 mAb partitioning preferentially into the
Lo-like phase in GPMVs with fluid/fluid phase coexistence. In
contrast, several lipid-anchored proteins that localize to the
inner leaflet of the plasma membrane were found to partition
preferentially into the Ld-like phase.
Fig. 3B shows that Lyn-GFP, which reconstitutes Fc?RI-
mediated signaling (39, 40), partitions preferentially into the Ld
phase of GPMVs. However, several sucrose gradient analysis
studies had suggested that Lyn itself preferentially associates
with ‘‘lipid rafts’’ under a variety of cell lysis conditions (39, 41,
42). Similarly, the GFP chimera PM-GFP, which is anchored to
the plasma membrane inner leaflet by myristate and palmitate
acyl chains attached to the first 20 amino acid residues of Lyn
(21), preferentially partitions into the Ld-like phase in GPMVs
(Fig. 3C), and a geranylgeranyl-anchored chimera of GFP (21)
similarly partitions into Ld-like phases (Fig. 3D). Sucrose gra-
dient fractionation of detergent-lysed cells suggests that the GFP
module enhances Ldpartitioning (39). However, the strong Ld
partitioning observed with these inner-leaflet lipid-anchored
proteins in GPMVs represents a significant quantitative differ-
ence from detergent fractionation predictions.
We find that A488-labeled IgE bound to Fc?RI strongly
partitions into the Ld-like phase of GPMVs, as shown in Fig. 3E.
These results are consistent with those obtained from sucrose
gradient analysis of TX-100-lysed RBL cells over a large range
of detergent concentrations (41, 43, 44). Cross-linking of this
IgE-receptor complex has been shown to substantially increase
its partitioning into detergent-resistant lipid rafts (41), and it will
be interesting to investigate the effects of Fc?RI cross-linking on
its phase partitioning in GPMVs.
Fig. 3F shows that the FITC-conjugated lectin, Con A, which
binds to a large number of ?-methyl mannoside-containing
glycoproteins and glycolipids, preferentially partitions into the
Ld-like phase as well, as evidenced by colabeling with R-DOPE.
Comparison of the fluorescence intensity of FITC-Con A label-
ing of two GPMVs attached to a cell in Fig. 3G shows that the
glycoproteins and glycolipids that segregate into the emerging
GPMVs represent a substantial fraction of the Con A binding
protein content versus cellular membrane protein content is
uncertain because of the highly folded nature of the cellular
membrane, compared with the smooth bleb membranes.
GUV model membranes enable examination of mechanical
aspects of membranes with fluid/fluid phase coexistence, in-
cluding curvature coupling to membrane phase patterns and line
tension at phase boundaries (14, 45–47), as well as experimental
tests of mechanical membrane theories (14, 48). GUVs with
Lo/Ld phase coexistence and relatively monodisperse domain
sizes show hexagonal arrays of phase domains in superstructures
that are reminiscent of modulated phase separation patterns
observed in many other physical systems (49). SI Fig. 5A
illustrates the hexagonally modulated phase patterns that also
are occasionally observed in GPMVs. Modulated phase patterns
can be stabilized by competing short-range attractive and long-
range repulsive forces, and model membrane systems have
indicated compositional variations arising from short-range at-
tractions that couple to membrane curvature modulations, pos-
sibly leading to long-range repulsion (14, 49). These modulated
patterns are likely to be kinetically trapped nonequilibrium
structures subject to domain coalescence and possibly other
coarsening mechanisms (50) due to line tension at phase bound-
aries typically leading to complete phase separation after long
strating characteristic phase preferences resembling the Lo/Ldpartitioning
behavior in model membranes. GPMVs, all prepared by formaldehyde/DTT
treatment of RBL cells, were colabeled by Nap, R-DOPE, or DiIC16 and by
A488-CTB bound to GM1or A568-annexin V bound to phosphatidylserine.
Images are equatorial CM sections obtained at ?23°C. (A) GPMVs colabeled
with Nap and R-DOPE show contrasting partitioning. (B) GPMVs colabeled
with CTB and R-DOPE show contrasting partitioning. (C) GPMVs
colabeled with CTB and DiI C16:0 show contrasting partitioning. (D) CTB/
annexin V-colabeled GPMV shows contrasting partitioning, indicating that
annexin V labels an Ld-like phase.
Plasma membrane lipids and lipid fluorophores in GPMVs demon-
Baumgart et al. PNAS ?
February 27, 2007 ?
vol. 104 ?
no. 9 ?
