Resources - Application Bulletins
Microplate-based Cell Viability Assays using Absorbance, Fluorescence, or Luminescence DetectionDownload
Related Products: Synergy LX
May 31, 2018
As many as one-third of all putative drugs fail from toxicity issues which contributes to the high cost of pharmaceutical R&D, particularly if toxicity is proven in clinical trials. Thus toxicity testing of small molecules is typically performed pre-clinically using cell-based in-vitro assays as a first step to establishing any toxicity issues. There are numerous assay technologies available commercially for probing cellular viability where adverse effects cause a drop in assay signal. These assays are typically designed for workflows that use microplates and optical detection typical of microplate readers. In this technical bulletin, we demonstrate three of these cell viability technologies that use absorbance, fluorescence or luminescence detection all measured on the low cost Synergy™ LX Multi-Mode Reader.
Materials and Methods
Human Prostate Cancer cell line (PC-3) cells were cultured in Hams F12K Nutrient mixture supplemented with 10% fetal bovine serum and penicillin-streptomycin at 37 °C in 5% CO2. Cultures were routinely trypsinized (0.05% Trypsin-EDTA) at 80% confluence.
Cells lines were plated into Corning 3904 black sided clear bottom 96-well microplates using DMEM/ F12 media without phenol red such that there were 30,000 total cells/well in 100 μL. After 24 hours to allow for attachment, the cytotoxic compounds cycloheximide and tamoxifen were added to the cultures at various concentrations in 100 μL. After 24 hours of exposure, 100 μL of cell media was removed and diluted reagent added according to the outlines below.
Colorimetric MTT Assay
10 μL of 12 mM Vybrant™ MTT Cell Proliferation Assay reagent (Life technologies, cat # V 13154) was added. Reaction was allowed to proceed for 4 hours at 37 °C in a humidified environment. The reaction was stopped and the insoluble formazan product resolublized by the addition of 100 μL of 10% SDS in 0.01 N HCl solution and incubation for 16 hours at 37 °C in a humidified environment. Absorbance at 570 nm was measured with a Synergy LX Multi-Mode Reader (BioTek Instruments, Winooski, VT) using the dedicated UV-Vis monochromator.
Fluorometric Calcein AM Assay
100 μL of 5 μM Calcein AM (Life technologies, cat # C34852) was added. Cells were incubated at 37°C for 30 minutes, after which fluorescence was determined using a Synergy LX using a green fluorescence cube. The green fluorescence cube is configured with a 485/20 excitation filter, a 528/20 emission filter, and a 510 nm cut off dichroic mirror.
Luminescent CellTiter-Glo® Assay
100 μL of reconstituted CellTiter-Glo Cell Viability reagent (Promega cat # G7572) was added. The plate was shaken on an orbital shaker for 2 minutes then incubated for 10 minutes in the dark at room temperature within the Synergy LX reader prior to luminescence determination using a Synergy LX with a dedicated luminescence cube. This cube allows direct passage of light from the microplate well to the PMT detector. The default settings for PMT gain (135) and the collection time (1 sec) were used.
Cell Titration Experiments
For cell titration experiments, a range of PC-3 cell concentrations were used up to 36,000 cells/well. After 24 hours, reagent was added according to manufacturer’s specifications and read on the Synergy LX using the detection modes described above.
Results and Discussion
Each of the reagents tested probes cell health, albeit in different ways. The colorimetric MTT assay relies on endogenous NAD(P)H oxidoreductase enzymes to reduce MTT to a colored formazan dye; the Calcein AM reagent is converted by endogenous cytoplasmic esterases from a non-fluorescent to a fluorescent compound; and CellTiter-Glo is based on the quantification of ATP present, which indicates the presence of metabolically active cells. Thus for each reagent, one would expect greater assay signals as more viable cells are present. This is evident in Figure 1 demonstrating cell titrations for each of the detection technologies tested.
Figure 1. Cell titration curves for colorimetric MTT, fluorometric Calcein AM and luminescent CellTiter-Glo. All data were normalized to the maximum signal for each detection technology. Each data point represents an average of eight replicates.
In the case of a toxicity experiment, where cell health is probed after addition of small molecule compounds, one would expect reduction in signals for each of these detection technologies should the compound display toxicity. The extent of reduction depends on how the specific enzymes involved in generating signal are affected or the metabolic activity of the cells in the case of ATP measurement. Figure 2 illustrates these impacts when the cells are treated with cycloheximide and tamoxifen.
Figure 2. Dose response curves of the compounds cycloheximide and tamoxifen for A) colorimetric MTT assay; B) fluorometric Calcein AM assay; C) luminescent CellTiter-Glo assay. Signal is represented as a percentage of the negative control. Each data point represents an average of eight replicates.
Cycloheximide is used widely in biomedical research to inhibit protein synthesis in eukaryotic cells studied in vitro. Its toxic effect is plainly seen in Figure 2 where for each technology, a significant drop in signal is evident with increasing dose of the compound. For each technology, the dose at half the maximum signal drop is approximately 0.1 μM. Note also that the extent of cytotoxicity appears to be greater for the detection technologies based on cytosolic enzyme turnover (MTT and Calcein AM) compared to ATP measurement (CellTiter-Glo). Conversely, tamoxifen demonstrates little toxicity over its full dose range, which is not unexpected for this widely used medication for breast cancer.
The Synergy™ LX Multi-Mode Reader is a low cost solution for the most common detection technologies used in life science research including absorbance, fluorescence and luminescence detection. Here we demonstrated its utility to quantify cellular toxicity using widely used cell viability assays that employ these common detection modes.