Quantitative, Real-Time Measurements of Intracellular Target Engagement Using Energy Transfer.

Intracellular target affinity and residence time are fundamental aspects of pharmacological mechanism (Lu and Tonge, Curr Opin Chem Biol 14:467-474, 2010). Although various robust biochemical approaches exist to measure these binding characteristics, analysis of compound binding with isolated targets may not accurately reflect engagement in the milieu of living cells. To realize the influence of cellular context, methods are needed that are capable of quantifying affinity and residence time in the presence of the intracellular factors that may impact target engagement. Bioluminescence resonance energy transfer (BRET) offers a solution for intracellular target engagement when quantitative metrics or kinetic analyses are required.


Introduction
While quantitation of compound binding to isolated targets is readily achieved, similar biophysical assessments in living systems represent a challenge. Cell-based assays of target engagement are most commonly achieved by assessing the dynamics of cell signaling. Although these methods allow for interrogation of compound potency using live cells, pathway analysis methods generally integrate the activities of multiple protein targets. Consequently, the molecular targets of drug molecules can be ambiguous when analyzed within the framework of a pathway. The ideal target engagement format provides a direct, biophysical assessment of compound binding at the selected intracellular target, therefore providing a bridge between reductionist biochemical assays and traditional cellular pathway analysis readouts. A number of novel techniques have been recently developed that allow for the interrogation of targets derived from cells or cell extracts. Each technique offers certain advantages and disadvantages that should be evaluated according to the requirements of the study. The cellular thermal shift assay (CETSA) represents a significant advancement for cellular analysis, as it queries compound binding of endogenously expressed targets, using intact cells [1]. However, CETSA is an indirect measure of compound engagement, and is reportedly prone to noteworthy false negative and false positive results for clinically relevant probe molecules [1]. Activitybased proteomics reagents offer a more direct assessment of compound binding via mass spectrometry (MS) [2]. However, the majority of such MS techniques involve dissolution of the cell membrane, and consequently a dilution of key cellular factors that are known to impact inhibitor potency. While these methods enable analysis of endogenously expressed targets, each has a significant limitation that should be considered. Activity-based proteomics methods do not assess target engagement under a thermodynamic equilibrium with the unlabeled drug molecule in living cells, thus limiting their ability to measure intracellular affinity. Acquisition of CETSA data to estimate IC 50 values can be labor-intensive and does not necessarily correlate directly to thermodynamic affinity. Such approaches also fail to offer real-time analysis of target engagement inside intact cells. When quantitation of affinity and residence time is desired, alternate approaches should be considered.
A recently described technique using Bioluminescence Resonance Energy Transfer (BRET) offers a quantitative analysis of target engagement in living cells under both equilibrium and nonequilibrium conditions [3,4]. This method, termed NanoBRET (TM), is a highly sensitive measure of molecular proximity and offers a direct and real-time capability for measuring molecular interactions in live cells. Briefly, reporter complexes are formed inside live cells, when a luciferase (e.g., NanoLuc(R)) -tagged target protein reaches dynamic equilibrium with cell-permeable fluorescent probe molecules (tracers). Upon binding of an unlabeled compound, the complex is disrupted, leading to a loss of BRET that can easily be monitored and scaled in a microplate format (Fig. 1). In many cases, the NanoBRET tracers can be readily designed from drug or tool compounds, generally offering a quantitative analysis of apparent affinity and a real-time analysis of residence time [3, [5][6][7].
However, this approach has technical requirements that must first be considered and carefully followed in order to achieve quantitation in live cells. The following chapter outlines: (1) considerations for development of novel cell-permeable tracers, (2) optimization of conditions for intracellular BRET, and (3) protocols for quantitative and real-time analysis of target engagement in live cells in the context of HTS work flows.

