Nanoelectropulse-driven membrane perturbation and small molecule permeabilization
© Vernier et al; licensee BioMed Central Ltd. 2006
Received: 07 June 2006
Accepted: 19 October 2006
Published: 19 October 2006
Nanosecond, megavolt-per-meter pulsed electric fields scramble membrane phospholipids, release intracellular calcium, and induce apoptosis. Flow cytometric and fluorescence microscopy evidence has associated phospholipid rearrangement directly with nanoelectropulse exposure and supports the hypothesis that the potential that develops across the lipid bilayer during an electric pulse drives phosphatidylserine (PS) externalization.
In this work we extend observations of cells exposed to electric pulses with 30 ns and 7 ns durations to still narrower pulse widths, and we find that even 3 ns pulses are sufficient to produce responses similar to those reported previously. We show here that in contrast to unipolar pulses, which perturb membrane phospholipid order, tracked with FM1-43 fluorescence, only at the anode side of the cell, bipolar pulses redistribute phospholipids at both the anode and cathode poles, consistent with migration of the anionic PS head group in the transmembrane field. In addition, we demonstrate that, as predicted by the membrane charging hypothesis, a train of shorter pulses requires higher fields to produce phospholipid scrambling comparable to that produced by a time-equivalent train of longer pulses (for a given applied field, 30, 4 ns pulses produce a weaker response than 4, 30 ns pulses). Finally, we show that influx of YO-PRO-1, a fluorescent dye used to detect early apoptosis and activation of the purinergic P2X7 receptor channels, is observed after exposure of Jurkat T lymphoblasts to sufficiently large numbers of pulses, suggesting that membrane poration occurs even with nanosecond pulses when the electric field is high enough. Propidium iodide entry, a traditional indicator of electroporation, occurs with even higher pulse counts.
Megavolt-per-meter electric pulses as short as 3 ns alter the structure of the plasma membrane and permeabilize the cell to small molecules. The dose responses of cells to unipolar and bipolar pulses ranging from 3 ns to 30 ns duration support the hypothesis that a field-driven charging of the membrane dielectric causes the formation of pores on a nanosecond time scale, and that the anionic phospholipid PS migrates electrophoretically along the wall of these pores to the external face of the membrane.
Nanosecond, megavolt-per-meter pulsed electric fields nondestructively perturb the intracellular environment, causing calcium bursts [1, 2], eosinophil sparklers , vacuole permeabilization , and the appearance of apoptotic indicators such as release of cytochrome c into the cytoplasm  and caspase activation [6, 7]. In addition to these effects in the cell interior, nanoelectropulse exposure also induces phosphatidylserine (PS) externalization – translocation of PS from the cytoplasmic face of the plasma membrane to the cell exterior – a normal event in platelet activation and blood coagulation , a diagnostic feature of apoptotic cells which serves as a physiological semaphore for their phagocytic removal , and a means of intramembrane signal transduction in lymphocytes .
Previously we have demonstrated, using annexin V binding as a measure of PS externalization , that exposing Jurkat T cells to 50, 7 ns pulses causes immediate PS translocation with field strengths above 2 MV/m, with little response to 1 MV/m pulses . Increasing the pulse count produces a proportionally greater response . The presence of 5 millimolar EGTA in the cell suspension during pulse exposure does not reduce subsequent annexin V binding, indicating that nanoelectropulse-induced PS translocation does not require calcium in the external medium . In addition, by employing the fluorescent dye FM1-43 as an indicator of relative changes in the phospholipid composition of the external leaflet of the plasma membrane , we have achieved real-time microscopic visualization of pulse-induced phospholipid scrambling, which occurs within milliseconds of pulse delivery, is pulse count- and field-dependent, and is confined always to the anode-directed pole of the cell .
PS is normally confined in healthy cells to the inner leaflet of the membrane lipid bilayer. This asymmetry is enforced by an energy barrier of approximately 100 kJ/mol  that impedes transport of the charged phospholipid head group across the hydrophobic interior of the membrane [16, 17]. Physiological regulation of PS distribution in the membrane is maintained by enzymatic activities that both scramble and restore the normal asymmetry [18–21], and is associated with the release of Ca2+ from internal stores , the proximity of depolarized mitochondria , and the restructuring of membrane-cytoskeletal attachments [24, 25].
Electroporation of cells under conditions conducive to the stabilization of large pores, using relatively low-field pulses of microsecond or millisecond duration, causes PS externalization in erythrocyte membranes [26, 27]. At the site of a long-lasting (milliseconds to seconds) pore, the inner and outer membrane leaflets align and merge, and PS can rapidly diffuse [28, 29] along this now contiguous surface.
What about nanosecond pulses? For a given pulsed bioelectrical experimental system at the cellular level, if the pulse duration is short enough relative to the charging time constant of the resistive-capacitive network formed by the conductive intracellular and extracellular fluids and the cell membrane dielectric, then the electric field is expressed across the intracellular space, while at the same time the potential difference that develops across the external membrane, initially very small, may not reach porating voltage levels [30, 31]. For human lymphocytes in growth medium the charging time constant for the plasma membrane lies in the range of 50 to 100 ns, using a dielectric shell model of the cell [32, 33]. Thus it is not surprising that previous reports have shown that nanosecond, megavolt-per-meter pulses (7–300 ns, 2.5–30 MV/m) also induce PS translocation, but without significant poration of the external membrane [5, 7], although a mechanism for this phospholipid rearrangement after submicrosecond pulse exposure remains to be established.
