Treating Cells as Reagents to Design Reproducible Assays.

The reproducibility of high-throughput cell-based assays is dependent on having a consistent source of cells for each experiment. Developing an understanding of the nature of cells growing in vitro and factors that influence their responsiveness to test compounds will contribute to the development of reproducible cell-based assays. Using good cell culture practices and establishing standard operating procedures (SOPs) for handling cultures can eliminate several potential contributors to variability in the responsiveness and performance of cells. The SOPs for handling each cell type must have clear and detailed instructions that can be understood and followed among different laboratories. The SOPs should include documenting the source of cells and authenticating their identity, both of which have become required to achieve peer acceptance of experimental data. Variability caused by biological issues such as phenotypic drift can be reduced by using standardized subculture procedures or using cryopreserved cells to set up experiments. Variability caused by inconsistent dispensing of cells per well and edge effects can be identified by measuring how many cells are present and whether they are alive or dead. Multiplex methods for real-time measurement of viable or dead cell number in each sample can be used for normalizing data and determining if proliferation or cytotoxicity has occurred during the experiment. Following good cell culture practices will go a long way toward executing reproducible cell-based assays. Resources will be included describing good cell culture practices, cell line authentication, and multiplex determination of cell number as an internal control.

"Multiplexed viability, cytotoxicity, and caspase activity assays".

Multiplexed assay chemistries provide for multiple measurements of cellular parameters within a single assay well. This experimental practice is not only more cost efficient, but also provides more information about a compound or treatment. The ability to combine the activity profiles within the same sample provides a level of normalization not possible with parallel assays. Furthermore, multiplexing caspase activity assays with viability and/or cytotoxicity assays can support conclusions regarding cytotoxic mechanism and provide normalization, which may help correct for differences in cell number.

Homogeneous, bioluminescent proteasome assays.

Protein degradation is mediated predominantly through the ubiquitin-proteasome pathway. The importance of the proteasome in regulating degradation of proteins involved in cell-cycle control, apoptosis, and angiogenesis led to the recognition of the proteasome as a therapeutic target for cancer. The proteasome is also essential for degrading misfolded and aberrant proteins, and impaired proteasome function has been implicated in neurodegerative and cardiovascular diseases. Robust, sensitive assays are essential for monitoring proteasome activity and for developing inhibitors of the proteasome. Peptide-conjugated fluorophores are widely used as substrates for monitoring proteasome activity, but fluorogenic substrates can exhibit significant background and can be problematic for screening because of cellular autofluorescence or interference from fluorescent library compounds. Furthermore, fluorescent proteasome assays require column-purified 20S or 26S proteasome (typically obtained from erythrocytes), or proteasome extracts from whole cells, as their samples. To provide assays more amenable to high-throughput screening, we developed a homogeneous, bioluminescent method that combines peptide-conjugated aminoluciferin substrates and a stabilized luciferase. Using substrates for the chymotrypsin-like, trypsin-like, and caspase-like proteasome activities in combination with a selective membrane permeabilization step, we developed single-step, cell-based assays to measure each of the proteasome catalytic activities. The homogeneous method eliminates the need to prepare individual cell extracts as samples and has adequate sensitivity for 96- and 384-well plates. The simple "add and read" format enables sensitive and rapid proteasome assays ideal for inhibitor screening.

Cytotoxicity testing: measuring viable cells, dead cells, and detecting mechanism of cell death.

Testing the effects of compounds on the viability of cells grown in culture is widely used as a predictor of potential toxic effects in whole animals. Among the several alternative assays available, measuring the levels of ATP is the most sensitive, reliable, and convenient method for monitoring active cell metabolism. However, recently developed combinations of methods have made it possible to collect more information from in vitro cytotoxicity assays using standard fluorescence and luminescence plate readers. This chapter describes two assay methods. The first utilizes beetle luciferase for measuring the levels of ATP as a marker of viable cells. The second more recently developed multiplex method relies on selective measurement of three different protease activities as markers for viable, necrotic, and apoptotic cells. Data analysis from the measurement of three marker protease activities from the same sample provides a useful tool to help uncover the mechanism of cell death and can serve as an internal control to help identify assay artifacts.

