Bacterial viability and antibiotic susceptibility testing with SYTOX green nucleic acid stain.

A fluorescent nucleic acid stain that does not penetrate living cells was used to assess the integrity of the plasma membranes of bacteria. SYTOX Green nucleic acid stain is an unsymmetrical cyanine dye with three positive charges that is completely excluded from live eukaryotic and prokaryotic cells. Binding of SYTOX Green stain to nucleic acids resulted in a > 500-fold enhancement in fluorescence emission (absorption and emission maxima at 502 and 523 nm, respectively), rendering bacteria with compromised plasma membranes brightly green fluorescent. SYTOX Green stain is readily excited by the 488-nm line of the argon ion laser. The fluorescence signal from membrane-compromised bacteria labeled with SYTOX Green stain was typically > 10-fold brighter than that from intact organisms. Bacterial suspensions labeled with SYTOX Green stain emitted green fluorescence in proportion to the fraction of permeabilized cells in the population, which was quantified by microscopy, fluorometry, or flow cytometry. Flow cytometric and fluorometric approaches were used to quantify the effect of beta-lactam antibiotics on the cell membrane integrity of Escherichia coli. Detection and discrimination of live and permeabilized cells labeled with SYTOX Green stain by flow cytometry were markedly improved over those by propidium iodide-based tests. These studies showed that bacterial labeling with SYTOX Green stain is an effective alternative to conventional methods for measuring bacterial viability and antibiotic susceptibility.     

Loss of host cell plasma membrane integrity following cell traversal by Plasmodium sporozoites in the skin

Plasmodium sporozoites are able to migrate through host cells by breaching their plasma membrane and gliding inside their cytoplasm. This migratory activity, called cell traversal (CT), was studied in vivo mainly using mutant sporozoites lacking the ability to wound host cells, and thus to perform CT. However, direct evidence of CT activity in host tissues by wild-type sporozoites remains scarce. Here, we describe a double-wounding assay to dynamically image CT activity in vivo and monitor cell membrane integrity over time. Based on the incorporation kinetics of a first live cell-impermeant dye, propidium iodide, we could determine whether traversed cells repair their wounded membranes or not. A second impermeant dye, SYTOX Green, was used to confirm the transient or the permanent loss of membrane integrity of traversed cells. This assay allowed, for the first time, the direct observation of sporozoites wounding and traversing host skin cells and showed that, while some traversed cells resealed their membrane, most became irreversibly permeable to these live cell-impermeant dyes. In combination with the study of CT-deficient sporozoites and the use of specific host cell markers, this intravital assay will provide the means to identify the nature of the cells traversed by sporozoites and will thus contribute to elucidating the role of CT by apicomplexan parasites in the vertebrate host.     

Ion channel-mediated uptake of cationic vital dyes into live cells: a potential source of error when assessing cell viability

Ionic “vital dyes” are commonly used to assess cell viability based on the idea that their permeation is contingent on a loss of membrane integrity. However, the possibility that dye entry is conducted into live cells by endogenous membrane transporters must be recognized and controlled for. Several cation-selective plasma membrane-localized ion channels, including the adenosine 5?-triphosphate (ATP)-gated P2X receptors, have been reported to conduct entry of the DNA-binding fluorescence dye, YO-PRO-1, into live cells. Extracellular ATP often becomes elevated as a result of release from dying cells, and so it is possible that activation of P2X channels on neighboring live cells could lead to exaggerated estimation of cytotoxicity. Here, we screened a number of fluorescent vital dyes for ion channel-mediated uptake in HEK293 cells expressing recombinant P2X2, P2X7, or TRPV1 channels. Our data shows that activation of all three channels caused substantial uptake and nuclear accumulation of YO-PRO-1, 4?,6-diamidino-2-phenylindole (DAPI), and Hoechst 33258 into transfected cells and did so well within the time period usually used for incubation of cells with vital dyes. In contrast, channel activation in the presence of propidium iodide and SYTOX Green caused no measurable uptake and accumulation during a 20-min exposure, suggesting that these dyes are not likely to exhibit measurable uptake through these particular ion channels during a conventional cell viability assay. Caution is encouraged when choosing and employing cationic dyes for the purpose of cell viability assessment, particularly when there is a likelihood of cells expressing ion channels permeable to large ions.     