Vm(t) = 1.5 E0 a cos θ [1 - exp(-t/τm)], (1)
where E0 is the applied electric field, a is the cell radius, θ is the position angle relative to the electric field, t is the time after the initiation of the pulse, τm is the membrane charging time constant, and values for the parameters reflect the electrophysical characteristics of lymphocytes in serum (a = 5.0 μm, θ = 0, τm = 83 ns). As we stressed previously , the cell charging time constant is not precisely known, the dielectric shell model embodies only the most general electrophysical properties of the system, and a real population of cells is heterogeneous in size, shape, and physiological state. Nevertheless we may draw from these numbers, in agreement with those obtained from more sophisticated models [36, 37], the expectation that even a pulse of nanosecond duration will charge the external membrane of the cell to supraphysiological, porating potentials when the pulsed field strength is on the order of megavolts per meter. The conclusion follows that high-field pulses in the picosecond regime will be required in order to avoid producing significant (porating) plasma membrane potentials with megavolt-per-meter pulses.
Until sub-nanosecond pulse generators that can develop the requisite potentials across biological loads are available, we cannot make the simplifying assumption that the external membrane is unaffected by ultra-short, high-field electric pulses. In fact, all of the evidence we have assembled here and elsewhere points to the pulse-induced increase in transmembrane voltage as the primary driver for the PS translocation observed immediately after nanoelectropulse exposure in lymphocyte-derived cell lines.
In this paper we describe the membrane restructuring responses of cells to 3 ns and 4 ns pulses with applied field amplitudes up to 8 MV/m. Even with these very short pulses we must expect that the potential across the plasma membrane exceeds levels associated with increases in membrane conductance (poration) . Although it has not been clearly established whether poration is occurring under these circumstances or whether poration enables or facilitates nanoelectropulse-induced phospholipid rearrangement and PS externalization, our results here are consistent with nanosecond pulse-induced permeabilization of the cell membrane to small molecules. This new evidence suggests that some poration, undetectable with conventional methods, is occurring even with pulse durations as short as 3 ns, if the electric field is high enough, and that these nanoelectropulse-induced membrane defects may be the sites for the migration of PS to the outer leaflet of the lipid bilayer.
We tested four overlapping hypotheses relating to the mechanism of nanoelectropulse-induced phospholipid rearrangement and PS externalization: 1. that the PS molecule is driven across the membrane lipid bilayer by the action of the electric field on the negatively charged PS head group, either directly across the hydrophobic interior of the membrane or as an electrophoretic migration at transient membrane nanopores; 2. that nanosecond pulse-induced membrane restructuring and PS translocation depends on the charging of the membrane dielectric; 3. that pulse-driven PS externalization does not require intracellular or extracellular calcium even with pulse durations as short as 3 ns; 4. that the formation of transient, nanometer-scale pores facilitates PS translocation, either through electrophoresis in the pore walls or as a result of the phospholipid scrambling that accompanies pore formation and subsequent passive "lateral" diffusion from the PS-rich inner leaflet along the solvent-facing surface of the pore to the outer leaflet of the membrane.
Pulse polarity and membrane perturbation patterns are consistent with electric field-driven PS translocation
Although we observe a similar anodic polarization in images of cells pulsed in the presence of fluorescent-tagged annexin V , the high fluorescence background and the slower kinetics of annexin V binding lead us to prefer membrane-bound FM1-43 fluorescence as a rapidly responding marker for perturbation of the lipid bilayer. FM1-43, which partitions between the aqueous medium and the cytoplasmic membrane has been identified as an effective and rapidly responsive indicator of PS translocation in Jurkat cells . Translocation of the negatively charged PS head group to the outer face of the membrane provides additional electrostatic attraction for the quaternary ammonium of FM1-43, resulting in more dye binding per unit area and a concomitant increase in fluorescence emission. The fluorescence quantum yield of FM1-43 increases by several orders of magnitude on membrane binding , facilitating real-time microscopic observations of changes in externalized PS by eliminating the need for washing. Because the increased FM1-43 fluorescence associated with PS externalization results from the insertion of additional dye molecules into the membrane, the time resolution for observations of PS translocation is limited by the rate of diffusion of FM1-43 to the medium-membrane interface and by the rate of insertion of the FM1-43 tail into the array of phospholipids at the membrane surface. Although FM1-43 does not have the PS specificity of annexin V, observations of membrane restructuring at time scales of seconds or less than a second are greatly facilitated by the more rapid kinetics of the FM1-43 response . Extensions of this study will be necessary to define more precisely the details of electric pulse-driven membrane reorganization, but all of our evidence is consistent with the interpretation that PS externalization is a significant component of that reorganization.