Cell-based bioluminescent assays for all three proteasome activities in a homogeneous format.

A luminescent method to individually measure the chymotrypsin-like, trypsin-like, or caspase-like activities of the proteasome in cultured cells was developed. Each assay uses a specific luminogenic peptide substrate in a buffer optimized for cell permeabilization, proteasome activity, and luciferase activity. Luminescence is generated in a coupled-enzyme format in which proteasome cleavage of the peptide conjugated substrate generates aminoluciferin, which is a substrate for luciferase. The homogeneous method eliminates the need to prepare individual cell extracts as samples. Luminogenic proteasome substrates and buffer formulations enabled development of a single reagent addition method with adequate sensitivity for 96- and 384-well plate formats. Proteasome trypsin-like specificity was enhanced by incorporating a mixture of protease inhibitors that significantly reduce nonspecific serum and cellular backgrounds. The assays were used to determine EC(50) values for the specific proteasome inhibitors epoxomicin and bortezomib for each of the catalytic sites using a variety of cancer lines. These cell-based proteasome assays are direct, simple, and sensitive, making them ideal for high-throughput screening.

In vitro viability and cytotoxicity testing and same-well multi-parametric combinations for high throughput screening.

In vitro cytotoxicity testing has become an integral aspect of drug discovery because it is a convenient, costeffective, and predictive means of characterizing the toxic potential of new chemical entities. The early and routine implementation of this testing is testament to its prognostic importance for humans. Although a plethora of assay chemistries and methods exist for 96-well formats, few are practical and sufficiently sensitive enough for application in high throughput screening (HTS). Here we briefly describe a handful of the currently most robust and validated HTS assays for accurate and efficient assessment of cytotoxic risk. We also provide guidance for successful HTS implementation and discuss unique merits and detractions inherent in each method. Lastly, we discuss the advantages of combining specific HTS compatible assays into multi-parametric, same-well formats.

Bioluminescent assays for ADMET.

Bioluminescent assays couple a limiting component of a luciferase-catalyzed photon-emitting reaction to a variable parameter of interest, while holding the other components constant or non-limiting. In this way light output varies with the parameter of interest. This review describes three bioluminescent assay types that use firefly luciferase to measure properties of drugs and other xenobiotics which affect their absorption, distribution, metabolism, elimination and toxicity. First, levels of the luciferase enzyme itself are measured in gene reporter assays that place a luciferase cDNA under the control of regulatory sequences from ADMET-related genes. This approach identifies activators of nuclear receptors that regulate expression of genes encoding drug-metabolizing enzymes and drug transporters. Second, drug effects on enzyme activities are monitored with luminogenic probe substrates that are inactive derivatives of the luciferase substrate luciferin. The enzymes of interest convert the substrates to free luciferin, which is detected in a second reaction with luciferase. This approach is used with the drug-metabolizing CYP and monoamine oxidase enzymes, apoptosis-associated caspase proteases, a marker protease for non-viable cells and with glutathione-S-transferase to measure glutathione levels in cell lysates. Third, ATP concentration is monitored as a marker of cell viability or cell death and as a way of identifying substrates for the ATP-dependent drug transporter, P-glycoprotein. Luciferase activity is measured in the presence of a sample that supplies the requisite luciferase substrate, ATP, so that light output varies with ATP concentration. The bioluminescent ADMET assays are rapid and sensitive, amenable to automated high-throughput applications and offer significant advantages over alternative methods.

Caspase activity assays.