Development and Characterization of NanoBRET™ Tracers with Optimal Cell Permeability
To achieve quantitation in living cells, the BRET technique exploits permeable fluorescent reporter probes (or tracers), derived from chemical matter with appropriate binding characteristics for the select target protein or protein family. Tracers may be derived from compounds with high selectivity for the target protein, but in many cases, broad-spectrum inhibitors or published tool compounds can be utilized to achieve greater coverage if desired [4]. The chemical synthesis of functional tracers involves the covalent conjugation of a biologically active small molecule to a fluorescent organic dye. Certain organic dyes have proven optimal in maintaining cell permeability with spectral properties required for NanoBRET(TM) (Fig. 2a). These dyes are readily coupled to base compounds containing pendant amine groups via a one-step reaction of a highly reactive, activated ester group on the dye to produce a stable amide linkage.
Tracers must permeate live cells and function in a complex intracellular environment. Thus, there are several physical requirements that must be considered during the design phase. First, high affinity compounds may yield the most useful intracellular tracers. Within the milieu of cells, strong affinity may be required to overcome competition from endogenous metabolites or enzymatic Fig. 2 The structures of NanoBRET(TM) activated ester dyes (a) and example linker building blocks (b). NanoBRET(TM) dyes balance permeability and energy transfer efficiency, resulting in higher signal, stability and reactivity. Dyes directly coupled to the inhibitor yield the tracers, though it may be necessary to install a linker group to provide separation between the core and the fluorescent tag. In general, C3 to C6 alkyl, as well as O1 to O4 PEGs are suitable as starting points substrates that may compete directly with the tracer. Second, the intrinsic binding kinetics of tracer for the target may also be important for consideration. In general, compounds with rapid equilibration kinetics also offer better capabilities for real-time analysis of target engagement (i.e., residence time analysis). Finally, the base scaffold must have a solvent exposed reactive group for conjugation. This site can be determined through cocrystal structure, SAR analysis, or homology models. Although a variety of synthetic approaches can be employed, NanoBRET(TM) dyes prepared as activated esters can be readily conjugated to the scaffold via a primary or secondary aliphatic amine. These amine groups have been shown to react quickly and quantitatively with activated ester dyes and amino acid linkers.
A variety of dye classes have been evaluated in BRET assay formats, and dyes representing two fluorophore classes (Fig. 2a) have been identified that demonstrate consistently robust cell permeability and optimal spectral overlap for energy transfer. Derivatives containing varied linkers and dyes may perform differently in the assay (examples provided in Fig. 2). Therefore, as a starting point for assay development, it is initially recommended that at least four derivatives be prepared and evaluated in the BRET configuration: Minimal/no linker derivatives conjugated to NanoBRET™ 618 and NanoBRET™ 590 dyes and extended linkers (e.g., multi-PEG or alkyl derivatives) conjugated to NanoBRET™ 618 and NanoBRET™ 590 dyes. This panel of tracer candidates can be created from common intermediates and will provide structural diversity required to ensure the highest probability of success, and if required, guide further optimization. To serve as examples, these principles have been employed to create a panel of candidate cellpermeable tracers based on crizotinib, a multikinase inhibitor scaffold (Fig. 3).

Example Synthesis of Amine-Linked Tracers
1. Charge the small molecule precursor, functionalized with an amine, (9.9 μmol) into a 5 mL amber vial.
4. Add 5.0 mg NanoBRET™ 590 SE. Cap and allow to react in the dark for 1 h.

5.
Monitor the reaction for consumption of the starting amine by analytical HPLC. The reaction is judged complete when this material has been consumed. The reaction progresses quickly and is often near completion after 30 min (see Note 1).
6. Dilute the crude mixture with the reaction quenching solution.
7. Purify the compound using reverse-phase preparative HPLC. Most tracers can be purified using standard HPLC methods.
Use a gradient of trifluoroacetic acid (TFA) HPLC Buffer (or 0.1% formic acid in water) in acetonitrile as an eluent.
8. Pool product containing fractions and concentrate to dryness under reduced pressure.
9. Dissolve the resulting film in approximately 10 mL acetonitrile and concentrate to dryness a total of three times (see Note 2).
10. Dry the resulting film for a minimum of 1 h to remove trace volatile solvents.
11. Dissolve the resulting solid in an appropriate volume of DMSO to give a 2.0 mM solution.

