- Research article
- Open Access
Maitotoxin-induced membrane blebbing and cell death in bovine aortic endothelial cells
© Estacion and Schilling; licensee BioMed Central Ltd. 2001
- Received: 28 December 2000
- Accepted: 6 February 2001
- Published: 6 February 2001
Maitotoxin, a potent cytolytic agent, causes an increase in cytosolic free Ca2+ concentration ([Ca2+]i) via activation of Ca2+-permeable, non-selective cation channels (CaNSC). Channel activation is followed by formation of large endogenous pores that allow ethidium and propidium-based vital dyes to enter the cell. Although activation of these cytolytic/oncotic pores, or COP, precedes release of lactate dehydrogenase, an indication of oncotic cell death, the relationship between CaNSC, COP, membrane lysis, and the associated changes in cell morphology has not been clearly defined. In the present study, the effect maitotoxin on [Ca2+]i, vital dye uptake, lactate dehydrogenase release, and membrane blebbing was examined in bovine aortic endothelial cells.
Maitotoxin produced a concentration-dependent increase in [Ca2+]i followed by a biphasic uptake of ethidium. Comparison of ethidium (Mw 314 Da), YO-PRO-1 (Mw 375 Da), and POPO-3 (Mw 715 Da) showed that the rate of dye uptake during the first phase was inversely proportional to molecular weight, whereas the second phase appeared to be all-or-nothing. The second phase of dye uptake correlated in time with the release of lactate dehydrogenase. Uptake of vital dyes at the single cell level, determined by time-lapse videomicroscopy, was also biphasic. The first phase was associated with formation of small membrane blebs, whereas the second phase was associated with dramatic bleb dilation.
These results suggest that maitotoxin-induced Ca2+ influx in bovine aortic endothelial cells is followed by activation of COP. COP formation is associated with controlled membrane blebbing which ultimately gives rise to uncontrolled bleb dilation, lactate dehydrogenase release, and oncotic cell death.
- Single Cell Level
- Human Embryonic Kidney Cell
- Human Skin Fibroblast
- Membrane Blebbing
- Bovine Aortic Endothelial Cell
Maitotoxin (MTX), one of the most potent marine toxins known, is found in the "red-tide" dinoflagellate, Gambierdiscus toxicus, and is responsible in part for Ciguatera seafood poisoning. In all cells examined to date, MTX at subnanomolar concentrations causes a profound increase in cytosolic free Ca2+ concentration ([Ca2+]i) . This occurs, not by release of Ca2+ from internal stores, but rather from activation of a ubiquitously-expressed, non-selective, Ca2+-permeable cation channel (CaNSC), present in the plasmalemma [2,3,4,5,6,7,8]. Channel activation is followed after a short lag by the activation or formation of large endogenous pores that allow organic molecules with molecular weights of <800 Da to cross the plasma membrane . The activation of these pores can be determined experimentally by following the uptake of ethidium and propidium-based vital dyes. These dyes, of varying molecular weights, are normally excluded from the cytoplasm of intact viable cells, but gain access to the cell interior following pore formation where they bind to nucleic acids with a concomitant increase in dye fluorescence. The large pores activated by MTX have been referred to as cytolytic/oncotic pores, or COP, since their activation ultimately leads to the release of lactate dehydrogenase (LDH), an indication of necrotic or oncotic cell death .
The cell death cascade activated by MTX is not unique to this toxin. Stimulation of P2X purinergic receptors by ATP causes similar changes in cytosolic Ca2+ and vital dye uptake [10,11,12,13,14,15,16,17] suggesting that MTX activates a cell death cascade that is physiologically relevant, although the exact role of either the P2X- or MTX-induced cascade in normal cellular biology remains unknown. For the P2X receptor it has been suggested that the Ca2+-permeable channels grow in size to form the dye-permeable pores through either aggregation of channel subunits or through dilation of the existing channel pore structure [12,18,19,20,21]. In support of this model it has been found that the kinetics of ATP-induced pore formation in HEK cells, heterologously expressing the P2X7 receptor, appears to depend on molecular size of the permeating ionic species . However, we recently showed that although MTX and ATP activate distinct channels, the characteristics of the ATP- and MTX-activated COP are indistinguishable . These results suggest that the channel and COP are unique molecular structures. The aggregation or dilation model make specific predictions concerning the kinetics of dye uptake. In particular, this model predicts a delay between channel activation and dye uptake and this delay should be directly proportional to the molecular size of the permeating dye. Furthermore, if pores grow in size, dye uptake should be nonlinear with time. In contrast, if channel activation causes the formation or activation of a molecularly unique COP with fixed pore dimensions, the delay between channel activation and dye uptake should be independent of molecular size, but the subsequent rate of dye uptake should be linear and inversely proportional to molecular weight. To distinguish between these two models, the effect of MTX on [Ca2+]i, vital dye uptake and LDH release was examined in bovine aortic endothelial cells, a cell line particularly sensitive to the cytolytic effects of MTX. The results of the present study are consistent with the activation of an endogenous COP of fixed pore dimensions.