Caspase activity assays in multi-well plate formats represent powerful tools for understanding experimental modulation of the apoptotic response. These assays are configured to exploit functional, biochemical, and temporal differences in substrate specificity and selectivity, which are useful in defining the magnitude and mechanism of a compound or treatment effect. New advances in fluorescent and luminescent chemistries now enable single addition "add-mix- measure" determinations of caspase activity directly in the sample plate with unprecedented sensitivity. Unlike other more cumbersome or laborious techniques, caspase activity induction or inhibition measures are quantifiable and definitive. The highlighted techniques in this chapter are cost efficient and allow for the rapid exploration of thousands of combinations and conditions.

Multiplex caspase activity and cytotoxicity assays.

Multiplexed assay chemistries provide for multiple measurements of cellular parameters within a single assay well. This experimental practice not only is more cost efficient but provides more informational content about a compound or treatment. For instance, multiplexed caspase activity assays can help establish the kinetics and magnitude of initiator and effector caspase induction by candidate compounds or treatments. The ability to combine the activity profiles within the same sample provides a level of normalization not possible with parallel assays. Furthermore, multiplexing caspase activity assays with viability and/or cytotoxicity assays can support conclusions regarding cytotoxic mechanism and provide normalization that may help correct for differences in cell number.

Homogeneous, bioluminescent proteasome assays.

Protein degradation is mediated predominantly through the ubiquitin-proteasome pathway. The importance of the proteasome in regulating degradation of proteins involved in cell-cycle control, apoptosis, and angiogenesis led to the recognition of the proteasome as a therapeutic target for cancer . The importance of the proteasome for general cell homeostasis has been established, and the 2004 Nobel Prize for Chemistry honored the researchers that discovered the ubiquitin-proteasome pathway. Robust, sensitive assays are essential for monitoring proteasome activity and for developing inhibitors of the proteasome. Peptide-conjugated fluorophores are widely used as substrates for monitoring proteasome activity, but fluorogenic substrates can exhibit significant background and can be problematic for screening because of cellular autoflorescence or fluorescent library compounds. To address these issues, we developed a homogeneous, bioluminescent method that combines peptide-conjugated aminoluciferin substrates and a stabilized luciferase. We have developed homogeneous, bioluminescent assays for all three proteasome activities, the chymotrypsin-like, trypsin-like, and caspase-like, using purified proteasome. We have also applied this technology to a cellular assay using the substrate for the chymotrypsin-like activity in combination with a selective membrane permeabilization step (patent pending). The proteasome assays are designed in a simple "add and read" format and have been tested in 96-and 384-well plates. The bioluminescent, coupled-enzyme format enables sensitive and rapid protease assays ideal for inhibitor screening.

Update on in vitro cytotoxicity assays for drug development.

BACKGROUND: in vitro cytotoxicity testing provides a crucial means of ranking compounds for consideration in drug discovery. The choice of using a particular viability or cytotoxicity assay technology may be influenced by specific research goals. OBJECTIVE: Although the high-throughput screening (HTS) utility is typically dependent upon sensitivity and scalability, it is also impacted by signal robustness and resiliency to assay interferences. Further consideration should be given to data quality, ease-of-use, reagent stability, and matters of cost-effectiveness. METHODS: Here we focus on three main classes of assays that are at present the most popular, useful, and practical for HTS drug discovery efforts. These methods measure: i) viability by metabolism reductase activities; ii) viability by bioluminescent ATP assays; or iii) cytotoxicity by enzymes 'released' into culture medium. Multi-parametric technologies are also briefly discussed. RESULTS/CONCLUSION: Each of these methods has its relative merits and detractions; however multi-parametric methods using both viability and cytotoxicity markers may mitigate the inherent shortcomings of single parameter measures.

A homogeneous assay to measure live and dead cells in the same sample by detecting different protease markers.