Verification of Tracer Permeability and Optimization of BRET
BRET is highly sensitive to molecular distance and orientation between the donor (luciferase) and acceptor (fluorescent tracer) partners. This feature enables a bona fide measurement of direct molecular interactions inside intact cells. However, optimization may be warranted to identify the conditions producing optimal BRET between the donor/acceptor partners. This can generally Fig. 3 Chemical structures of four candidate tracer derivatives based upon the crizotinib scaffold. Similar dye/linker variants can be created for a wide variety of base molecules by conjugation to solvent exposed primary or secondary amines be achieved without a laborious effort, via transient transfection of plasmids encoding target/NanoLuc(R) fusion proteins (see Note 3) [4]. The following basic protocol can be used to determine the optimal orientation of NanoLuc(R) luciferase for target engagement analysis via BRET. It is generally recommended that novel NanoBRET(TM) tracers are evaluated in both live cells, as well as permeabilized cells (via addition of digitonin or Passive Lysis buffer), to assess tracer affinity in the absence of interfering cellular factors. Figure 4 provides an example where the protocol is used to determine the optimal tracer for a kinase target, and Figs. 5 and 6 provide examples wherein the protocol is used to determine optimal NanoLuc(R) fusion orientation or expression level, respectively. 1. Cultivate desired cells (e.g., HEK293) appropriately prior to assay and resuspend cells into a single-cell suspension using complete cell culture medium.
2. Adjust the cell density to 2 Â 10 5 /mL in cell culture medium in a sterile, conical tube.  4. Prepare transfection complexes using the manufacturer's protocol.
6. Dispense cells/lipid-DNA complex into a sterile tissue culture flask, and incubate at least 20 h to allow expression to occur. We recommend a cell density of approximately 55,000-80,000 cells/cm 2 during the transfection (for example use approximately 4À6 million cells for a T75 flask). Larger or smaller bulk transfection should be scaled accordingly, using this ratio. As described above (see Subheading 3.2), the basic protocol details the measurement of the intracellular engagement potency (IC 50 of BRET attenuation) of a test compound at a single concentration of tracer. In general, compound affinity is measured under steadystate conditions between the test compound, the tracer, and the intracellular target protein. For the simple determination of compound rank-order affinity, it is recommended to use the tracer at a fixed concentration approximating 50À80% occupancy at the target. However, tracers can be exploited to provide a more quantitative apparent affinity value, as engagement potency is often dependent on the concentration and affinity of the tracer used in the assay. As the tracer and test compound bind to the target in a competitive and mutually exclusive manner, the relationship between the apparent IC 50 of the test compound and the concentration of tracer used in the assay is governed by the Cheng-Prusoff Equation [8] (Eq. 2).
Equation 2 provides the quantitative capability to extract an apparent dissociation constant (K i,app ) for the test compound. This analysis yields a value that is insensitive to tracer concentration. Considering the limits of Eq. 2 with respect to tracer concentration, in situations where the concentration of tracer is much less than its affinity (K d,app ), the measured IC 50 for the test compound will generally be within twofold of the K i,app (i.e., if [tracer] << K d, app , then IC 50 ffi K i,app ). Conversely, when the concentration of tracer increases above the K d,app , the apparent IC 50 value of the test compound shifts to higher concentrations.
The Cheng-Prusoff relationship can be used to determine the K i,app for a test compound in multiple ways. For example, if the apparent affinity of the tracer (K d,app ) has already been measured, Eq. 2 can be used to convert an IC 50 value measured at a single, known concentration of tracer to the K i,app for the test compound. Alternatively, Eq. 2 can be algebraically linearized (Eq. 3) and used experimentally to extract the K i,app , a method known as linearized Cheng-Prusoff analysis [9]. In practice, the apparent IC 50 value for the test compound is measured at multiple tracer concentrations, after which the IC 50 values are replotted as a function of tracer concentration. Regression analysis yields a linear plot with a y-intercept equal to the K i,app , and slope equal to K i,app /K d,app . Figure 7 provides examples in which linearized Cheng-Prusoff analysis was used to quantify the K i,app for the binding of the broad spectrum bromodomain inhibitor bromosporine to NanoLuc-bromodomain fusions.
The linearized Cheng-Prusoff analysis is generally recommended for determinations of K i,app for test compounds, particularly if binding of the tracer is saturable. For targets where tracer binding is weak and not saturable, but signal window (SW) is still adequate for IC 50 determination (in practice, SW ! 1.6), the measured IC 50 will often be a good approximation for the K i,app (generally within twofold, as discussed above) (see Note 6).