Pulse width and pulse amplitude. Shorter pulses require higher fields, consistent with a time-dependent charging of the membrane dielectric
Nanoelectropulse-induced membrane restructuring and PS externalization does not require extracellular or intracellular calcium
Small-molecule electropermeabilization after nanosecond pulse exposure
The failure of previous efforts to demonstrate influx of ions and small molecules from the medium into the cytoplasm after nanosecond, megavolt-per-meter pulse treatment [1, 7, 12, 14] has not conclusively established that nanoporation – the generation of nanometer-diameter pores with lifetimes of nanoseconds – does not occur, but rather only that it has not been detectable under the conditions of our experiments. Because even relatively small amounts of calcium entering or sodium leaving the cytoplasm can trigger a physiologically large response through cascading signal transduction chains or membrane depolarization, we have continued to seek evidence that nanosecond pulsed electric fields generate pores that might conduct ions or larger species into (or out of) the cell even for a few nanoseconds.
To test the possibility that nanosecond pulsed electric fields in these experiments are activating the P2X7 receptors, allowing YO-PRO-1 to cross the membrane through these channels, we pulsed cells in the presence of the P2X7 receptor inhibitor Brilliant Blue G . No measurable effect on YO-PRO-1 influx was observed even at Brilliant Blue G concentrations as high as 100 μM.
This new evidence for membrane permeabilization after nanosecond electric pulse exposure (nanoporation) is consistent with the pore-facilitated phospholipid translocation proposed in the fourth hypothesis above.
The idea that very short electric pulses can bypass the capacitance of the plasma membrane and reach the cell interior has stimulated an expanding variety of experimental studies and the development of a new technology . Calculations based on a simple dielectric shell model of the cell indicate, however, that even for pulse durations as short as 2 ns, the megavolt-per-meter external fields needed to develop significant potentials across intracellular structures will charge the plasma membrane to the critical voltage associated with the appearance of high conductance pores after longer pulse exposures (Fig. 1). It is reasonable to expect then that nanoelectropulse manipulations of cells will have effects both in the cytoplasm and at the external cell membrane.
While most studies of nanosecond, megavolt-per-meter bioelectrical phenomena have focused on intracellular events (apoptosis, calcium signaling, intracellular membrane permeation, nuclear organization), the PS externalization that appears immediately after nanoelectropulse exposure offers the possibility of characterizing within a relatively constrained and well understood system (the phospholipid bilayer membrane and the aqueous cytoplasmic and extracellular environment at the membrane boundary) the mechanism or mechanisms that directly mediate the interactions of pulsed electric fields with living cells.
We have now established that nanoelectropulse-induced membrane perturbation is field-driven and polarized (phospholipid scrambling occurs only at the anode-facing pole of the cell; the magnitude of the response follows the field strength), that shorter pulses require higher fields for lipid bilayer rearrangement (as would be expected for a mechanism that requires an increase in the membrane potential above the resting level), that calcium is not required (indicating that the calcium-sensitive enzymatic activities that maintain or scramble the normal membrane phospholipid asymmetry are not needed for the membrane reorganization that immediately follows pulse exposure), and that permeabilization of the plasma membrane to small molecules can be detected after nanoelectropulse exposure, albeit with higher fields and faster pulse repetition rates than are needed for visualization of membrane perturbation and intracellular calcium release. In addition, although localized FM1-43 fluorescence intensification cannot be taken in isolation as a specific indicator of PS externalization, previous studies of nanoelectropulse-driven PS translocation indicated by annexin V binding [7, 12], and recent work combining annexin V and FM1-43 fluorescence imaging results and molecular dynamics simulations , point to a close association between the nanoelectropulse-induced membrane perturbations reported here and the PS translocation associated with ultra-short, high-field electric pulse exposure.
Current models of electroporation incorporate the well-established observation that the conductivity of a lipid bilayer increases by orders of magnitude when the transmembrane potential approaches 1 V, or even as low as 200 mV under some conditions . Transient, aqueous, stochastic pore models [47, 48] accommodate higher external electric fields with conductive pores that increase in number and diameter, clamping the membrane voltage at the critical, porating value . Without this pore-dependent voltage regulation the transmembrane potential during a megavolt-per-meter pulsed field that lasts for only a few nanoseconds could rise to several volts, corresponding to a gigavolt-per-meter averaged across the 5 nm thickness of the lipid bilayer. Recent theoretical work [36, 37] and experimental evidence  suggests that the membrane potential can increase to 1.5 V or more under these conditions, but determining what is really occurring on the nano scale – spatial and temporal – remains a challenge for those who model and those who measure.
Our observations of immediate phospholipid scrambling after exposure of cells to pulsed fields from 3 ns to 30 ns and 2 MV/m to 8 MV/m are consistent with the hypothesis that under the conditions of our experiments the critical membrane voltage is reached and exceeded, at least for a few nanoseconds, generating nanometer-diameter, nanosecond-duration openings in the lipid bilayer [48, 51]. Although these pores would be expected to close quickly after the trailing edge of the pulse under physiological conditions , they would provide a low-energy path for migration of PS from the inner leaflet of the membrane to the outer surface. Repeated cycles of pulse-induced nanoporation would successively permit additional molecules of inner-membrane PS to find these tunnels to the external face of the cell.
Although this descriptive model may be sufficient to explain experimental observations at a broad level, it is predictive only in a qualitative sense. It should be considered progress nevertheless, since even a simplified engineering analysis presents substantial computational challenges, and the dynamic complexity of living biological structures raises a caution flag over even the most rigorous reduction of the cell to compartments of conductors and insulators. Future investigations will benefit from an ongoing synthesis, of hypothesis-driven data generation and data-constrained model hypotheses.