Improved flow cytometric analysis of the budding yeast cell cycle

The budding yeast, Saccharomyces cerevisiae has been a remarkably useful model system for the study of eukaryotic cell cycle regulation. Flow cytometric analysis of DNA content in budding yeast has become a standard tool for the analysis of cell cycle progression. However, popular protocols utilizing the DNA binding dye, propidium iodide, suffer from a number of drawbacks that confound accurate analysis by flow cytometry. Here we show the utility of the DNA binding dye, SYTOX Green, in the cell cycle analysis of yeast. Samples analyzed using SYTOX Green exhibited better coefficients of variation, improved linearity between DNA content and fluorescence, and decreased peak drift associated with changes in dye concentration, growth conditions or cell size.     

A Novel Staining Protocol for Multiparameter Assessment of Cell Heterogeneity in Phormidium Populations (Cyanobacteria) Employing Fluorescent Dyes

Bacterial populations display high heterogeneity in viability and physiological activity at the single-cell level, especially under stressful conditions. We demonstrate a novel staining protocol for multiparameter assessment of individual cells in physiologically heterogeneous populations of cyanobacteria. The protocol employs fluorescent probes, i.e., redox dye 5-cyano-2,3-ditolyl tetrazolium chloride, ‘dead cell’ nucleic acid stain SYTOX Green, and DNA-specific fluorochrome 4′,6-diamidino-2-phenylindole, combined with microscopy image analysis. Our method allows simultaneous estimates of cellular respiration activity, membrane and nucleoid integrity, and allows the detection of photosynthetic pigments fluorescence along with morphological observations. The staining protocol has been adjusted for, both, laboratory and natural populations of the genus Phormidium (Oscillatoriales), and tested on 4 field-collected samples and 12 laboratory strains of cyanobacteria. Based on the mentioned cellular functions we suggest classification of cells in cyanobacterial populations into four categories: (i) active and intact; (ii) injured but active; (iii) metabolically inactive but intact; (iv) inactive and injured, or dead.     

CELLULAR DNA CONTENT OF MARINE PHYTOPLANKTON USING TWO NEW FLUOROCHROMES: TAXONOMIC AND ECOLOGICAL IMPLICATIONS1

Two new fluorochromes, PicoGreen® and SYTOX Green? stain (Molecular Probes, Inc.), are useful with flow cytometry for quantitative detection of cellular DNA in a variety of marina phytoplankton. The basic instrument configuration of modern low-power flow cytometers (15 mW, 488 nm excitation) is sensitive enough to detect the DNA signal in nearly all of the 121 strains (from 12 taxonomic classes)examined. The major advantages of these dyes over others are 1)suitability for direct use in seawater, 2)green fluorescence emission of the DNA-dye complex (wavelength 525 ± 15 nm) showing no overlap with the autofluorescence of the plankton pigments in the red band, 3) high fluorescence yield of the DNA-dye complex with an increase in fluorescence > 100-fold compared to the unstained cell, and 4)dyes can be used to quantify double-stranded DNA. The high sensitivity allowed the quantification of the DNA of the smallest known phyto-plankter (Prochlorococcus) as well as bacteria found in some of the algal cultures. Of the 12 taxonomic classes tested, only the 3 Nannochloropsis spp. (Eustagmatophyceae) stained poorly, and a few members of the Chlorophyceae and Pelagophyceae showed poor staining occasionally. In general, maximal fluorescence was achieved within 15 min after addition of the dye. Although the PicoGreen dye stained some living phytoplankton species, preservation is recommended for quantitation. SYTOX Green did not stain live cells. The combination of the dyes, therefore, allows the discrimination between live and dead cells in some algal groups (Prochlorococcus, diatoms, prasinophytes, and pelagophytes). Paraformaldehyde was preferred over glutaraldehyde for fixation to avoid (induced) green autofluorescence. Total DNA values measured in 90 algal species (ca. 121 strains) varied by a factor of 20,000. The lowest values were found in Prochlorococcus and the highest in a large dinoflagellate (Prorocentrum micans). DNA content appears to be a scaleable cell component covarying with the carbon and nitrogen contents of the phytoplankton cells. This covariation allows the total DNA content to be used as an accurate, independent estimate of total cell carbon biomass in unicellular pelagic phytoplankton.     