Although domains of our phase-separated GPMVs show small
curvature gradients, i.e., the membrane geometries approach
circular domains on a smooth sphere, a notable exception is
GPMVs with small domains that are labeled with CTB, as seen
Lo-like domains develop significant inward curvature. Interest-
ingly, internalization of CTB bound to GM1occurs in cells in a
cholesterol-dependent fashion (51), and it is possible that CTB
promotes internalization by inducing a spontaneous inward
curvature that facilitates budding and fission. Similar inward
curvature is occasionally observed for CTB-labeled Lodomains
in GUV model membranes (A.T.H., unpublished data).
Occasionally, phase-separated GPMVs show domain shapes
fluctuating via in-plane domain boundary undulations. SI Fig.
5C shows sequential images of a vesicle at 23°C with domain
undulations. These two-dimensional undulations also are ob-
served in GUV model membranes with fluid/fluid phase coex-
istence near mixing/demixing transition temperatures, where
line tension can become relatively small (14, 45). These undu-
lations further highlight the presence of fluid/fluid phase coex-
istence in GPMVs. Fluid phase coexistence also is supported by
fast recovery of spot photobleaching of all labeled lipids and
membrane proteins examined here (data not shown).
Plasma membrane vesicles, commonly called blebs, are naturally
formed in a variety of physiological processes that include
blebbing in locomoting cells, in cells undergoing mitosis, and in
apoptotic cells. Bleb formation can be artificially induced by a
variety of methods (52), including our addition of solvents or
sulfhydryl group-blocking reagents. Depending on the method,
different types of blebs can be obtained (52, 53). Ours were
formed through cell swelling and blebbing, as in oncosis (53).
These blebs have been shown to be free of cellular organelles,
with lipid compositions representative of the plasma membrane,
with phospholipid/cholesterol ratios of ?2:1 (6, 16, 24). Our
GPMVs from RBL cells contain constitutively active tyrosine
kinase Lyn (N. Smith, D.A.H., and B.A.B., unpublished data).
A possible question is the cellular source of GPMV mem-
branes, considering the apparent increased plasma membrane
area during blebbing (see Figs. 1 and 3G). Membrane capaci-
tance measurements via patch-clamping of mast cells have
revealed that osmotic inflation of cells by approximately 4 times
the resting volume did not change membrane conductance and
only caused small reversible changes of total cell membrane
capacitance (54). These results combined with the finding of
exocytosis inhibition by inflation (54) suggest that GPMV mem-
branes are likely to accrue from excess membrane area stored in
membrane microvilli and various protrusions including coated
pits, lamellipodia, and ruffles, but more direct comparisons are
The overall protein content of GPMVs must influence
membrane phase behavior. GPMVs from RBL cells have been
reported to contain ?20–25% of the cellular IgE-receptor
complexes (15), roughly comparable with the apparent frac-
tion of cellular plasma membrane extruded as GPMV. This
conclusion is supported by abundant Con A labeling via their
glycosylated protein binding sites retained in cell-attached
GPMVs (Fig. 3G) and by recent ESR measurements that
provided evidence for similar phase coexistence behavior in
GPMV and in living cell plasma membranes (55). Earlier
IgE-receptor diffusion measurements have indicated signifi-
cant mobility increase due to observed reductions of molecular
crowding relative to cell membranes on hypertonically swollen
cells and chemically induced membrane blebs (56, 57). Exten-
sive experiments will be required to establish the important
relations between membrane phases and protein contents. We
find that the F-actin probe Alexa Fluor 488 phalloidin does
free GPMVs. Fluorescence images of equatorial confocal sections through
GPMVs comparing the fluid phase partitioning of membrane-associated pro-
teins (left column) to the lipid probes R-DOPE and CTB bound to GM1(right
column). All GPMVs were prepared by formaldehyde/DTT treatment of RBL
cells and imaged at ?23°C. (A) GPI-anchored protein Thy-1 labeled with
A488-anti-Thy1 mAb is preferentially in Lophase, showing fluorescence in
regions contrasting to R-DOPE partitioning in the Ld-like phase. (B) Lyn-GFP
partitions preferentially into the Ld-like phase, in contrast with the CTB-
labeled Lo-like phase. (C) PM-GFP partitions strongly into the Ld-like phase, in
contrast to the CTB-enriched phase, in a cell-attached GPMV. (D) GG-GFP
partitions preferentially into the Ld-like phase, complementary to CTB. (E)
Fc?RI labeled with A488-IgE partitions into the Ld-like phase colabeled with
cosegregate with the Ldphase marker R-DOPE. (G) A significant fraction of
Con A receptors populate GPMVs, compared with those in the attached cell.
(Scale bar, 5 ?m.)
