Two Gαi1 Rate-Modifying Mutations Act in Concert
to Allow Receptor-Independent, Steady-State
Measurements of RGS Protein Activity
THOMAS ZIELINSKI,1 ADAM J. KIMPLE,2 STEPHANIE Q. HUTSELL,3 MARK D. KOEFF,1
DAVID P. SIDEROVSKI,2,4,5 and ROBERT G. LOWERY1
RGS proteins are critical modulators of G-protein-coupled receptor (GPCR) signaling given their ability to deactivate Gα
subunits via GTPase-accelerating protein (GAP) activity. Their selectivity for specific GPCRs makes them attractive therapeutic targets. However, measuring GAP activity is complicated by slow guanosine diphosphate (GDP) release from Gα and
lack of solution phase assays for detecting free GDP in the presence of excess guanosine triphosphate (GTP). To overcome
these hurdles, the authors developed a Gαi1 mutant with increased GDP dissociation and decreased GTP hydrolysis rates,
enabling detection of GAP activity using steady-state GTP hydrolysis. Gαi1(R178M/A326S) GTPase activity was stimulated
6- to 12-fold by RGS proteins known to act on Gαi subunits and not affected by those unable to act on Gαi, demonstrating that
the Gα/RGS domain interaction selectivity was not altered by mutation. The selectivity and affinity of Gαi1(R178M/A326S)
interaction with RGS proteins was confirmed by molecular binding studies. To enable nonradioactive, homogeneous detection of RGS protein effects on Gαi1(R178M/A326S), the authors developed a Transcreener fluorescence polarization immunoassay based on a monoclonal antibody that recognizes GDP with greater than 100-fold selectivity over GTP. Combining
Gαi1(R178M/A326S) with a homogeneous, fluorescence-based GDP detection assay provides a facile means to explore the
targeting of RGS proteins as a new approach for selective modulation of GPCR signaling. (Journal of Biomolecular
Screening 2009:1195-1206)
Key words: fluorescence polarization, GDP detection, regulators of G-protein signaling, surface plasmon resonance
INTRODUCTION
T
HE STANDARD MODEL OF G-PROTEIN-COUPLED RECEPTOR
(GPCR) SIGNAL TRANSDUCTION had long been restricted
to a 3-component system: receptor, G-protein, and effector.1 The
7-transmembrane domain receptor is coupled to a membraneassociated heterotrimeric complex composed of a guanosine
triphosphate (GTP)–hydrolyzing Gα subunit and a Gβγ dimeric
partner. Agonist-induced conformational changes enhance the
guanine nucleotide exchange activity of the receptor, leading to
the release of guanosine diphosphate (GDP) (and subsequent
binding of GTP) by the Gα subunit. On binding GTP, conformational changes within the 3 “switch” regions of Gα allow the
release of Gβγ. Separated Gα⋅GTP and Gβγ subunits are then
1
BellBrook Labs, Madison, Wisconsin.
Departments of 2Pharmacology, 3Biochemistry & Biophysics, 4Lineberger
Comprehensive Cancer Center, and 5UNC Neuroscience Center, University of
North Carolina at Chapel Hill, Chapel Hill.
Thomas Zielinski and Adam J. Kimple contributed equally to this work.
Received Mar 28, 2009, and in revised form Aug 1, 2009. Accepted for publication Aug 4, 2009.
Journal of Biomolecular Screening 14(10); 2009
DOI: 10.1177/1087057109347473
© 2009 Society for Biomolecular Sciences
free to propagate intracellular signaling via diverse effectors.2
The intrinsic GTP hydrolysis (GTPase) activity of Gα resets the
cycle by forming Gα⋅GDP, which has low affinity for effectors
but high affinity for Gβγ. In this way, the inactive, GDP-bound
heterotrimer (Gα⋅GDP/Gβγ) is reformed and capable once again
to interact with activated receptor.