Improved Flow Cytometric Analysis of the Budding Yeast Cell Cycle

The budding yeast, Saccharomyces cerevisiae has been a remarkably useful model system for the study of eukaryotic cell cycle regulation. Flow cytometric analysis of DNA content in budding yeast has become a standard tool for the analysis of cell cycle progression. However, popular protocols utilizing the DNA binding dye, propidium iodide, suffer from a number of drawbacks that confound accurate analysis by flow cytometry. Here we show the utility of the DNA binding dye, SYTOX Green, in the cell cycle analysis of yeast. Samples analyzed using SYTOX Green exhibited better coefficients of variation, improved linearity between DNA content and fluorescence, and decreased peak drift associated with changes in dye concentration, growth conditions or cell size.

Key Words:

Flow cytometry, Cell cycle, Saccharomyces cerevisiae, SYTOX Green, Propidium iodide     

Antifungal mechanism of an anti-Pythium protein (SAP) from the marine bacterium Streptomyces sp. strain AP77 is specific for Pythium porphyrae,a causative agent of red rot disease in Porphyra spp

Previously we reported an antifungal protein specific to Pythium porphyrae, a causative agent of red rot disease afflicting seaweed Porphyra spp. This study was carried out to identify the antifungal mechanism of the antifungal protein to P. porphyrae. When we first examined the effect of an anti- Pythium protein (SAP) on the P. porphyrae cell walls, SAP did not decompose the six structural polysaccharides in Pythium cell walls. However, hyphal growth was significantly inhibited in Pythium cells treated with 50 microg/ml of SAP by MTT assay. Protoplasmic leakage was observed in P. porphyrae hyphae treated with SAP for 1 h, followed by hyphal swelling and disintegration, using SYTOX Green, and SAP permeabilized the membrane of P. porphyrae in a dose-dependent manner. Treating P. porphyrae cells with SAP in the presence of carbonyl cyanide m-chlorophenylhydrazone (CCCP), a membrane-depolarizing agent, significantly reduced the membrane permeability to SYTOX Green. Moreover, a similar effect was observed when the P. porphyrae cells were treated with SAP in the presence of MgCl2. In contrast, identical treatment in the presence of KCl significantly increased the membrane permeability to SYTOX Green. These results suggested that anti- Pythium mechanism of SAP was related to alteration of the membrane permeability in P. porphyrae.     

Cell death in individual freshwater phytoplankton species: relationships with population dynamics and environmental factors