GPMVs reveal membrane protein phase preferences in detergent-
www.pnas.org?cgi?doi?10.1073?pnas.0611357104Baumgart et al.
penetrate the membranes and uniformly stains the volume of
the GPMV plus the actin cytoskeleton in the residual cell body
(data not shown), confirming the absence of a cortical actin
assembly on GPMVs, as shown previously by electron micros-
copy (23) and flourescence microscopy (20). This uncoupling
from the cortex is likely to be critical for the observed
membrane phase separations. Polyphosphoinositide lipids (24,
58) and cytoskeletally immobilized proteins may be excluded
from GPMVs (59, 60), a future question that needs to be
Important results of this study are the defined mixing/
demixing transition temperatures in the protein-containing
membranes of individual GPMVs. The significant temperature
dependence of plasma membrane phase behavior also has
been demonstrated recently by photobleaching recovery mea-
surements (61). We find that individual vesicles show large
variations in transition temperatures, with the vast majority of
vesicles undergoing phase separations only at temperatures
between ?10°C and 25°C. These low-temperature phase sep-
arations are defined by the coexistence of two fluid membrane
phases with sharp phase boundaries at optical resolution. Two
distinct fluid phases do form despite the complex GPMV
membrane composition, relative to simple ternary lipid mix-
tures of model membranes with composition-dependent fluid-
phase-coexistence temperatures (38, 45, 47). Coexisting fluid
membrane phases in GPMVs show fluorescence probe parti-
tioning behavior similar to model membranes with Lo/Ldphase
Demixing phase separations, particularly in binary or ternary
systems, can be considered in regular solution theory, where an
enthalpic term due to preferential molecular interactions balances
against the entropic contribution proportional to temperature to
determine the free energy change of mixing. Highly preferential
interactions lead to lower demixing temperatures. Local concen-
tration fluctuations associated with nonideal mixing (62) may
diverge on approaching critical (consolute) points of multicompo-
nent phase diagrams (63). Our finding of Lo/Ld-like phase separa-
tion only below physiological temperatures suggests correlated
concentration fluctuations above the demixing temperatures that
may lead to local composition fluctuations amenable to protein
interactions. Correlated concentration fluctuations in native, mac-
roscopically homogenous plasma membranes could yield an in-
creased encounter probability of signaling molecules with similar
membrane phase preference and, likewise, decreased encounter
probabilities of signaling components with differing phase prefer-
ences. Our experiments do not yet include lifetimes or length scales
of such composition fluctuations.
The large-scale development of membrane phase domains is
driven by the interphase energy of the phase boundaries.
Whereas this line tension at fluid phase boundaries can be
substantial in lipid model membrane systems (14), line tension
magnitudes could differ significantly and be much smaller in
more complex membrane compositions, possibly favoring small-
scale cell membrane heterogeneities (64), because line tensions
are generally reduced significantly by solute segregation to the
In summary, we find that GPMVs from RBL mast cells
undergo fluid phase segregation that permits the characteriza-
tion of lipid and protein partitioning in complex biological
membranes. These GPMVs, which contain integral and periph-
eral membrane proteins and hundreds of different lipids, seg-
regate into Lo/Ld-like fluid membrane phases at low tempera-
tures, indicating nonideal, nonrandom lateral distributions of
membrane components and permitting determination of mem-
brane phase preferences of labeled lipids and of membrane
proteins. The high-affinity IgE receptor partitions into Ld-like
and CTB bound to GM1segregate into Lo-like phases. Several
acyl-chain-anchored, GFP-labeled proteins, including palmitoyl/
myristoyl-anchored Lyn, partition preferentially to Ld-like (i.e.,
‘‘non-raft’’) phases in GMPVs, in contrast to their reported
association with detergent-resistant membrane particles, that
have been hypothesized to represent ‘‘rafts.’’ These inner-leaflet
acyl-chain-anchored proteins may be affected by changes in lipid
asymmetry during the formation of GPMVs.
Our method avoids membrane disruption by detergent treat-
ment or depletion of membranes of cholesterol or sphingomy-
elin. The approach is suitable for examining the distribution of
lipids and proteins between membrane domains and therefore
allows testing predictions from the raft hypothesis in laterally
intact cellular bilayer membranes. Our results present clear
evidence that these complex biological cell plasma membranes
can phase segregate into coexisting fluid phases but primarily at
of this segregation is consistent with expectations from model
membrane studies and implies that, at temperatures above the
demixing transition temperature, diffusing membrane hetero-
geneities may persist. Further investigation will be necessary to
clarify the differences between GPMV and cellular plasma
membranes in temperature-dependent phase behavior. Future
studies can use GPMVs to examine the dependence of mem-
brane protein phase partitioning on biochemical activities, in-
cluding the regulation of membrane-associated kinases and
phosphatases in cell signaling.