The opening of large pores in the plasmalemma is expected to cause a dramatic change in the ionic concentration gradients that normally exist between the extracellular and intracellular milieus, i.e., loss of K+, and gain of Na+, Ca2+, and Cl- by the cell. The concomitant flow of water into the cell as a result of this ionic redistribution, will drive the cell towards the Gibbs-Donnan equilibrium. The change in osmotic pressure will produce cell swelling and ultimately membrane rupture and release of large macromolecules from the cytoplasm. This final phase in the cell death cascade can be monitored experimentally by measuring the release of the ubiquitous cytosolic enzyme, LDH. The role of COP and the biophysical mechanism associated with this rather violent cellular event remains unknown. However, many cell types undergo membrane blebbing in response to changes in osmotic pressure. Such membrane blebbing, which may in a sense represent a cellular safety valve, has been reported during both ATP- and MTX-induced cell death [19,22], but it is unclear if blebbing occurs before, during, or after COP formation or LDH release. In the present study, the effect of MTX on vital dye uptake in BAECs was correlated with changes in cell morphology using single cell fluorescence videomicroscopy. The videos presented demonstrate that COP activation as indicated by vital dye uptake correlates in time with the formation of membrane blebs, and that membrane lysis, i.e., LDH release, is associated with dramatic bleb dilation.
MTX increases [Ca2+]i in BAECs
MTX activates COP in BAECs
MTX induces LDH release
MTX produces similar changes in dye uptake in single BAECs
Previous studies suggested that ATP-induced pores in HEK cells heterologously expressing the P2X7 purinergic receptor, were formed either by dilation of the channel structure or by aggregation of channels subunits . However, these studies relied on shifts in the reversal potential of whole-cell membrane currents. Although this is a sensitive technique for determining the time course of pore formation, these experiments do not eliminate the possibility that COP and the P2X channel are separate entities. In the present study, the effect of MTX on membrane permeability occurred in three distinct phases. The first phase reflects the activation of a CaNSC and a large and rapid increase in [Ca2+]i. After a short lag, the activation of COP allowed uptake of vital dyes into the cell and the lag was independent of dye molecular weight. At the highest concentration of MTX examined, dye uptake via COP was linear and inversely proportional to molecular weight. These results suggest that COP does not increase in size as a function of time, as would be predicted by the dilation or aggregation model. Furthermore, these results strongly suggest that the CaNSC and the COP are unique molecular structures.
MTX causes biphasic membrane blebbing
File 1: Montage.avi: BAECs on glass cover-slips were perfused with HBS at 37°C. A phase (left) and fluorescence (right) image pair was obtained every 30 sec for 40 min. MTX (0.3 nM) was added to the bath solution at time 5 min. The time-lapse video was created from the captured images as described in Material and Methods, with a time compression of 3.5 minutes (i.e., 7 images) per second. (AVI )
To better appreciate the dynamic nature of bleb formation and to clearly observe the rapid nuclear staining associated with bleb dilation, we created time-lapsed movies in which the bright-field and fluorescence images were merged into a single video (Fig 2, EB.avi and Fig 3, YO-PRO.avi; Additional Data Files section). By setting your video viewer to continuously loop (i.e., auto replay), and by focusing during each sequence on a single cell within the field of view, it can be seen that fluorescence increases slowly during bleb formation, but that intense rapid dye staining occurs during the bleb dilation phase. As seen in Fig 5, and in each of these videos, MTX-induced blebbing results in an enormous increase in membrane surface area which may represent stretching of the membrane or an evagination of existing caveolar structures associated with the plasmalemma of endothelial cells. Endothelial cells are also known to have an extensive system of intracellular vesicles which are used for transporting substances from the blood to the interstitial space, i.e., transcytotic vesicles. Thus, membrane blebbing could reflect a massive exocytotic event. Why this would occur at selective sites on the plasmalemma remains unknown. Interestingly, the videos show several examples of blebs forming on the surface of pre-existing blebs during the dilation phase. Thus, the structural element(s) that are required for localized evagination of membrane appears to be membrane-associated and/or "pulled" from the cytoplasm during the initial bleb formation. Irrespective of the exact mechanism, the experiments reported in the present study are the first to correlate MTX-induced vital dye uptake with alterations in cell morphology.
MTX-induced membrane blebbing requires Ca2+
In conclusion, MTX treatment of BAECs causes a specific sequence of events (i.e., a cell death cascade) that is triggered by the activation of CaNSC and a rise in [Ca2+]i. This is followed by formation or activation of COP which is correlated with the formation of membrane blebs. COP appears to be a unique molecule associated with the plasma membrane and to have a fixed pore geometry and conductance for each vital dye examined. Furthermore, activation of COP provides the initial driving force for osmotic swelling and bleb formation. LDH release, indicative of the final phase of MTX-induced cell death, is associated with massive bleb dilation. Although, the molecular mechanisms associated with each step in the cell death cascade remain unknown, MTX may prove to be an important tool for understanding the biochemical and biophysical links between channel activation, COP formation, and membrane blebbing.