ABSTRACT

Understanding and predicting changes in phytoplankton populations requires knowledge of losses due not only to sedimentation and grazing, but also to intrinsic processes (here, collectively termed ‘cell death’). Cell death is poorly understood, especially in freshwater phytoplankton, but experiments in culture often suggest involvement of abiotic factors (e.g. temperature, light, nutrients). The occurrence of cell death was examined in a simple, natural environment: a small, well-mixed, temperate, urban pond during a period of phytoplankton growth, from mid-July to mid-November. Abundances of 18 phytoplankton taxa were measured weekly and fluorescence microscopy and staining was used to detect dead cells (using SYTOX which measures loss of membrane integrity) and cells undergoing cell death (using Annexin-V, which measures lipid inversions of membranes, an early signal of cell death). Dead and dying cells occurred in most phytoplankton taxa, but incidence and timing varied considerably, e.g. species like the chlorophyte Ankistrodesmus spiralis showed 20–30% of cells staining with SYTOX and Annexin in late autumn when the population was decreasing, while the dinoflagellate Peridinium sp. showed staining of up to 50% of cells with STYOX throughout the period, and the cyanobacterium Microcystis aeruginosa occasionally showed staining of 100% of cells with SYTOX. Overall, there was some association between cell death staining and growth phase with 10–15% of the total community showing SYTOX and Annexin staining in late autumn, when most populations were declining. Cell death could not be correlated with thresholds or rapid changes in abiotic conditions (e.g. temperature, irradiance) or with indicators of nutrient limitation (e.g. N:P ratios). While abiotic factors have been clearly implicated in cell death within unialgal culture experiments, in natural freshwater ecosystems interactions between biotic factors, such as pathogens or allelopathy, may play greater roles in losses related to cell death and be distinct for different taxa.     

Staining of viable and nonviable myotubes and of myofibrils by the fluorescent dye merocyanine 540

Merocyanine 540 (MC 540) has been reported to interact specifically with excitable plasma membranes in live cells [3]. Here we show that the MC 540 fluorescence staining pattern previously believed to be characteristic of viable myotubes [3] is observed in formaldehyde-fixed cells. In contrast, viable myotubes show an MC 540 fluorescence staining pattern that is characteristic of cell surface staining (no internal structures fluoresce). The specific I-band and H-zone fluorescence of isolated myofibrils is also consistent with the interpretation that the fluorescence patterns previously reported for viable myotubes are in fact characteristic of cells with disrupted plasma membranes. Time-course observations of MC 540 and trypan blue staining of myotubes suggest that when plasma membrane integrity is lost, MC 540 fluorescence can be visualized inside the cell 5-10 min before trypan blue absorbance. Thus the trypan blue viability assay can be misleading when applied to myotubes.     

Utility of Green Fluorescent Nucleic Acid Dyes and Aluminum Oxide Membrane Filters for Rapid Epifluorescence Enumeration of Soil and Sediment Bacteria

High background fluorescence and unspecific staining hampered the epifluorescence enumeration of bacteria in 45% of the tested soil and sediment samples with 4′,6-diamidino-2-phenylindole (DAPI) and polycarbonate membrane filters. These problems of the determination of total cell counts can be circumvented by using green fluorescent high-affinity nucleic acid dyes and aluminum oxide membrane filters. Due to the bright staining of cells, we recommend SYBR Green II as dye.     

Fluorescent Fingerprints of Endolithic Phototrophic Cyanobacteria Living within Halite Rocks in the Atacama Desert

Halite deposits from the hyperarid zone of the Atacama Desert reveal the presence of endolithic microbial colonization dominated by cyanobacteria associated with heterotrophic bacteria and archaea. Using the λ-scan confocal laser scanning microscopy (CLSM) option, this study examines the autofluorescence emission spectra produced by single cyanobacterial cells found inside halite rocks and by their photosynthetic pigments. Photosynthetic pigments could be identified according to the shapes of the emission spectra and wavelengths of fluorescence peaks. According to their fluorescence fingerprints, three groups of cyanobacterial cells were identified within this natural extreme microhabitat: (i) cells producing a single fluorescence peak corresponding to the emission range of phycobiliproteins and chlorophyll a, (ii) cells producing two fluorescence peaks within the red and green signal ranges, and (iii) cells emitting only low-intensity fluorescence within the nonspecific green fluorescence signal range. Photosynthetic pigment fingerprints emerged as indicators of the preservation state or viability of the cells. These observations were supported by a cell plasma membrane integrity test based on Sytox Green DNA staining and by transmission electron microscopy ultrastructural observations of cyanobacterial cells.     