Based on this cycle of receptor-catalyzed GTP exchange and
intrinsic GTP hydrolysis by Gα, the duration of heterotrimeric
G-protein signaling is thought to be controlled by the lifetime of
the Gα subunit in its GTP-bound state. After the establishment
of this basic model,1 RGS proteins (regulators of G-protein signaling) were subsequently discovered3-5 to bind Gα subunits (via
a conserved ~120–amino acid RGS domain) and dramatically
accelerate their intrinsic GTPase activity,6 thereby attenuating
heterotrimer-linked signaling. Nearly 40 human proteins contain
at least 1 RGS domain, with many of these proteins (e.g., RGS4,
RGS16) serving as GTPase-accelerating proteins (GAPs) for
Gαi/o subunits, yet others such as RGS2 and p115-RhoGEF are
particularly attuned to Gαq/11 and Gα12/13 substrates, respectively.7
The discovery of this superfamily of Gα-directed GAPs resolved
apparent timing paradoxes between observed rapid physiological
responses mediated by GPCRs and the slow hydrolysis activity
of the cognate G-proteins seen in vitro. Thus, in this capacity as
negative regulators of GPCR signal transduction, the RGS
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proteins present themselves as excellent potential drug discovery targets.7 For example, pharmacological inhibition of RGS
domain GAP activity should lead to prolonged signaling from
G-proteins activated by agonist-bound GPCRs.
The most direct way to detect RGS protein function is by
measuring the increased GTPase activity exhibited by its target
Gα protein. However, accurate in vitro measurements of
Gα-catalyzed GTP hydrolysis are difficult to obtain without
laborious biochemical reconstitutions with purified Gβγ and an
activated GPCR (e.g., Ingi et al.8). In the absence of GPCRmediated nucleotide exchange, it is GDP release (rather than
GTP hydrolysis) that is the rate-limiting step in the Gα nucleotide cycle.9 Thus, to examine the effect of an RGS protein in
accelerating GTP hydrolysis by an isolated Gα subunit in vitro,
a single round of hydrolysis of radiolabeled GTP is usually
performed (aka the “single-turnover GTPase assay”; Berman
et al.6). This standard assay for measuring RGS domain-mediated
GAP activity is low throughput and requires discrete steps of
[γ-32P]GTP loading onto Gα, protein reactant admixture (with
addition of the critical cofactor Mg2+ to initiate hydrolysis),
isolation (in discrete time intervals) of released [32P]phosphate
with activated charcoal precipitation and centrifugation, and
finally scintillation counting. We have described an alternative
single-turnover GTPase assay10 using a coumarin-labeled, phosphate-binding protein to facilitate fluorescence-based detection
of inorganic phosphate production; however, this method demands
stringent controls on multiple experimental steps to eliminate
phosphate contaminants that interfere with the detection of
GTPase activity. Such convoluted protocols of inorganic phosphate detection are difficult for the nonspecialist and especially
not suited for high-throughput screening (HTS) of large compound libraries for RGS domain inhibitors. We and others have
reported alternative, fluorescence-based strategies for detecting
the binding between RGS protein and Gα substrate,11-13 but none
has specifically facilitated a discrete endpoint measurement of
RGS domain-mediated GAP activity per se.
To develop a facile steady-state GTPase assay for RGS domain
GAP activity, we first set out to increase the spontaneous GDP
release rate of Gα (koff(GDP)) while also decreasing its intrinsic
rate of GTP hydrolysis (kcat(GTPase)), thereby allowing detection
of at least a 5-fold enhancement of steady-state GTP hydrolysis
by RGS proteins to provide an adequate signal-to-noise ratio.
Gαi1 and closely related Gα proteins have been the focus of
extensive structure/function studies,14-17 and point mutations
that affect both koff(GDP) and kcat(GTPase) without affecting functional interaction with the RGS domain have been identified
previously15-18 (e.g., Fig. 1A). Two of the most striking Gα
mutations have been made to the highly conserved active-site
arginine (R178C; Coleman et al.15), which causes a ~100-fold
reduction in GTPase activity, and to the alanine residue within
the conserved TCAT loop that contacts the guanine ring
(A326S; Posner et al.16), which results in a ~25-fold increase in
koff(GDP) relative to wild-type yet an identical kcat(GTPase).