Materials and Methods
For lipid probes, antibodies, GFP constructs, cell culture and trans-
fection, and imaging methods, see SI Materials and Methods.
GPMV Formation. GPMVs were formed by three different meth-
ods aimed to produce either cell-attached or free GPMVs of
RBL cell plasma membranes.
Cell-attached GPMVs. Cell-attached GPMVs were prepared by
addition of 1–5% (vol/vol) ethanol, acetone, or DMSO to RBL
cells suspended at 106cells per milliliter in PBS for 15 min at
room temperature (23°C) or by addition of solvents to adherent
NIH 3T3 cells in four-well plates. Solvents used to induce
membrane vesiculation typically contained R-DOPE or
DiIC16:0 at 200 ?g/ml or Nap at 50 ?g/ml.
Cell-Free GPMVs. Cell-free GPMVs were prepared by either of the
two following methods. The primary protocol for GPMV for-
mation used a procedure modified from Scott (16, 17) and
described in ref. 15. Briefly, cells were grown to confluency in a
25-cm2tissue culture flask, then cells were washed twice with
and ?1.5 ml of freshly prepared GPMV reagent was added,
consisting of 25 mM formaldehyde and 2 mM DTT in GPMV
buffer. The flasks were then incubated for 1 h at 37°C while
slowly shaking (60–80 cycles per minute). After incubation,
GPMVs that had detached from the cells were gently decanted
into a conical tube. Previously published protocols (15) further
purified the vesicles by centrifugation and dialysis, but we found
that these procedures caused fragmentation of large GPMVs,
making microscopic analysis difficult. For the present experi-
ments, we allowed GPMVs to settle on ice for 10- 45 min and
collected them by removing ?20% of the total volume from the
bottom of the tube. By using this method, a single confluent
25-cm2flask yields sufficient GPMVs to create several dozen
by 2 mM N-ethylmaleimide, a reagent previously shown to cause
GPMV formation (17). All other steps are identical. The yield of
GPMV is lower, and more cells detach under these conditions.
Therefore, this protocol was used primarily to verify that the small
amount of formaldehyde and DTT present in the primary method
did not affect the results obtained.
Baumgart et al. PNAS ?
February 27, 2007 ?
vol. 104 ?
no. 9 ?
This work was supported by Science and Technology Centers Program
Agreement ECS-9876771 from the Nanobiotechnology Center of
the National Science Foundation and by National Institute of Al-
lergy and Infectious Diseases Grant R01 AI18603 and National
Institute of Biomedical Imaging and Biotechnology Grant P41
1. Simons K, Ikonen E (1997) Nature 387:569–572.
2. Edidin M (2003) Ann Rev Biophys Biomol Struct 32:257–283.
3. Munro S (2003) Cell 115:377–388.
4. Brown D, Rose J (1992) Cell 68:533–544.
5. Schroeder R, London E, Brown D (1994) Proc Natl Acad Sci USA 91:12130–
6. Gidwani A, Holowka D, Baird B (2001) Biochemistry 40:12422–12429.
7. Ge MT, Gidwani A, Brown HA, Holowka D, Baird B, Freed JH (2003) Biophys
8. London E (2002) Curr Opin Struct Biol 12:480–486.
9. Anderson RGW, Jacobson K (2002) Science 296:1821–1825.
10. Engelman DM (2005) Nature 438:578–580.
11. Ryan TA, Myers J, Holowka D, Baird B, Webb WW (1988) Science 239:61–64.
12. Hao MM, Mukherjee S, Maxfield FR (2001) Proc Natl Acad Sci USA
13. Mayor S, Rao M (2004) Traffic 5:231–240.
14. Baumgart T, Hess ST, Webb WW (2003) Nature 425:821–824.
15. Holowka D, Baird B (1983) Biochemistry 22:3466.
16. Scott R, Maercklein P (1979) J Cell Sci 35:245–252.
17. Scott RE (1976) Science 194:743–745.
18. Wu ES, Tank DW, Webb WW (1982) Proc Natl Acad Sci USA 79:4962–4966.
19. Tank DW, Wu ES, Webb WW (1982) J Cell Biol 92:207–212.
20. Barak LS, Webb WW (1982) J Cell Biol 95:846–852.
21. Pyenta PS, Holowka D, Baird B (2001) Biophys J 80:2120–2132.
22. Korlach J, Schwille P, Webb WW, Feigenson GW (1999) Proc Natl Acad Sci
23. Scott R, Perkins R, Zschunke M, Hoerl B, Maercklein P (1979) J Cell Sci
24. Fridriksson EK, Shipkova PA, Sheets E, Holowka D, Baird BA, McLafferty
FM (1999) Biochemistry 38:8056–8063.