Development of a mechanism-based, DNA staining protocol using SYTOX orange nucleic acid stain and DNA fragment sizing flow cytometry

Accurate measurement of single DNA fragments by DNA fragment sizing flow cytometry (FSFC) depends upon precise, stoichiometric DNA staining by the intercalating dye molecules. In this study, we determined the binding characteristics of a commercially available 532 nm wavelength-excitable dye and used this information to develop a universal DNA staining protocol for DNA FSFC using a compact frequency-doubled Nd:YAG laser excitation source. Among twelve 532 nm wavelength-excitable nucleic acid staining dyes tested, SYTOX Orange stain showed the highest fluorescence intensity along with a large fluorescence enhancement upon binding to double-stranded DNA ( approximately 450-fold). Furthermore, using SYTOX Orange stain, accurate fragment-size-distribution histograms were consistently obtained without regard to the staining dye to base pair (dye/bp) ratio. A model describing two binding modes, intercalation (primary, yielding fluorescence) and external binding (secondary, involving fluorescence quenching), was proposed to interpret the performance of the dyes under different dye/bp ratios. The secondary equilibrium dissociation constant was found to be the most critical parameter in determining the sensitivity of each fluorophore to the staining dye/bp ratio. The measurements of both equilibrium dissociation constants provided us with a theoretical framework for developing a universal protocol which was successfully demonstrated over a wide range of DNA concentrations on a compact flow cytometer equipped with a frequency-doubled, diode-pumped, solid-state Nd:YAG laser for rapid and sensitive DNA fragment sizing.     

Ultrastructural alterations of Erwinia carotovora subsp. atroseptica caused by treatment with aluminum chloride and sodium metabisulfite

Aluminum and bisulfite salts inhibit the growth of several fungi and bacteria, and their application effectively controls potato soft rot caused by Erwinia carotovora. In an effort to understand their inhibitory action, ultrastructural changes in Erwinia carotovora subsp. atroseptica after exposure (0 to 20 min) to different concentrations (0.05, 0.1, and 0.2 M) of these salts were examined by using transmission electron microscopy. Plasma membrane integrity was evaluated by using the SYTOX Green fluorochrome that penetrates only cells with altered membranes. Bacteria exposed to all aluminum chloride concentrations, especially 0.2 M, exhibited loosening of the cell walls, cell wall rupture, cytoplasmic aggregation, and an absence of extracellular vesicles. Sodium metabisulfite caused mainly a retraction of plasma membrane and cellular voids which were more pronounced with increasing concentration. Bacterial mortality was closely associated with SYTOX stain absorption when bacteria were exposed to either a high concentration (0.2 M) of aluminum chloride or prolonged exposure (20 min) to 0.05 M aluminum chloride or to a pH of 2.5. Bacteria exposed to lower concentrations of aluminum chloride (0.05 and 0.1 M) for 10 min or less, or to metabisulfite at all concentrations, did not exhibit significant stain absorption, suggesting that no membrane damage occurred or it was too weak to allow the penetration of the stain into the cell. While mortality caused by aluminum chloride involves membrane damage and subsequent cytoplasmic aggregation, sulfite exerts its effect intracellularly; it is transported across the membrane by free diffusion of molecular SO2 with little damage to the cellular membrane.     

Effect of u.v. light irradiation, starvation and heat on Escherichia coliββ-D-galactosidase activity and other potential viability parameters

The effect of u.v. light irradiation and two other types of stress (heat and starvation) on cellular functions of Escherichia coli have been studied. The severe reduction of the culturable cell number (cfu) and the direct viable count (DVC) after exposure to moderate u.v. light doses (48 mWs cm-2), was not reflected by the dehydrogenase activity (5-cyano-2,3-ditolyl tetrazolium chloride (CTC)-positive cells), the membrane integrity (SYTOX Green-negative cells), the membrane potential (bis-(1,3-dibutylbarbituric acid) trimethine oxonol (DiBAC4[3]) (OXONOL)-negative cells), and the beta-D-galactosidase activity. All parameters were affected by high u.v. light doses. Cellular activities (CTC, SYTOX, OXONOL, beta-D-galactosidase activity) were intact in non-culturable cells with presumably severe damage to DNA, and the activities seemed not to be appropriate for detection of viable E. coli after u.v. light irradiation. Heating for 20-30 min at 63 degrees C was required to cause a severe loss of the beta-D-galactosidase activity and the numbers of CTC-positive, SYTOX Green-negative or OXONOL-negative cells. A large portion (> or = 38%) of pre-irradiated (190 mWs cm-2) cells maintained their ability to reduce CTC and exclude SYTOX Green and OXONOL after 51 d of starvation (dark, 7 degrees C) in phosphate-buffered saline.     