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To detect RGS protein-accelerated GTPase activity, we
adapted a monoclonal antibody and fluorescent tracer, previously developed for the Transcreener adenosine diphosphate
(ADP) assay,19 for selective immunodetection of GDP with a
fluorescence polarization readout. Measurement of GTPase
activity using this Transcreener GDP assay overcomes the
signal-to-noise limitations of phosphate detection methods and
has been validated as a robust HTS method in the case of ADP
detection for kinases and ATPases.20-22 Moreover, because it is
a catalytic assay rather than a substrate-binding assay, it should
enable detection of all types of modulators of RGS protein
GAP activity, including those that bind at allosteric sites and
affect RGS protein-catalytic activity without directly targeting
the RGS domain Gα binding site.23
In this present study, we tested multiple-point mutant Gαi1
proteins with increased GDP dissociation and/or decreased GTP
hydrolysis rates for their ability to enable detection of RGS
domain GAP activity using a steady-state GTPase assay format
(i.e., multiple rounds of turnover of GTP to GDP). Coupling one
of these variants, Gαi1(R178M/A326S), to the Transcreener
GDP detection system has not only allowed facile detection of
RGS protein GAP activity but also was useful in helping establish (along with surface plasmon resonance spectroscopy) that
the mutant Gαi1 interacted with RGS proteins with the same
specificity and affinity as the wild-type Gαi1 protein.
MATERIALS AND METHODS
Chemicals and assay materials
GDP and GTP were purchased from USB Corp. (Cleveland,
OH). The monoclonal antibody and tracer used for GDP detection were developed at BellBrook Labs (Madison, WI) as
described,19 with the tracer comprising ADP conjugated to
Alexa Fluor 633 (Invitrogen/Molecular Probes, Carlsbad, CA).
Unless otherwise specified, all additional reagents were of the
highest quality obtainable from Sigma (St. Louis, MO) or
Fisher Scientific (Hampton, NH).
Protein expression and purification
Wild-type, full-length human Gαi1 and various RGS proteins used in these studies were expressed in Escherichia coli
and purified as previously described.24 Gαi1 point mutants
were created using PCR-based site-directed mutagenesis
(QuikChange II, Stratagene, La Jolla, CA) on the wild-type
pProEXHTb-Gαi1 expression vector; mutagenesis primers
were designed using Stratagene’s QuikChange primer design
program and synthesized/PAGE purified by Sigma-Genosys.
All mutant constructs were sequence verified at Functional
Biosciences LLC (Madison, WI) before protein expression,
purification, concentration, quantitation, and cryopreservation
using established protocols.10,24
Journal of Biomolecular Screening 14(10); 2009
Fluorescent Steady-State RGS Protein GAP Assay
FIG. 1. Increased guanosine diphosphate (GDP) release and decreased guanosine triphosphate (GTP) hydrolysis of the Gαi1(R178M/A326S)
mutant compared to wild-type Gαi1 and single-point mutants, as measured by [35S]GTPγS binding and single-turnover [γ-32P]GTP hydrolysis,
respectively. (A) Point mutations to Gαi-family subunits previously reported in the literature15-18 to alter intrinsic GTP hydrolysis and GDP dissociation rates. (B) Binding of [35S]GTPγS to wild-type or indicated mutant Gαi1 subunits. (C) Single-turnover GTP hydrolysis activities of
wild-type or indicated mutant Gαi1 subunits. (D) Initial rates of GTP binding and hydrolysis for the Gαi1(R178M/A326S) mutant, as well as other
Gαi1 point mutants derived from data similar to that of panels B and C.