A method to simultaneously determine the relative numbers of live and dead cells in culture by introducing a combination of two fluorogenic substrates or a fluorogenic and a luminogenic protease substrate into the sample is described. The method is based on detection of differential ubiquitous proteolytic activities associated with intact viable cells and cells that have lost membrane integrity. A cell-permeable peptide aminofluorocoumarin substrate detects protease activity restricted to intact viable cells. Upon cell death, the viable cell protease marker becomes inactive. An impermeable peptide rhodamine 110 (or aminoluciferin) conjugated substrate detects protease activity from nonviable cells that have lost membrane integrity. The multiplex assay can detect 200 dead cells in a population of 10,000 viable cells. The protease substrate reagents do not damage viable cells over the course of the assay, thus the method can be multiplexed further with other assays in a homogeneous format. Ratiometric measurement of viable and dead cells in the same sample provides an internal control that can be used to normalize data from other cell-based assays.

A bioluminescent assay for monoamine oxidase activity.

This article describes a novel two-step homogeneous bioluminescent assay for monoamine oxidase (MAO) that is simple, sensitive, and amenable to high-throughput screening. In the first step, MAO reacts with an aminopropylether analog of methyl ester luciferin. In the second step, a luciferin detection reagent inactivates MAO and converts the product of the first step into a luminescent signal. The amount of light produced is proportional to the amount of MAO and the time of incubation in the first step, but the luminescent signal is stable in the second step with a half-life greater than 5h. The assay has high precision, is more sensitive than current fluorescent methods, and can accurately measure the binding constants of known substrates and inhibitors. An automated screen of the Sigma-RBI Library of Pharmacologically Active Compounds (LOPAC(1280)) revealed a surprisingly high percentage of MAO inhibitors (16%) with a low false hit rate (0.9%). This implies that a significant number of compounds interact with the MAO enzymes and suggests that it is important to include MAO assays in drug metabolism studies. Other advantages of this bioluminescent assay over comparable fluorescent assays are discussed.

New bioluminogenic substrates for monoamine oxidase assays.

Novel bioluminogenic substrates were designed for probing monoamine oxidase (MAO) activity based on a simple and effective beta-elimination strategy. By modifying the amino group and the central core of luciferin derivatives, we have developed a series of substrates useful for assays of MAO A or B, or both. One of these substrates, exhibiting low Km values and high signal-to-background ratios with both isozymes, was shown to accurately measure the Ki values of known MAO inhibitors. This substrate is a key component in the development of a highly sensitive homogeneous MAO assay for high-throughput screening (HTS) of compounds in drug discovery and for monitoring MAO activity in complex biological systems. This design strategy should be applicable to fluorogenic MAO substrates and could broaden the structural requirements of substrates for other enzyme assays.

Use of multiple assay endpoints to investigate the effects of incubation time, dose of toxin, and plating density in cell-based cytotoxicity assays.

Here we show the results of comparing cell viability, cytotoxicity, and apoptosis assays for measuring the time- and dose-dependent toxic effects of tamoxifen on HepG2 cells. The quantitation of adenosine 5'-triphosphate (ATP), 5-(3-carboxymethoxyphenyl)-2-(4,5- dimethylthiazolyl)-3-(4-sulfophenyl) tetrazolium, inner salt (MTS) tetrazolium reduction, and resazurin reduction methods used to estimate the number of viable cells all showed a similar trend of decreased cell viability after longer periods of tamoxifen exposure to HepG2 cells. The release of lactate dehydrogenase (LDH) as a marker for cells with a compromised membrane and the increase in caspase-3/7 activity as a marker for apoptosis were both shown to increase using the same tamoxifen exposure conditions that caused a decrease in HepG2 cell viability. The longer the duration of exposure of tamoxifen, the lower the concentration required to kill or induce apoptosis in HepG2 cells. In contrast, there was no change in LDH release from HL-60 cells using conditions of vinblastine treatment that caused an increase in caspase activity and a decrease in ATP content, suggesting a difference in the mechanism of cell death between the two model systems. Both the density of parent stock cultures used as a source of cells to prepare assay plates and the density of cells per well in the assay plates were demonstrated to be factors than can influence the apparent potency of a toxin in viability, toxicity, and apoptosis assays. These results illustrate the importance of understanding the kinetics and mechanism of cell death of each in vitro model system as prerequisites for choosing the most appropriate assay method.