Fluorescence microplate-based assay for tumor necrosis factor activity using SYTOX Green stain

We have developed a simple, sensitive, fluorescence microplate-based assay for tumor necrosis factor (TNF) biological activity. The assay employs SYTOX Green nucleic acid stain to detect TNF-induced cell necrosis in actinomycin D sensitized cultured cell lines. SYTOX Green stain is a cationic unsymmetrical cyanine dye that is excluded from live cells but can readily penetrate cells with compromised cell membranes. Upon binding to cellular nucleic acids, the dye exhibits a large enhancement in fluorescence, which is monitored at fluorescein wavelengths. We detected 2.5 pg/mL and quantitated 25-500 pg/mL recombinant murine (rm) and recombinant human (rh) TNF-alpha, using mouse fibroblast-derived WEHI 164, WEHI 13var, and L929 cell lines. The procedure can also be used to detect agents that modulate TNF activity. We demonstrated complete inhibition of rhTNF-alpha using monoclonal anti-human TNF-alpha antibody and determined that approximately 20 ng/mL antibody was sufficient to neutralize 50% of the biological activity of 250 pg/mL rhTNF-alpha in these cell lines. Reagents are added in a single step, followed by a 6- to 8-h incubation period, during which the cytokine exhibits its effects. There are no wash steps, and the assay is readily amenable to automation and high-throughput screening procedures.     

Ultrastructural Alterations of Erwinia carotovora subsp. atroseptica Caused by Treatment with Aluminum Chloride and Sodium Metabisulfite

Aluminum and bisulfite salts inhibit the growth of several fungi and bacteria, and their application effectively controls potato soft rot caused by Erwinia carotovora. In an effort to understand their inhibitory action, ultrastructural changes in Erwinia carotovora subsp. atroseptica after exposure (0 to 20 min) to different concentrations (0.05, 0.1, and 0.2 M) of these salts were examined by using transmission electron microscopy. Plasma membrane integrity was evaluated by using the SYTOX Green fluorochrome that penetrates only cells with altered membranes. Bacteria exposed to all aluminum chloride concentrations, especially 0.2 M, exhibited loosening of the cell walls, cell wall rupture, cytoplasmic aggregation, and an absence of extracellular vesicles. Sodium metabisulfite caused mainly a retraction of plasma membrane and cellular voids which were more pronounced with increasing concentration. Bacterial mortality was closely associated with SYTOX stain absorption when bacteria were exposed to either a high concentration (0.2 M) of aluminum chloride or prolonged exposure (20 min) to 0.05 M aluminum chloride or to a pH of 2.5. Bacteria exposed to lower concentrations of aluminum chloride (0.05 and 0.1 M) for 10 min or less, or to metabisulfite at all concentrations, did not exhibit significant stain absorption, suggesting that no membrane damage occurred or it was too weak to allow the penetration of the stain into the cell. While mortality caused by aluminum chloride involves membrane damage and subsequent cytoplasmic aggregation, sulfite exerts its effect intracellularly; it is transported across the membrane by free diffusion of molecular SO₂ with little damage to the cellular membrane.     