Solutions and reagents
Unless otherwise indicated, HEPES-buffered saline (HBS) contained 140 mM NaCl, 5 mM KCl, 1 mM MgCl2, 10 mM D-glucose, 1.8 mM CaCl2, 15 mM HEPES, 0.1% bovine serum albumin, pH adjusted to 7.40 at 37°C with NaOH. Ca2+-free HBS contained 0.3 mM EGTA and the same salts as HBS without added CaCl2. Fura-2 acetoxymethyl ester (fura-2/AM), ethidium bromide, YO-PRO-1 and POPO-3 were obtained from Molecular Probes (Eugene, OR, USA). Maitotoxin, obtained from LC Laboratories (Woburn, MA) or Wako Bioproducts (Richmond, VA), was stored at -20°C in ethanol. All other salts and chemicals were of reagent grade.
Bovine aortic endothelial cells were cultured as previously described  using Dulbecco's modified Eagles medium (GIBCO) supplemented with 10% fetal bovine serum (Hyclone, Logan UT), 100 μg/ml streptomycin and 100 μg/ml penicillin (complete-DMEM). All cultures demonstrated contact-inhibited cobblestone appearance typical of endothelial cells.
Measurement of the apparent cytosolic free Ca2+ concentration
[Ca2+]i was measured using the fluorescent indicator, fura-2, as previously described . Experiments were performed with cells in the twelfth to twentieth passage and 2-3 days post-confluency. Briefly, cells were harvested and re-suspended in HBS containing 20 μM fura-2/AM. Following 30 min incubation at 37°C, the cell suspension was diluted ∼ 10-fold with HBS, incubated for an additional 30 min, washed and resuspended in fresh HBS. Aliquots from this final suspension were subjected to centrifugation and washed twice immediately prior to fluorescence measurement. Fluorescence was recorded using an SLM 8100 spectrophotofluorometer; excitation wavelength alternated between 340 and 380 nm and fluorescence intensity was monitored at an emission wavelength of 510 nm. All measurements were performed at 37°C.
Measurement of vital dye uptake
An aliquot (2 ml) of dispersed cells suspended in HBS at 37°C was placed in a cuvette. Following addition of ethidium bromide (final concentrations of 5 μM), fluorescence was recorded as a function of time with excitation and emission wavelengths of 302/560 nm, respectively. All ethidium bromide fluorescence values are corrected for background (extracellular) dye fluorescence and expressed as a percentage relative to the value obtained following complete permeabilization of the cells with 50 μM digitonin. Uptake of POPO-3 and YO-PRO-1 was determined as described for ethidium with excitation/emission wavelengths of 530/565 and 468/510 nm, respectively.
For single cell measurement of vital dye uptake, BAECs in complete-DMEM were sparsely seeded on circular glass coverslips and used within 2-3 days of seeding. The coverslips were mounted in temperature-controlled perfusion chambers and placed on the stage of Nikon Diaphot inverted microscope. The cells were illuminated with light from a 75 watt xenon lamp using a O-5717 filter cube obtained from Molecular Probes. Epifluorescence was recorded using a Hamamatsu intensified CCD camera (model XC-77) and images were acquired and analyzed using Image-1 software (Universal Imaging, West Chester, PA). During each experiment, image pairs were collected at thirty second intervals. Images (8-bit gray scale) were stored as averages of sixteen video frames (phase images) or as accumulations of four video frames (fluorescent images) with shutter controllers switching between light and fluorescent illumination. The fluorescence images were used to determine dye uptake as a function of time. Using Image-1 software, regions were defined over single cells and the average fluorescence intensity of the region was quantified. The phase images were contrast enhanced using Debabelizer Pro software (Equilibrium, Sausalito, CA) and merged with the corresponding fluorescent images using Spot™ camera software (Diagnostic Instruments, Sterling Heights, MI). Time-lapse videos were created using Debabelizer Pro software with ethidium and YO-PRO epifluorescence displayed as red and green pseudocolor images, respectively.
Measurement of lactate dehydrogenase (LDH) release
Aliquots of dispersed cells (2 ml) were incubated at 37°C for various lengths of time in the presence and absence of MTX. The cells were pelleted by centrifugation for 15 sec at 12,000 rpm in an Eppendorf centrifuge (model 5415 C). The supernatants were removed, and placed on ice. Enzyme activity in aliquots (50 μl) of the supernatants was determined using the LD-L kit from Sigma. All values are expressed as percent LDH released relative to the value obtained following permeabilization of the cells with 50 μM digitonin.
This work was supported in part by NIH grant GM52019 and grant 9806267 from the American Heart Association. We gratefully acknowledge the technical assistance of Zack Novince and Justin Weinberg.
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