Liquid Handling Requirements and
Considerations for High-Throughput Screening (HTS) and Lead Optimization Cellular target engagement assays can provide critical information for hit prioritization at both the HTS and lead optimization stages, particularly when the biochemical and cell-based assays fail to correlate. Accordingly, compounds that are similarly active in biochemical, cellular target engagement, and cellular activity assays can be assigned highest priority, while those that are very weak or inactive in a cellular target engagement assay, yet active in the other two formats, should be binned as suspicious. Such compounds are likely to trigger cellular activity assay inhibition through indirect effects. A sensitive cellular target engagement assay may also show correlative activity with the biochemical assay for certain compounds, yet fail to demonstrate cellular activity. In this case, the compound or compound series may be valid, yet require chemical optimization to allow cellular activity. It would therefore be valuable to apply the NanoBRET™ target engagement assay for HTS and as a key aid for dissection of mechanism in lead optimization.
It is possible to configure the steps and equipment to higher throughput, in order to enable efficient intracellular target engagement-based HTS and lead optimization. In order to afford the throughput required for HTS and lead optimization, several steps to streamline the NanoBRET™ process are suggested. Strategies to maximize efficiency include switching from 96-well to 384-well format to reduce the number of plates required and the plate "real estate" occupied by controls, reducing the number of steps by using assay-ready plates, and implementation of robotic liquid handling protocols. Preparation of assay-ready plates requires acoustic droplet liquid dispensing technology. While relatively expensive, it is becoming increasingly available in core facilities within both academic and industrial research centers.
It is recommended that each 384-well plate contain a set of controls occupying one entire row of 24 wells and comprising a dose response with a 12-point concentration range. Be sure to include appropriate controls including a zero BRET control (i.e., no tracer) as well as a "BRET specificity control" (i.e., a high concentration of a control inhibitor in the presence of tracer) (see Notes 7 and 8). Table 1 summarizes the results of target engagement analysis for a panel of full-length intracellular kinases in a scaled format (i.e., automated, 384-well format). As a measure of statistical robustness, each assay yielded a Z' above 0.4, supporting suitability in HTS work flows. As a future direction, scaling the BRET technique to higher density (e.g., 1536-well plates) may be possible.

Aliquot test and control compound stocks in 100% DMSO at
high concentration (typically either 5 or 10 mM depending on desired final assay concentration of 10 or 20 μM, respectively) to acoustic dispense qualified mother plates. Depending on equipment, one or more additional dilutions likely are required.
2. Adjust instrument to dispense 80 nL of highest concentration, then 1:3 dilutions using 100% DMSO as backfill in order to create a 12-point dilution series of 80 nL total volume in each well. Since the lowest dispense amount may be 5 nL, several intermediate dilutions of the initial 5 or 10 mM stock likely are required to achieve the required dispenses.
3. Seal plates tightly and store at 4 C until day 2 of assay.