25. Parton RG, Richards AA (2003) Traffic 2003:724–738.
26. Kahya N, Scherfeld D, Bacia K, Poolman B, Schwille P (2003) J Biol Chem
27. Hammond AT, Heberle FA, Baumgart T, Holowka D, Baird B, Feigenson GW
(2005) Proc Natl Acad Sci USA 102:6320–6325.
28. Thomas J, Holowka D, Baird B, Webb W (1994) J Cell Biol 125:795–802.
29. Pierini L, Holowka D, Baird B (1996) J Cell Biol 134:1427–1439.
30. Gerke V, Creutz CE, Moss SE (2005) Nat Rev Mol Cell Biol 6:449–461.
31. Sims PJ, Wiedmer T (2001) Thromb Haemost 86:266–275.
32. Ayuyan AG, Cohen FS (2006) Biophys J 91:2172–2183.
33. Yavin E, Zutra A (1979) Biochim Biophys Acta 553:424–437.
34. Brown DA, London E (2000) J Biol Chem 275:17221–17224.
35. Sheets ED, Holowka D, Baird B (1999) J Cell Biol 145:877–887.
36. Varma R, Mayor S (1998) Nature 394:798–801.
37. Friedrichson T, Kurzchalia TV (1998) Nature 394:802–805.
38. Dietrich C, Bagatolli LA, Volovyk ZN, Thompson NL, Levi M, Jacobson K,
Gratton E (2001) Biophys J 80:1417–1428.
39. Kovarova M, Tolar P, Arudchandran R, Draberova L, Rivera J, Draber P
(2001) Mol Cell Biol 21:8318–8328.
40. Larson DR, Gosse JA, Holowka DA, Baird BA, Webb WW (2005) J Cell Biol
41. Field KA, Holowka D, Baird B (1995) Proc Natl Acad Sci USA 92:9201–9205.
42. Young RM, Holowka D, Baird B (2003) J Biol Chem 278:20746–20752.
43. Field K, Holowka D, Baird B (1997) J Biol Chem 272:4276–4280.
44. Field K, Holowka D, Baird B (1999) J Biol Chem 274:1753–1758.
45. Veatch SL, Keller SL (2003) Biophys J 85:3074–3083.
46. Staneva G, Angelova MI, Koumanov K (2004) Chem Phys Lipids 129:53–62.
47. Bacia K, Schwille P, Kurzchalia T (2005) Proc Natl Acad Sci USA 102:3272–
48. Baumgart T, Das S, Webb WW, Jenkins JT (2005) Biophys J 89:1067–1080.
49. Seul M, Andelman D (1995) Science 267:476–483.
50. Samsonov AV, Mihalyov I, Cohen FS (2001) Biophys J 81:1486–1500.
51. Sharma P, Sabharanjak S, Mayor S (2002) Cell Dev Biol 13:205–214.
52. Keller H, Rentsch P, Hagmann J (2002) Exp Cell Res 277:161–172.
of Apoptosis and Programmed Cell Death, eds Lockshin R, Zakeri Z, Tilly JL
(Wiley–Liss, New York), pp 57–96.
54. Solsona C, Innocenti B, Fernandez JM (1998) Biophys J 74:1061–1073.
55. Swamy MJ, Ciani L, Ge MT, Smith AK, Holowka D, Baird B, Freed JH (2006)
Biophys J 90:4452–4465.
56. Thomas JL, Feder TJ, Webb WW (1992) Biophys J 61:1402–1412.
58. Hagelberg C, Allan D (1990) Biochem J 271:831–834.
59. Menon AK, Holowka D, Webb WW, Baird B (1986) J Cell Biol 102:541–550.
60. Menon A, Holowka D, Webb W, Baird B (1986) J Cell Biol 102:534–540.
61. Meder D, Moreno MJ, Verkade P, Vaz WLC, Simons K (2006) Proc Natl Acad
Sci USA 103:329–334.
62. Kirkwood JG, Goldberg RJ (1950) J Chem Phys 18:54–57.
63. Stanley HE (1971) Introduction to Phase Transitions and Critical Phenomena
64. Simons K, Vaz WLC (2004) Ann Rev Biophys Biomol Struct 33:269–295.
www.pnas.org?cgi?doi?10.1073?pnas.0611357104Baumgart et al.