Most of the details that must be managed are susceptible to biophysical analysis. Pulse electrical properties (rise and fall time, shape), pore formation kinetics, distribution and migration of intracellular and extracellular ions after pore formation , electrical requirements and time course of PS electrophoresis through pores, the unknown but potentially significant role of membrane proteins in pore formation [54–57], and other complex parameters are all factors that may be incorporated at some point into molecular dynamics simulations or distributed network, transport lattice, or more abstract models. Molecular dynamics seems particularly suitable as a partner for experimental studies of the immediate interactions between the pulsed electric field and the cell. Initial work along these lines in our laboratory  and others [37, 58, 59], including simulations of PS externalization [39, 60] indicates the utility of this approach.
In addition, we have presented evidence here for nanoelectropulse-induced small molecule permeabilization. Our previous inability to demonstrate membrane permeability after nanoelectropulse exposure, despite repeated attempts with many indicators and assays, represents a lack of sensitivity in the test methods and not an absence of the poration that theory, if not intuition, calls for. We can detect evidence of poration with our fluorescence microscopy system only if we use higher fields than have previously been available to us, and if they are delivered at a higher rate than we have used in our prior work.
It is not clear at this point whether the nanoelectropulse-induced YO-PRO-1 influx we observe is the result of the formation of hydrophilic pores in a process similar to long-pulse electroporation, or whether it is the consequence of activating purinergic receptor channels, perhaps specifically the P2X7 receptor channel, or some combination of these. Activation of the P2X7 receptor is associated with apoptosis , and YO-PRO-1 influx is used not only to detect P2X7 receptor activation [44, 62] but also as a sensitive indicator of early apoptosis  which has been incorporated into a commercially available assay. This may be a key to the mechanism for nanoelectropulse-induced apoptosis. In our experiments we see a polarized entry of YO-PRO-1 into cells at both the anodic and cathodic faces, implying electroporation, but nanoelectropulse-induced activation of the P2X7 receptor channel or another member of the P2X receptor channel family cannot be ruled out on this evidence alone. It will also be of interest to investigate why higher pulse repetition rates increase the amount of YO-PRO-1 (and propidium iodide) that enters the cell. Experimentally verifiable schemes involving channel or pore opening set-up times and-or hysteresis in the channel or pore relaxation (closing) process that occurs when the pulsed field is withdrawn are not difficult to devise.
The localized electrically driven perturbation of the lipid bilayer that results in PS externalization serves as an experimental entry point to several paths of investigation. The event itself is biophysically interesting, and the individual components are well characterized, which makes it a reasonable focus for testing and refining models of the cell membrane, including more and more realistic membranes containing proteins, a heterogeneous population of phospholipids, and other lipid, protein, and polysaccharide species. Nanoelectropulse perturbation of cells and tissues may be expected to lead also to fruitful biochemical and cell biological investigations. The role of PS externalization in mediating cell clearance in immune and apoptotic processes is well known, and new signaling functions for PS externalization are coming to light , but it can also reflect regulatory modifications to cytoskeletal-membrane associations [24, 25], and it may be possible to manipulate these cellular structures with nanoelectropulse treatment. Finally, the ability to nondestructively mark cells with a physiologically significant semaphore by means of a remotely delivered stimulus which could be targeted to specific cells and even specific regions of specific cells with a combination of varying pulse train recipes (amplitude, duration, pattern) and appropriate electrode placement and cell-binding ligands could be used to modulate cell activity and communication, including potentially the ability to induce malignant and other diseased cells to signal for their own removal [63, 64].
Electric pulses as short as 3 ns produce polarized (anode-directed) membrane disturbances that can be imaged with fluorescence microscopy and which are associated with phospholipid rearrangements and the influx of small molecules from the medium into the cytoplasm. Cellular responses to these previously uninvestigated very short pulse widths are similar to those observed with longer duration pulses and are consistent with a nanopore-facilitated, electrophoretic mechanism for the PS externalization observed after exposure of cells to nanosecond, megavolt-per-meter electric fields.
Cell lines and culture conditions
Human Jurkat T lymphoblasts (ATCC TIB-152) were grown in RPMI 1640 medium (Irvine Scientific, Irvine, CA) containing 10% heat-inactivated fetal bovine serum (FBS; Gibco, Carlsbad, CA), 2 mM L-glutamine (Gibco, Carlsbad, CA), 50 units/mL penicillin (Gibco, Carlsbad, CA), and 50 μg/mL streptomycin (Gibco, Carlsbad, CA) at 37 C in a humidified, 5% carbon dioxide atmosphere.
Pulse generators and pulse exposures
For microscopic observations, cells were placed in a rectangular channel 100 μm wide, 30 μm deep, and 12 mm long, with gold-plated electrode walls, microfabricated with photolithographic methods on a glass microscope slide . A fast MOSFET MicroPulser  was mounted on the microscope stage for delivery of 30 ns pulses directly to the microchamber electrodes in ambient atmosphere at room temperature as previously described . For bipolar pulse exposures, a standard USC MicroPulser was capacitively coupled to the load, so that for every trigger event a negative pulse followed by a positive pulse was delivered to the cells (a low-value resistor provides a current return path for the second pulse). A USC-designed and fabricated NanoPulser, with fast recovery diode switching, provided pulses with widths less than 10 ns .