Optimization of Energy Transfer for Residence Time Studies in Live Cells
Although equilibrium-based analysis is predictive of engagement in a closed system (i.e., conditions of static drug concentrations), nonequilibrium analysis may better predict target occupancy in open systems, where drug concentrations are dynamic. The compound residence time (i.e., k off À1 ) may better dictate target occupancy in the dynamic regime of a living organism [10,11]. The energy transfer technique can be readily configured to measure real-time binding kinetics in live cells, thus providing an approach to assess drug residence in an artificial open system. The open system can be simulated by applying an acute treatment of test compound to the cells, followed by removal of unbound compound and a real-time measurement of residence time using energy transfer (Fig. 8).
Prior to performing a residence time analysis, it is important to determine a few key parameters. First, it is important to select an optimal tracer and determine a working concentration of the tracer for BRET measurement after compound washout. In general, it is recommended to use a saturating concentration of tracer that has fast association and dissociation kinetics with the target of interest. While this may be achievable in practice, the binding of the tracer might not be saturable for some targets. Thus, it is important to optimize the association kinetics at the highest tracer concentration possible. For new tracers and/or new target combinations, it is recommended to initially evaluate the kinetic parameters in a dose-responsive manner to ensure that an optimal tracer and working concentration are selected for the downstream residence time analysis. This is accomplished via observed rate constant (k obs ) analysis, wherein the establishment of BRET at the target is measured kinetically over time at increasing tracer concentrations. Subsequently, the k obs is determined by nonlinear regression analysis of the kinetic curves for each tracer concentration using the one-phase association equation (Eq. 4), assuming pseudo-first order association [12]. The k obs values are replotted with respect to tracer concentration, which yields a linear relationship. Fitting Eq. 5 to the data allows dissection of the k on (from the slope) and k off (from the y-intercept) of the tracer. Figure 9 provides an example in which a k obs analysis is performed to choose between two different tracers for kinetic analysis of the BRD9 Bromodomain.
Generally, higher values of both k on and k off are desired for residence time analysis to ensure that the tracer binding is at equilibrium with the target at any given time once the test compound dissociates. However, in many cases, a simple comparison of the Fig. 9 Kinetic optimization of bromodomain tracers. HEK293 cells transiently expressing NanoLuc(R)-BRD9 bromodomain were seeded into 96-well plates, after which a dilution series of tracer was added and the BRET measured kinetically. Panels A and B depict tracer association curves for two different bromodomain tracers. Individual points represent the mean of three technical replicates. Nonlinear regression analysis using the one-phase association equation (Eq. 4) was performed to extract an observed rate constant (k obs ) at each tracer concentration. Observed rate constants were replotted with respect to tracer concentration (panel C), yielding linear relationships. Kinetic parameters extracted by linear regression using Eq. 5 are tabulated in panel D. Tracer 2 gave faster association and dissociation kinetics compared to tracer 1 and was chosen for downstream residence time analyses at a working concentration of 1 μM relative k obs value itself may be sufficient to select an optimal tracer among a few lead candidates. Though equilibration for tracers may vary greatly (nearly instantaneous to hours), equilibration of the tracer at the target within 20À30 min is sufficient for a qualitative assessment (i.e., rank-order assessment) of test compound residence time.
After the tracer and working concentrations are established, it is recommended to determine an appropriate acute dose of the test compound, as well as the length of time required to achieve equilibration with the target in the cellular context (see Note 9). Figure 10 provides an example for the determination of the acute dose and equilibration time for the binding of two test compounds to the histone deacetylase, HDAC1. Figures 11 and 12 provide example residence time analyses for the binding of the same two test compounds at HDAC1, with cell permeabilization controls to evaluate the effect of intracellular trapping, respectively. Fig. 10 Determination of optimal inhibitor concentrations for compound treatment prior to residence time analysis. BRET analysis was performed in real-time to determine an appropriate equilibration time and inhibitor concentration for cellular washout experiments. In general, an inhibitor concentration approximating 90% occupancy (e.g., 10À20Â K i,app ) is optimal prior to washout studies. (a) For HDAC1, equilibration with SAHA was proven to be rapid, indicating that a concentration of 1 μM SAHA is suitable following a short incubation time. (b) For FK228, equilibration kinetics were slower, indicating that a dose of 100 nM is appropriate, and 3 h of equilibration is required to achieve HDAC1 occupancy 3.5.1 Adding Test Compound to Cells 1. After transfecting cells (as described in Subheading 3.2.1), resuspend cells using prewarmed assay medium (e.g., Opti-MEM without serum or phenol red).
2. Adjust the density to 2 Â 10 5 cells/mL in assay medium in a 15 mL sterile polypropylene conical tube. We recommend a minimum volume of 1 mL of cells, ideally 5 mL of cells.  3. Prepare test compound at 10Â final concentration in appropriate solvent (e.g., 1% DMSO).