Effects of hyperoxia on microvascular cells in vitro

Summary Microvascular cells are most vulnerable to direct oxygen damage. Using an in vitro model system we have investigated the effect of elevated oxygen on the proliferation, morphology, and integrity of microvascular endothelial cells (EC) and pericytes. Cultivation of these cells at oxygen concentrations of 40% for 1 wk resulted in the inhibition of EC proliferation but had no effect on the growth of the pericytes. Similarly, hyperoxia induced a dramatic change in the shape of the EC, increasing their spread area by close to six-fold. Under the same conditions, the spread area of the pericytes was unaffected. To understand the effect of the hyperoxic treatment on the cells, the integrity of various membrane systems was assessed.⁵¹Chromium release was used to monitor plasma membrane integrity. There was no difference in chromium release by EC and pericytes over the 7 d of growth under normoxic and hyperoxic conditions. Mitochondrial integrity was examined by staining the cells with Rhodamine 123, which is selectively accumulated by the mitochondria. The staining pattern of the mitochondria of both EC and pericytes was altered by growth in the elevated oxygen. Finally, the lysosomes were visualized using acridine orange. The acridine orange staining pattern revealed enlarged and perinuclear lysosomes in the EC but no change in the pericyte lysosomal staining pattern. Thus, the cells of the microvasculature seem to be differentially affected by hyperoxia, a fact that may be significant in the etiology of reperfusion injury, ischemic disease, and pathologies associated with prematurity. This research was supported by grant E4-05318 from the National Institutes of Health, Bethesda, MD.     

Live-cell assay for detection of apoptosis by dual-laser flow cytometry using Hoechst 33342 and 7-amino-actinomycin D

This protocol describes a rapid and simple method for the identification of apoptotic cells. Owing to changes in membrane permeability, early apoptotic cells show an increased uptake of the vital DNA dye Hoechst 33342 (HO342) compared with live cells. The nonvital DNA dye 7-amino-actinomycin D (7-AAD) is added to distinguish late apoptotic or necrotic cells that have lost membrane integrity from early apoptotic cells that still have intact membranes as assayed by dye exclusion. The method is suitable to be combined with cell surface staining using Abs of interest labeled with fluorochromes that are compatible with HO342 and 7-AAD emissions. Surface antigen staining is carried out according to standard methods before staining for apoptosis. The basic assay can be completed in 30 min, and extra time is needed for cell surface antigen staining.     

Modified Annexin V/Propidium Iodide Apoptosis Assay For Accurate Assessment of Cell Death

Studies of cellular apoptosis have been significantly impacted since the introduction of flow cytometry-based methods. Propidium iodide (PI) is widely used in conjunction with Annexin V to determine if cells are viable, apoptotic, or necrotic through differences in plasma membrane integrity and permeability^1,2. The Annexin V/ PI protocol is a commonly used approach for studying apoptotic cells³. PI is used more often than other nuclear stains because it is economical, stable and a good indicator of cell viability, based on its capacity to exclude dye in living cells ^4,5. The ability of PI to enter a cell is dependent upon the permeability of the membrane; PI does not stain live or early apoptotic cells due to the presence of an intact plasma membrane ^1,2,6. In late apoptotic and necrotic cells, the integrity of the plasma and nuclear membranes decreases^7,8, allowing PI to pass through the membranes, intercalate into nucleic acids, and display red fluorescence ^1,2,9. Unfortunately, we find that conventional Annexin V/ PI protocols lead to a significant number of false positive events (up to 40%), which are associated with PI staining of RNA within the cytoplasmic compartment¹⁰. Primary cells and cell lines in a broad range of animal models are affected, with large cells (nuclear: cytoplasmic ratios <0.5) showing the highest occurrence¹⁰. Herein, we demonstrate a modified Annexin V/ PI method that provides a significant improvement for assessment of cell death compared to conventional methods. This protocol takes advantage of changes in cellular permeability during cell fixing to promote entry of RNase A into cells following staining. Both the timing and concentration of RNase A have been optimized for removal of cytoplasmic RNA. The result is a significant improvement over conventional Annexin V/ PI protocols (< 5% events with cytoplasmic PI staining).