Fluorescence microscopy and microphotometry
Observations of live cells during pulse exposures were made with a Zeiss Axiovert 200 epifluorescence microscope. For visualization of PS translocation with FM1-43 (Molecular Probes, Eugene OR; λex = 480 nm, λem = 535 nm), cells were washed twice, resuspended in growth medium containing 5–20 μM FM1-43, incubated for 20 minutes at 37°C, and observed without additional washing. EGTA was from Calbiochem (EMD Biosciences, San Diego, CA), BAPTA-AM, DiI, propidium iodide (PI), and YO-PRO-1 were from Molecular Probes (Invitrogen, Eugene, OR), and Brilliant Blue G was from Sigma-Aldrich (St. Louis, MO). Images were captured and analyzed with a LaVision Imager QE camera and software (LaVision, Goettingen, Germany). Photometric data is from at least 20 representative cells from three independent experiments. Error bars represent the standard error of the sample mean.
We gratefully recognize Matthew Behrend and Andras Kuthi for pulse generator design and assembly, and Christin Chong, Mya Mya Thu, and Jingjing Wang for cell culture and technical assistance with fluorescence microscopic imaging.
This work was made possible by support from the Air Force Office of Scientific Research. PTV is supported by MOSIS, Information Sciences Institute, Viterbi School of Engineering, University of Southern California.
- Vernier PT, Sun Y, Marcu L, Salemi S, Craft CM, Gundersen MA: Calcium bursts induced by nanosecond electric pulses. Biochem Biophys Res Commun. 2003, 310 (2): 286-295. 10.1016/j.bbrc.2003.08.140.PubMedGoogle Scholar
- White JA, Blackmore PF, Schoenbach KH, Beebe SJ: Stimulation of capacitative calcium entry in HL-60 cells by nanosecond pulsed electric fields. J Biol Chem. 2004, 279 (22): 22964-22972. 10.1074/jbc.M311135200.PubMedGoogle Scholar
- Schoenbach KH, Beebe SJ, Buescher ES: Intracellular effect of ultrashort electrical pulses. Bioelectromagnetics. 2001, 22 (6): 440-448. 10.1002/bem.71.PubMedGoogle Scholar
- Tekle E, Oubrahim H, Dzekunov SM, Kolb JF, Schoenbach KH, Chock PB: Selective field effects on intracellular vacuoles and vesicle membranes with nanosecond electric pulses. Biophys J. 2005, 89 (1): 274-284. 10.1529/biophysj.104.054494.PubMed CentralPubMedGoogle Scholar
- Beebe SJ, Fox PM, Rec LJ, Somers K, Stark RH, Schoenbach KH: Nanosecond pulsed electric field (nsPEF) effects on cells and tissues: Apoptosis induction and tumor growth inhibition. IEEE Transactions on Plasma Science. 2002, 30 (1): 286-292. 10.1109/TPS.2002.1003872.Google Scholar
- Beebe SJ, Fox PM, Rec LJ, Willis EL, Schoenbach KH: Nanosecond, high-intensity pulsed electric fields induce apoptosis in human cells. FASEB J. 2003, 17 (11): 1493-1495.PubMedGoogle Scholar
- Vernier PT, Li AM, Marcu L, Craft CM, Gundersen MA: Ultrashort pulsed electric fields induce membrane phospholipid translocation and caspase activation: Differential sensitivities of Jurkat T lymphoblasts and rat glioma C6 cells. IEEE Transactions on Dielectrics and Electrical Insulation. 2003, 10 (5): 795-809. 10.1109/TDEI.2003.1237329.Google Scholar
- Balasubramanian K, Schroit AJ: Aminophospholipid asymmetry: A matter of life and death. Annu Rev Physiol. 2003, 65: 701-734. 10.1146/annurev.physiol.65.092101.142459.PubMedGoogle Scholar
- Fadok VA, de Cathelineau A, Daleke DL, Henson PM, Bratton DL: Loss of phospholipid asymmetry and surface exposure of phosphatidylserine is required for phagocytosis of apoptotic cells by macrophages and fibroblasts. J Biol Chem. 2001, 276 (2): 1071-1077. 10.1074/jbc.M003649200.PubMedGoogle Scholar
- Elliott JI, Surprenant A, Marelli-Berg FM, Cooper JC, Cassady-Cain RL, Wooding C, Linton K, Alexander DR, Higgins CF: Membrane phosphatidylserine distribution as a non-apoptotic signalling mechanism in lymphocytes. Nat Cell Biol. 2005, 7 (8): 808-816. 10.1038/ncb1279.PubMedGoogle Scholar
- Koopman G, Reutelingsperger CP, Kuijten GA, Keehnen RM, Pals ST, van Oers MH: Annexin V for flow cytometric detection of phosphatidylserine expression on B cells undergoing apoptosis. Blood. 1994, 84 (5): 1415-1420.PubMedGoogle Scholar
- Vernier PT, Sun Y, Marcu L, Craft CM, Gundersen MA: Nanoelectropulse-induced phosphatidylserine translocation. Biophys J. 2004, 86 (6): 4040-4048. 10.1529/biophysj.103.037945.PubMed CentralPubMedGoogle Scholar