Radiolabeled nucleotide binding and
single-turnover GTPase assays
Assessments of spontaneous GDP release and single-turnover
GTP hydrolysis rates by wild-type and mutant Gαi1 subunits,
using measurements of [35S]GTPγS binding and [γ-32P]GTP
hydrolysis, respectively, were conducted exactly as previously
described.24,25 Briefly, for [35S]GTPγS binding by 100 nM of
Gαi1 subunits at 20 °C, timed aliquots were removed, filtered
through nitrocellulose, and washed 4 times with 10 mL of wash
buffer before scintillation counting. Assays were conducted in
duplicate, counts were subtracted from analogous reactions in
“nonspecific binding” buffer,24 and normalized data were plotted as mean ± SEM. For single-turnover [γ-32P]GTP hydrolysis
assays, Gαi1 subunits (100 nM) were prebound to [γ-32P]GTP in
the absence of Mg2+ for 10 min at 30 °C. Reactions were then
initiated by the addition of 10 mM MgCl2 (final concentration),
and the production of 32Pi was measured by activated charcoal
filtration and liquid scintillation counting.9,25 Initial rates were
obtained by data analysis using GraphPad Prism (La Jolla, CA).
Radiolabeled nucleotide steady-state GTPase assays
Assessments of steady-state [γ-32P]GTP hydrolysis rates by
wild-type and mutant Gαi1 subunits were conducted essentially
as previously described.26 Briefly, Gαi1 protein was diluted to
Journal of Biomolecular Screening 14(10); 2009
50 nM in a buffer containing 50 mM Tris (pH 7.5), 100 mM
NaCl, 0.05% C12E10, 1 mM dithiothreitol (DTT), 5 mM EDTA,
10 mM MgCl2, and 5 µg/ml bovine serum albumin (BSA).
Assays were initiated with the addition of [γ-32P]GTP (and
RGS4 if used), aliquots stopped at indicated time intervals, and
free [γ-32P]Pi quantified as previously described.26
Transcreener GDP assays
Standard curves and GTPase reactions were both run at
30 °C in kinetic mode on a Tecan Safire2 multiwell reader in
Corning 384-well black round-bottom, low-volume polystyrene nonbinding surface microplates (part 3676). Fluorescence
polarization was read using 635-nm excitation (20 flashes per
well) and 670-nm emission. A free tracer reference was set to
20 mP by adjusting the photomultiplier tubes, and buffer containing GDP antibody alone was used as a blank for sample and
reference wells. EC50 and EC85 values, Hill slopes, and curves
were generated by GraphPad Prism. Unless otherwise indicated, reactions were run in 20 mM Tris (pH 7.5), 1 mM EDTA,
10 mM MgCl2, 10 µM GTP, 8 µg/mL GDP antibody, and 2 nM
tracer in a final 20-µL volume. GDP antibody was used at a
concentration 85% of the amount required for saturated binding
to tracer (i.e., the EC85). Where shown, polarization data were
converted to the amount of GDP produced using standard
curves. Reaction rates were then determined in GraphPad
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Prism using linear regression to estimate slope. For GTPase and
GAP assays, reactions were started with the addition of GTP
with or without RGS protein.
Compound interference test
To assess the robustness of the Transcreener GDP assay for
practical screening applications, we performed a control screen
using the GenPlus library of 960 bioactive molecules from Microsource Discovery Systems, many of which are approved drugs.
GDP assay reagents (as denoted above) were added to duplicate
wells containing 10 µM compound and either 10 µM GTP to
mimic no-enzyme control reactions or 9 µM GTP plus 1 µM
GDP to mimic completed enzyme reactions in 1% DMSO.
Pilot screen and counterscreen of GenPlus Library
Screens of the GenPlus library with the Transcreener GDP
assay (10 µM final compound concentration) for modulators of
RGS4 GAP activity on Gαi1(R178M/A326S), as well as for nonspecific modulators of intrinsic GTPase activity of Gαi1(R178M/
A326S) alone, were conducted as mentioned above with the following changes. GTPase reactions containing 50 nM Gαi1(R178M/
A326S) with or without 250 nM RGS4 were run in Corning
384-well microplates at 30 °C in 20 mM Tris (pH 7.5), 1 mM
EDTA, 10 mM MgCl2, 10 µM GTP, 12 µg/µL GDP antibody, 2
nM tracer, and 0.5% DMSO (v/v) in a final volume of 20 µL.
Fluorescence polarization was read at 60, 90, 120, and 180 min
of elapsed reaction time on a Tecan Safire2 multiwell reader as
described above.