4.
To determine the optimal concentration of test compound for residence time analysis, it is recommended to first determine the compound IC 50 using the equilibrium-based Target Engagement Protocol (see Subheading 3.2.2). Introduce the test compound at a final concentration of 10-20Â K i,app determined under equilibrium conditions. This insures that adequate washout conditions can be achieved prior to off-rate measurements. Add 100 μL of 10Â test compound to each 1 mL of cells in assay medium and mix gently.
(Optional) Include a positive control treatment of a compound at a high and saturating dose as a full-occupancy control, as well as a negative control treatment with compound vehicle.
5. Place the conical tube in a rack, and incubate the tube with the cap loosened at 37 C, 5% CO 2 for a minimum of 2 h or until sample is expected to reach equilibrium. 7. Immediately proceed to the next step (see Subheading 3.5.4).

BRET Detection in Kinetic Mode
1. Set a NanoBRET™ Assay-compatible instrument to perform repeat measurements for the desired time interval. As a starting point, use 5-min intervals between each measurement, and be sure to include a sufficient number of measurements to determine compound dissociation. Set the instrument at 25 C to minimize sample evaporation. However, as temperature may impact residence time profiles, it may be valuable to evaluate physiological temperatures.

Adapting the Residence Time Protocol to Adherent (ADH) Format
In addition to the residence time protocol described above, residence time analysis can be performed in adherent (ADH) format in which the cells are adhered to a tissue culture-treated assay plate and the compound incubations are performed directly in that assay plate. Adherent format has both benefits and drawbacks compared to the conventional format in the nonbinding surface assay plate (NBS format) described above that include the ability to test significantly more experimental conditions simultaneously (test compound concentrations and/or targets), and improved workflow for washout that reduces time between the initial washout and the tracer addition step and preserves kinetic information at early time points. However, in some cases the kinetics of the BRET signal may not achieve a constant value under steady state conditions, or may appear biphasic compared to those assessed in NBS-treated plates.
Users should consider their specific goals for the residence time analysis to help select between the assay formats. Figure 13 depicts an example residence time determination for dasatinib and ibrutinib at BTK kinase in both NBS and ADH formats for comparison. 13. Immediately measure BRET in kinetic mode as described in Subheading 3.5.4 in the protocol for residence time in NBS format.
14. Process data as described above in the protocol for residence time in NBS format (see Subheading 3.5.4).