- Zweifach A: FM1-43 reports plasma membrane phospholipid scrambling in T-lymphocytes. Biochem J. 2000, 349 (Pt 1): 255-260. 10.1042/0264-6021:3490255.PubMed CentralPubMedGoogle Scholar
- Vernier PT, Sun Y, Marcu L, Craft CM, Gundersen MA: Nanosecond pulsed electric fields perturb membrane phospholipids in T lymphoblasts. FEBS Lett. 2004, 572 (1–3): 103-108. 10.1016/j.febslet.2004.07.021.PubMedGoogle Scholar
- Homan R, Pownall HJ: Transbilayer diffusion of phospholipids: dependence on headgroup structure and acyl chain length. Biochim Biophys Acta. 1988, 938 (2): 155-166. 10.1016/0005-2736(88)90155-1.PubMedGoogle Scholar
- Taupin C, Dvolaitzky M, Sauterey C: Osmotic pressure induced pores in phospholipid vesicles. Biochemistry. 1975, 14 (21): 4771-4775. 10.1021/bi00692a032.PubMedGoogle Scholar
- Popescu D, Victor G: The transversal diffusion coefficient of phospholipid molecules through black lipid membranes. Bioelectrochemistry and Bioenergetics. 1991, 25 (1): 105-108. 10.1016/0302-4598(91)87022-9.Google Scholar
- Verhoven B, Schlegel RA, Williamson P: Mechanisms of phosphatidylserine exposure, a phagocyte recognition signal, on apoptotic T lymphocytes. J Exp Med. 1995, 182 (5): 1597-1601. 10.1084/jem.182.5.1597.PubMedGoogle Scholar
- Seigneuret M, Devaux PF: ATP-dependent asymmetric distribution of spin-labeled phospholipids in the erythrocyte membrane: relation to shape changes. Proc Natl Acad Sci USA. 1984, 81 (12): 3751-3755. 10.1073/pnas.81.12.3751.PubMed CentralPubMedGoogle Scholar
- Basse F, Stout JG, Sims PJ, Wiedmer T: Isolation of an erythrocyte membrane protein that mediates Ca2+-dependent transbilayer movement of phospholipid. J Biol Chem. 1996, 271 (29): 17205-17210. 10.1074/jbc.271.29.17205.PubMedGoogle Scholar
- Comfurius P, Williamson P, Smeets EF, Schlegel RA, Bevers EM, Zwaal RF: Reconstitution of phospholipid scramblase activity from human blood platelets. Biochemistry. 1996, 35 (24): 7631-7634. 10.1021/bi9606859.PubMedGoogle Scholar
- Martinez MC, Martin S, Toti F, Fressinaud E, Dachary-Prigent J, Meyer D, Freyssinet JM: Significance of capacitative Ca2+ entry in the regulation of phosphatidylserine expression at the surface of stimulated cells. Biochemistry. 1999, 38 (31): 10092-10098. 10.1021/bi990129p.PubMedGoogle Scholar
- Blom WM, De Bont HJ, Nagelkerke JF: Regional loss of the mitochondrial membrane potential in the hepatocyte is rapidly followed by externalization of phosphatidylserines at that specific site during apoptosis. J Biol Chem. 2003, 278 (14): 12467-12474. 10.1074/jbc.M201264200.PubMedGoogle Scholar
- Kunzelmann-Marche C, Freyssinet JM, Martinez MC: Regulation of phosphatidylserine transbilayer redistribution by store-operated Ca2+ entry: role of actin cytoskeleton. J Biol Chem. 2001, 276 (7): 5134-5139. 10.1074/jbc.M007924200.PubMedGoogle Scholar
- Manno S, Takakuwa Y, Mohandas N: Identification of a functional role for lipid asymmetry in biological membranes: Phosphatidylserine-skeletal protein interactions modulate membrane stability. Proc Natl Acad Sci USA. 2002, 99 (4): 1943-1948. 10.1073/pnas.042688399.PubMed CentralPubMedGoogle Scholar
- Dressler V, Schwister K, Haest CW, Deuticke B: Dielectric breakdown of the erythrocyte membrane enhances transbilayer mobility of phospholipids. Biochim Biophys Acta. 1983, 732 (1): 304-307. 10.1016/0005-2736(83)90216-X.PubMedGoogle Scholar
- Haest CW, Kamp D, Deuticke B: Transbilayer reorientation of phospholipid probes in the human erythrocyte membrane. Lessons from studies on electroporated and resealed cells. Biochim Biophys Acta. 1997, 1325 (1): 17-33. 10.1016/S0005-2736(96)00239-8.PubMedGoogle Scholar
- Sonnleitner A, Schutz GJ, Schmidt T: Free brownian motion of individual lipid molecules in biomembranes. Biophys J. 1999, 77 (5): 2638-2642.PubMed CentralPubMedGoogle Scholar
- Fujiwara T, Ritchie K, Murakoshi H, Jacobson K, Kusumi A: Phospholipids undergo hop diffusion in compartmentalized cell membrane. J Cell Biol. 2002, 157 (6): 1071-1081. 10.1083/jcb.200202050.PubMed CentralPubMedGoogle Scholar