Surface plasmon resonance spectroscopy
Optical detection of surface plasmon resonance (SPR) was
performed using a BIAcore 3000 (GE Healthcare, Piscataway,
NJ). Wild-type and mutant Gαi1 proteins were immobilized onto
nickel-nitrilotriacetic acid SPR sensor chips (GE Healthcare) by
hexahistidine tag-mediated capture coupling as previously described.27 Affinities of RGS proteins for immobilized Gαi1 proteins
were obtained from dose-response sensorgrams using equilibrium
saturation binding analyses as previously described.24
RESULTS AND DISCUSSION
Profiling multiple Gαi1 point mutations
for nucleotide cycling rate alterations
Using PCR-based site-directed mutagenesis, we created
several amino acid substitutions at various positions within
Gαi1 known to affect koff(GDP) and/or kcat(GTPase) (e.g., Fig. 1).
These mutants included aspartate, serine, or threonine replacing Ala-326; cysteine, lysine, or methionine replacing Arg-178;
alanine, serine, or valine replacing Thr-181; single mutants
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K192A and F336A; and double mutants K192A/F336A,
R178C/A326S, R178C/A326T, R178M/A326S, R178C/A326T,
and T181A/A326S. Note that multiple different substitutions
were made at several sites, including amino acids intended to
be more or less disruptive than the original reported mutation.
For instance, R178K and R178M were tested as more conservative substitutions at the catalytic arginine position relative to
the original R178C variant; it was thought that either of these
alternative substitutions might result in a smaller decrease in
kcat(GTPase) than the cysteine replacement, which reduces kcat(GTPase)
by 2 orders of magnitude.15 Although the R178C mutation
leads to a substantial decrease in kcat(GTPase), Berman et al.6 have
shown that the single-turnover GTPase rate of this Gα mutant
can still be increased by RGS domain-mediated GAP activity,
whereas the more conventional GTPase-crippling mutation of
Q204L renders Gαi1 truly dead in terms of responsiveness to
RGS proteins. Thus, the Gαi1(Q204L) mutant was not pursued
in this study.
Gαi1 mutants were initially profiled for enhanced GDP release
and/or reduced GTPase rate sufficient to see a change in
steady-state GTP hydrolysis upon RGS protein addition. This
initial profiling led us to focus on 2 positions: Arg-178 and Ala326. Binding of the nonhydrolyzable GTP analog, [35S]GTPγS,
to Gαi1⋅GDP was used to measure the rate of GDP dissociation
(e.g., Fig. 1B); the prevailing assumption for Gα subunits is
that kon for [35S]GTPγS binding is much more rapid than
koff(GDP).28 Single-turnover GTP hydrolysis measuring 32Pi
released from Gα-bound [γ-32P]GTP—an assay format that is
not rate limited by GDP dissociation9—was used to assess
intrinsic kcat rates for the Gαi1 mutants (e.g., Fig. 1C).
As expected, Gαi1 variants with mutation to the active-site
catalytic residue Arg-178 had very low or undetectable levels
of GTP hydrolysis, whereas Gαi1(A326S), the single mutation
reported to only affect GDP dissociation, had a GTPase rate
similar to wild-type Gαi1 (Fig. 1C,D). [35S]GTPγS binding
assays showed that 2 variants with mutations only at the catalytic site, R178M and R178C, had GDP dissociation rates
similar to wild-type Gαi1, whereas introduction of the A326S
mutation, either alone or in combination with R178C, caused a
3-fold acceleration in GDP dissociation (Fig. 1B,D). When the
A326S mutation was combined with methionine at Arg-178
(instead of cysteine), the GDP dissociation rate increased more
than 10-fold over wild-type: from 0.008 min–1 to 0.130 min–1
(Fig. 1D). We currently do not have a precise structural explanation for why the particular combination of R178M and
A326S mutations results in more rapid GDP release than the
single A326S mutation alone; it is not an additive effect because
the singly mutated Gαi1(R178M) variant exhibits wild-type GDP
dissociation (Fig. 1B). It is interesting to note that Posner and
colleagues,16 when reporting the crystal structure of the
Gαi1(A326S) mutant, suggested the presence of an indirect interaction between the Arg-178 and Ser-326 residues (via contacts
Journal of Biomolecular Screening 14(10); 2009
Fluorescent Steady-State RGS Protein GAP Assay
FIG. 2. RGS4 GTPase-accelerating protein (GAP) activity is observed as an increase in steady-state guanosine triphosphate (GTP) hydrolysis
only for the rate-altered Gαi1(R178M/A326S) variant. Time courses of steady-state [γ-32P]GTP hydrolysis by (A) 50 nM Gαi1(R178M/A326S)
mutant or (B) 50 nM wild-type Gαi1 in the presence or absence of 250 nM RGS4 at 20 °C. Results are the mean (± SEM) of duplicate samples.