Notes
1. Progress of the reaction can be monitored by analyzing a small aliquot every 15 min. Additional time may be required to achieve satisfactory results. Slow reaction can often be remedied by adding an additional 8.6 μL portion of diisopropylethyl amine. Overnight reaction is not recommended.
2. It is recommended that fraction pools be concentrated to dryness under reduced pressure. Coevaporation with acetonitrile will help remove spurious residual TFA that has been shown to affect the stability of some tracers. Lyophilization has been shown to enhance this effect during freeze-drying and is not recommended.
3. When possible, placement of the luciferase reporter at both termini of the target protein is recommended to identify the optimal donor orientation. Installation of a 4À10 residue linker between the target and luciferase reporter is also recommended. Standardized poly Gly/Ser linkers (e.g., Gly-Ser-Ser-Gly) are commonly used to ensure some level of flexibility between the target and the reporter. Although a variety of vectors can be configured for such purposes, common mammalian expression vectors such as pFN-31K or pFC-32K are predesigned for NanoBRET(TM).
4. It is recommended that the maximum concentration of tracer used at this stage is 0.4 mM so that the maximum concentration on cells does not exceed 4 μM. This is typically the solubility limit of cell-permeable NanoBRET(TM) tracers, so higher concentrations in culture medium should be avoided.
5. The Extracellular NanoLuc(R) inhibitor is recommended for live cell analysis as a means to inhibit any Nluc signal arising from targets in cell culture debris. For experiments with cell lysates, it should be omitted.
6. When planning the linearized Cheng-Prusoff analysis, it is important to consider the concentration range of both tracer and the test compound. Ideally, both will be used at or below the associated solubility threshold. When these thresholds are surpassed, deviations in linearity in the regression analysis are commonly observed, thus complicating quantitative analysis with NanoBRET(TM). When choosing tracer concentrations, it is ideal to include concentrations both above and below the K d,app , typically in the range of 0.25À20Â K d,app . This ensures adequate competition and establishment of the linear rightshifting of test compound IC 50 . As the analysis requires linear regression, linear spacing of the tracer concentration is ideal, although not always practical. Hence, a twofold dilution series of the tracer is often used to bracket the K d,app . In the case of the test compound, generally an 11-point, threefold dilution series is most appropriate for capturing the IC 50 values, often starting at 50Â the apparent IC 50 at a particular tracer concentration, or 1000À2000Â the K i,app of the test compound for a full analysis. In situations where a new test compound/tracer combination is being evaluated, it is often practical to perform a pilot analysis with a twofold dilution series of tracer starting in the range of 1À4 μM and a threefold dilution series of the test compound starting in the range of 10À20 μM, after which the concentration ranges can be adjusted as needed.
7. When test compounds are applied to the plate in 12-point concentration dilution, as many as 30 IC 50 curves can be determined on a single 384-well plate. If duplicate dose-response curves are determined on a single plate and a duplicate control compound dilution series also is run on every plate for interplate and interday statistical comparisons, then a reasonable throughput of 14 compounds per plate can be achieved. The NanoBRET™ signal is stable for at least 60 min; therefore at least 15-20 plates can be filled and scanned efficiently using appropriate bulk dispensing equipment without loss of signal between reading the first and last plates.
8. Adapting the competitive displacement format to high throughput requires additional tactics to assure consistency plate-to-plate and day-to-day. These include normalizing the amount of DMSO in every well and freezing many vials of cells at the same passage number. The robustness of this format should be assessed by repeating tracer dose response and dose response for a selected control test compound on multiple plates, on different days, with different transient transfections, and using cells with different passage numbers or different vials of frozen cells. Test-retest Minimum Significant Ratio (MSR) and moving MSR values should be within threefold in each repeat assay [13]. As is typical for assay development and daily evaluation, assay behavior also should be evaluated using Z' values. With appropriate assay development, the highthroughput format behaves essentially identical to the 96-well standard format. Tracer dose response K d,app , signal-background ratio, and Z' values have been found to be comparable between 96-and 384-well plate formats for multiple different kinase NanoBRET(TM) assays studied, for example. Table 1 illustrates data for ten archetypal enzymes across multiple kinase classes. In each case, the 384-well assay was developed, and the statistical effect size (measured as Z') is acceptable for HTS and lead optimization. There is no need to first develop and optimize an assay in 96-well format prior to adapting 384-well format.
9. The acute dose can be determined by measuring the K i,app or IC 50 of the test drug according to the protocols described above in Subheadings 2 and 3. Once determined, we recommend an acute dose of 10À20Â K i,app or IC 50 for the residence time analysis, which balances both meaningful binding of the test compound to the target of interest (approximately 90% occupancy) as well as the ability to wash away the compound after equilibration. To determine an appropriate equilibration time, it is recommended to monitor the affinity of the test compound to the target over time, and select a sufficient amount of time for stabilization of the IC 50 value (indicative of equilibration). The binding of many test compounds will reach equilibrium with the target within 2À3 h in a cellular context, although the incubation time might require adjustment for poorly permeable compounds.