- Sher LD, Kresch E, Schwan HP: On the possibility of nonthermal biological effects of pulsed electromagnetic radiation. Biophys J. 1970, 10 (10): 970-979.PubMed CentralPubMedGoogle Scholar
- Schoenbach KH, Joshi RP, Kolb JF, Chen NY, Stacey M, Blackmore PF, Buescher ES, Beebe SJ: Ultrashort electrical pulses open a new gateway into biological cells. Proceedings of the IEEE. 2004, 92 (7): 1122-1137. 10.1109/JPROC.2004.829009.Google Scholar
- Plonsey R, Altman KW: Electrical stimulation of excitable cells – a model approach. Proceedings of the IEEE. 1988, 76 (9): 1122-1129. 10.1109/5.9658.Google Scholar
- Polevaya Y, Ermolina I, Schlesinger M, Ginzburg BZ, Feldman Y: Time domain dielectric spectroscopy study of human cells. II. Normal and malignant white blood cells. Biochim Biophys Acta. 1999, 1419 (2): 257-271. 10.1016/S0005-2736(99)00072-3.PubMedGoogle Scholar
- Kinosita K, Tsong TY: Voltage-induced pore formation and hemolysis of human erythrocytes. Biochim Biophys Acta. 1977, 471 (2): 227-242. 10.1016/0005-2736(77)90252-8.PubMedGoogle Scholar
- Zimmermann U: Electric field-mediated fusion and related electrical phenomena. Biochim Biophys Acta. 1982, 694 (3): 227-277.PubMedGoogle Scholar
- Stewart DA, Gowrishankar IR, Weaver JC: Transport lattice approach to describing cell electroporation: Use of a local asymptotic model. IEEE Transactions on Plasma Science. 2004, 32 (4): 1696-1708. 10.1109/TPS.2004.832639.Google Scholar
- Hu Q, Viswanadham S, Joshi RP, Schoenbach KH, Beebe SJ, Blackmore PF: Simulations of transient membrane behavior in cells subjected to a high-intensity ultrashort electric pulse. Phys Rev E Stat Nonlin Soft Matter Phys. 2005, 71 (3 Pt 1): 031914-PubMedGoogle Scholar
- Benz R, Beckers F, Zimmermann U: Reversible electrical breakdown of lipid bilayer membranes: a charge-pulse relaxation study. J Membr Biol. 1979, 48 (2): 181-204. 10.1007/BF01872858.PubMedGoogle Scholar
- Vernier PT, Ziegler MJ, Sun Y, Chang WV, Gundersen MA, Tieleman DP: Nanopore formation and phosphatidylserine externalization in a phospholipid bilayer at high transmembrane potential. J Am Chem Soc. 2006, 128 (19): 6288-6289. 10.1021/ja0588306.PubMedGoogle Scholar
- Schote U, Seelig J: Interaction of the neuronal marker dye FM1-43 with lipid membranes. Thermodynamics and lipid ordering. Biochim Biophys Acta. 1998, 1415 (1): 135-146. 10.1016/S0005-2736(98)00188-6.PubMedGoogle Scholar
- Williamson P, Christie A, Kohlin T, Schlegel RA, Comfurius P, Harmsma M, Zwaal RF, Bevers EM: Phospholipid scramblase activation pathways in lymphocytes. Biochemistry. 2001, 40 (27): 8065-8072. 10.1021/bi001929z.PubMedGoogle Scholar
- Idziorek T, Estaquier J, De Bels F, Ameisen JC: YOPRO-1 permits cytofluorometric analysis of programmed cell death (apoptosis) without interfering with cell viability. J Immunol Methods. 1995, 185 (2): 249-258. 10.1016/0022-1759(95)00172-7.PubMedGoogle Scholar
- Hickman SE, el Khoury J, Greenberg S, Schieren I, Silverstein SC: P2Z adenosine triphosphate receptor activity in cultured human monocyte-derived macrophages. Blood. 1994, 84 (8): 2452-2456.PubMedGoogle Scholar
- Jiang LH, Mackenzie AB, North RA, Surprenant A: Brilliant blue G selectively blocks ATP-gated rat P2X7 receptors. Mol Pharmacol. 2000, 58 (1): 82-88.PubMedGoogle Scholar
- Schoenbach KH, Katsuki S, Stark RH, Buescher ES, Beebe SJ: Bioelectrics – new applications for pulsed power technology. IEEE Transactions on Plasma Science. 2002, 30 (1): 293-300. 10.1109/TPS.2002.1003873.Google Scholar
- Teissie J, Tsong TY: Electric field induced transient pores in phospholipid bilayer vesicles. Biochemistry. 1981, 20 (6): 1548-1554. 10.1021/bi00509a022.PubMedGoogle Scholar
- Sugar IP, Neumann E: Stochastic model for electric field-induced membrane pores. Electroporation. Biophys Chem. 1984, 19 (3): 211-225. 10.1016/0301-4622(84)87003-9.PubMedGoogle Scholar
- Popescu D, Rucareanu C, Victor G: A model for the appearance of statistical pores in membranes due to self-oscillations. Bioelectrochemistry and Bioenergetics. 1991, 25 (1): 91-103. 10.1016/0302-4598(91)87021-8.Google Scholar
- Weaver JC: Electroporation of biological membranes from multicellular to nano scales. IEEE Transactions on Dielectrics and Electrical Insulation. 2003, 10 (5): 754-768. 10.1109/TDEI.2003.1237325.Google Scholar