with nucleotide and Gly-45), thereby providing a possible
mechanism for the functional interaction we have observed
here between the R178M and A326S mutations.
Combined action of 2 Gαi1 mutations allows
steady-state measurement of GAP activity
With the R178M/A326S mutant of Gαi1 demonstrating the
largest change in GDP release rate of all mutants tested, we
next examined whether this particular Gαi1 variant would be
affected by RGS domain-mediated GAP activity in steadystate [γ-32P]GTP hydrolysis assays. Addition of purified RGS4
protein to the Gαi1(R178M/A326S) variant (in the presence of
free [γ-32P]GTP and Mg2+) resulted in a dramatic increase in
[32P]Pi detected over time. In contrast, there was no effect of
RGS4 on wild-type Gαi1 in this steady-state assay (Fig. 2A vs.
2B), as expected given the original report by Berman et al.6
Development of a Transcreener GDP assay
The Transcreener platform relies on highly selective antibodies for detection of nucleotides produced in enzyme reactions.29 To allow measurement of RGS protein-mediated
acceleration of steady-state GTP hydrolysis in a homogeneous
format without radioactivity, we developed a Transcreener
assay for GDP (Fig. 3A) using a competitive fluorescence
polarization immunoassay format. For this method, a recently
developed monoclonal antibody that recognizes GDP with
>100-fold higher affinity than GTP19 is added to the reaction,
along with a fluorescent tracer that binds to the antibody with
high affinity. When no free, unlabeled GDP is present in the
reaction, the fluorescent tracer remains antibody bound and
exhibits a high polarization given its high apparent molecular
weight. GDP produced in the reaction displaces the tracer from
Journal of Biomolecular Screening 14(10); 2009
the antibody, thereby reducing its apparent molecular weight,
increasing its rotational motion, and thus reducing the degree
of polarization of emitted light. A similar Transcreener assay
has been widely used for detection of ADP produced by kinases
and other ATP-hydrolyzing proteins (e.g., Huss et al.,20 Klink
et al.,21 Liu et al.22; reviewed in Lowery and Kleman-Leyer29).
Figure 3B shows typical fluorescence polarization standard
curves mimicking the conversion of GTP to GDP by a GTPase.
An important aspect of flexibility for a GTPase assay is the
ability to accommodate a range of initial GTP concentrations,
so that diverse enzymes and screening strategies can be employed; therefore, these studies were performed using different
GTP concentrations of 1, 10, and 100 µM. Because the antibody cross-reacts to some degree with GTP, its concentration
must be increased as higher GTP concentrations are used, to
buffer for the total guanine nucleotide pool. Thus, for this
analysis, the EC85 concentrations of monoclonal antibody were
first determined in the presence of the indicated initial GTP
concentrations (2.2, 12, and 64 µg/mL Ab for 1, 10, and 100
µM GTP, respectively), and the standard curves for GTP to
GDP conversion were performed with 16 replicates at those
antibody concentrations. At a GDP concentration equivalent to
10% conversion of GTP, which is generally considered to be
well within the initial velocity region, polarization shifts of
108, 134, and 148 mP were observed for the 1-, 10-, and
100-µM GTP concentration curves, respectively (Fig. 3B).
Acceptable Z′ factor values30 of greater than 0.5 were observed
down to 2% conversion for the 2 higher initial GTP concentrations and to 5% for the 1-µM initial GTP curve (Fig. 3C), suggesting that the Transcreener GDP assay should be capable of
very robust detection of GTPase enzyme initial velocity over at
least a 100-fold range of initial GTP concentration.
To assess the potential for compound interference with the
Transcreener GDP assay readout, we performed a control screen
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FIG. 3. Fluorescence polarization immunoassay for the detection of guanosine diphosphate (GDP). (A) Schematic representation of methodology
underlying the Transcreener GDP assay as applied to steady-state guanosine triphosphate (GTP) hydrolysis (and resultant GDP production) by a ratealtered Gα protein. Fluorescent tracer is illustrated with a jagged oval; when bound to the GDP-selective monoclonal antibody, emitted light remains
polarized, whereas there is low polarization of emitted light when tracer is displaced by free GDP. (B) The Transcreener GDP assay was used to generate standard curves for conversion of GTP into GDP at initial GTP concentrations of 1, 10, and 100 µM using appropriate EC85 concentrations of GDP
antibody established for these initial GTP concentrations (2.2, 12, and 64 µg/mL, respectively). (C) Z′ factor values, reflecting both assay signal window
and signal variability,30 were determined in 16 replicates for each of the points in the GDP detection standard curves presented in panel B. Although the
assay window was reduced at lower percent conversions (e.g., 57 mP for 3% conversion to GDP of 10 µM initial GTP; panel B), acceptable Z′ factors30
of >0.5 were observed down to 2% conversion for the 2 higher initial GTP concentrations and to 5% for the 1-µM initial GTP curve, given the very low
signal variability. (D) Control screen using the 960-compound GenPlus library. Assay components were added to duplicate wells containing 10 µM
compound and either 10 µM GTP (to mimic no-enzyme control reactions) or 9 µM GTP plus 1 µM GTP (to mimic completed GTPase reactions). The
range of signal observed (3 standard deviations about the mean; “µ ± 3σ”) in each condition is demarked with a dotted gray line.
(Fig. 3D) with the GenPlus library of 960 bioactive molecules,
many of which are approved drugs. This control screen was done
under conditions mimicking 10% conversion to GDP for a
GTPase reaction run at 10 µM initial GTP concentration. All
wells were run in duplicate. The vast majority of the compounds
clustered very tightly around the means for the 10-µM GTP and
the 9-µM GTP/1-µM GDP conditions; the Z′ factor for the nocompound controls in this screen was 0.93. Only 3 compounds in
the control screen caused the signal to vary more than 3 standard
deviations from the mean: dirithromycin, metazolamide, and
lonidamin (Fig. 3D). There is no obvious structural similarity
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between them, nor are any of them similar in structure to a guanine
nucleotide. These data suggest that compound interference with
the Transcreener GDP assay readout will be minimal.
Fluorescence polarization–based detection of RGS protein
GAP activity is dependent on 2 rate-altering mutations
Having validated the utility of the Transcreener assay in
detecting GDP in the presence of GTP, we next tested its use in
measuring RGS protein GAP activity on several rate-altered
Gαi1 variants (Fig. 4). In these experiments, the Gαi1 proteins
Journal of Biomolecular Screening 14(10); 2009
Fluorescent Steady-State RGS Protein GAP Assay
FIG. 4. RGS4 increases the steady-state GTPase activity of Gαi1(R178M/A326S) but not wild-type Gαi1, as measured using the Transcreener
guanosine diphosphate (GDP) assay and reported in absolute change in polarization (left panels) and GDP produced per Gα protein in reaction (right
panels). (A,B) R178M/A326S double-mutant and (C,D) wild-type Gαi1 proteins were present at a 50-nM final concentration. Dashed lines represent
reactions conducted in the presence and solid lines (“mock”) in the absence of 250 nM RGS4 protein. (A,C) Change in polarization (∆mP) at each
time point for indicated Gαi1 protein was calculated as ∆mP = |mP(Gαi1) – mP(no Gαi1)|. (B,D) Data from panels A and C were converted to GDP
produced per mol of input Gαi1 using previously established standard curves for GDP detection in the presence of guanosine triphosphate (GTP)
(e.g., Fig. 3B). (E) Summary of initial rates obtained by the Transcreener GDP assay for each Gαi1 mutant tested. “GAP factor” is defined as the
ratio between steady-state GTPase rate in the presence of RGS protein and steady-state GTPase rate in the absence of RGS protein.