- Frey W, White JA, Price RO, Blackmore PF, Joshi RP, Nuccitelli R, Beebe SJ, Schoenbach KH, Kolb JF: Plasma membrane voltage changes during nanosecond pulsed electric field exposure. Biophys J. 2006, 90 (10): 3608-3615. 10.1529/biophysj.105.072777.PubMed CentralPubMedGoogle Scholar
- Weaver JC, Chizmadzhev YA: Theory of electroporation: a review. Bioelectrochemistry and Bioenergetics. 1996, 41 (2): 135-160. 10.1016/S0302-4598(96)05062-3.Google Scholar
- Zimmermann U: The effect of high intensity electric field pulses on eukaryotic cell membranes: fundamentals and applications. Electromanipulation of Cells. Edited by: Zimmermann U, Neil GA. 1996, Boca Raton, FL: CRCGoogle Scholar
- DeBruin KA, Krassowska W: Modeling electroporation in a single cell. II. Effects of ionic concentrations. Biophys J. 1999, 77 (3): 1225-1233.PubMed CentralPubMedGoogle Scholar
- Eisenberg M, Hall JE, Mead CA: The nature of the voltage-dependent conductance induced by alamethicin in black lipid membranes. J Membr Biol. 1973, 14 (2): 143-176.PubMedGoogle Scholar
- Fattal E, Nir S, Parente RA, Szoka FC: Pore-forming peptides induce rapid phospholipid flip-flop in membranes. Biochemistry. 1994, 33 (21): 6721-6731. 10.1021/bi00187a044.PubMedGoogle Scholar
- Wu G, Hubbell WL: Phospholipid asymmetry and transmembrane diffusion in photoreceptor disc membranes. Biochemistry. 1993, 32 (3): 879-888. 10.1021/bi00054a020.PubMedGoogle Scholar
- Hessel E, Muller P, Herrmann A, Hofmann KP: Light-induced reorganization of phospholipids in rod disc membranes. J Biol Chem. 2001, 276 (4): 2538-2543. 10.1074/jbc.M009061200.PubMedGoogle Scholar
- Tieleman DP: The molecular basis of electroporation. BMC Biochem. 2004, 5 (1): 10-10.1186/1471-2091-5-10.PubMed CentralPubMedGoogle Scholar
- Tarek M: Membrane electroporation: a molecular dynamics simulation. Biophys J. 2005, 88 (6): 4045-4053. 10.1529/biophysj.104.050617.PubMed CentralPubMedGoogle Scholar
- Hu Q, Joshi RP, Schoenbach KH: Simulations of nanopore formation and phosphatidylserine externalization in lipid membranes subjected to a high-intensity, ultrashort electric pulse. Phys Rev E Stat Nonlin Soft Matter Phys. 2005, 72 (3 Pt 1): 031902-PubMedGoogle Scholar
- Wang Q, Wang L, Feng YH, Li X, Zeng R, Gorodeski GI: P2X7 receptor-mediated apoptosis of human cervical epithelial cells. Am J Physiol Cell Physiol. 2004, 287 (5): C1349-C1358. 10.1152/ajpcell.00256.2004.PubMedGoogle Scholar
- Surprenant A, Rassendren F, Kawashima E, North RA, Buell G: The cytolytic P2Z receptor for extracellular ATP identified as a P2X receptor (P2X7). Science. 1996, 272 (5262): 735-738.PubMedGoogle Scholar
- Vernier PT, Sun Y, Wang J, Thu MM, Garon E, Valderrabano M, Marcu L, Koeffler HP, Gundersen MA: Nanoelectropulse intracellular perturbation and electropermeabilization technology: phospholipid translocation, calcium bursts, chromatin rearrangement, cardiomyocyte activation, and tumor cell sensitivity. Proceedings of the IEEE Engineering in Medicine and Biology Society 27th International Conference: Shanghai. 1–4 September 2005;Google Scholar
- Nuccitelli R, Pliquett U, Chen X, Ford W, James Swanson R, Beebe SJ, Kolb JF, Schoenbach KH: Nanosecond pulsed electric fields cause melanomas to self-destruct. Biochem Biophys Res Commun. 2006, 343 (2): 351-360. 10.1016/j.bbrc.2006.02.181.PubMed CentralPubMedGoogle Scholar
- Sun Y, Vernier PT, Behrend M, Marcu L, Gundersen MA: Electrode microchamber for noninvasive perturbation of mammalian cells with nanosecond pulsed electric fields. IEEE Transactions on Nanobioscience. 2005, 4 (4): 277-283. 10.1109/TNB.2005.859544.PubMedGoogle Scholar
- Behrend M, Kuthi A, Gu XY, Vernier PT, Marcu L, Craft CM, Gundersen MA: Pulse generators for pulsed electric field exposure of biological cells and tissues. IEEE Transactions on Dielectrics and Electrical Insulation. 2003, 10 (5): 820-825. 10.1109/TDEI.2003.1237331.Google Scholar
- Kuthi A, Gabrielsson P, Behrend M, Vernier PT, Gundersen M: Nanosecond pulse generator using fast recovery diodes for cell electromanipulation. IEEE Transactions on Plasma Science. 2005, 33 (4): 1192-1197. 10.1109/TPS.2005.852403.Google Scholar
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