were incubated with and without the well-characterized,
Gαi-directed RGS protein RGS431 in the presence of the
Transcreener GDP assay reagents, and plates were read at
intervals starting at 15 min. The change in the absolute value of
polarization at each time point (∆mPt = |mPt(Gαi1) – mPt(no G
αi1)|) was plotted over a time course of 6 h; in addition, the
plotted change in polarization that occurred in the linear
region (over the first hour) was converted to GDP formation
using standard curves (akin to those of Fig. 3B) and normalized to the amount of Gαi1 protein present in the reaction, with
Journal of Biomolecular Screening 14(10); 2009
the resultant initial rates of GTP hydrolysis calculated from the
data shown in Figure 4E.
The 2 Gαi1 variants with single mutations at the catalytic
arginine only, R178C or R178M, each had lower steady-state
GTPase activity than wild-type Gαi1 and, like wild-type, were
unaffected by RGS4 (GAP factors of 0.9 and 1.2, respectively;
Fig. 4E). These results are expected because their steady-state
GTPase rate is limited by slow GDP dissociation. Conversely,
the A326S variant exhibited a much higher steady-state GTPase
rate than wild-type, as expected from its higher koff(GDP) (Fig. 1);
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FIG. 5. Structural features of the RGS16/Gαi1⋅GDP⋅AlF4– complex highlighting the locations of Arg-178 and Ala-326 residue positions mutated in
the Gαi1(R178M/A326S) variant. The RGS16/Gαi1 complex (PDB id 2IK8; Soundararajan et al.24) was rendered using PyMOL with the RGS16 RGS
domain in orange and Gαi1 protein in blue, respectively. Gαi1 switch regions are depicted in gray; switches 1 and 2 (SI, SII) are visible in the foreground, whereas switch 3 is in the background and thus unlabeled. GDP is shown in magenta, the AlF4– ion is red, and the Mg2+ ion is depicted as a
yellow sphere. Residues arginine-178 and alanine-326 are rendered as “sticks” in green with CPK atomic coloring (nitrogen = blue, oxygen = red).
however, its steady-state GTPase rate was unaffected by RGS4
(GAP ratio of 1.1; Fig. 4E), presumably because a further rate
increase in GTPase is limited by koff(GDP). Most important, the 2
double mutants, R178C/A326S and R178M/A326S, had very
low basal steady-state GTPase activities that became demonstrably higher in the presence of RGS4 (e.g., Fig. 4A,B); the
GAP effect on Gαi1(R178M/A326S) was greater than with the
Gαi1(R178C/A326S) variant (GAP factors of 6.5 and 3.6,
respectively; Fig. 4E). Given its high GAP factor response in
both the steady-state [γ-32P]GTP hydrolysis assay (Fig. 2) and
the Transcreener GDP assay (Fig. 4), the Gαi1(R178M/A326S)
variant was used in subsequent analyses.
Gαi1(R178M/A326S) interacts with RGS proteins with the
same affinity and specificity as wild-type
A possible concern about the use of a mutated Gα protein for
RGS protein GAP assays is that the mutation(s) could disrupt
the global fold of Gα or, at the very least, affect the disposition
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of the switch regions and other surface contact points to which
RGS proteins interact,24,31 thereby altering the normal affinity
and specificity that RGS proteins show for their various Gα
substrates. The 2 point mutations of R178M and A326S are
interior to the guanine nucleotide binding pocket (Fig. 5) but
could nevertheless affect the RGS domain interaction surface.
To test for this possibility, we used SPR to compare the
binding interactions of RGS2 and RGS16 with wild-type Gαi1
versus the Gαi1(R178M/A326S) variant. Multiple previous
studies8,24,32 have established that RGS2, a potent GAP for Gαq,
does not interact with wild-type Gαi1 in vitro; this same lack of
interaction was observed with the Gαi1(R178M/A326S) mutant
(data not shown). Conversely, RGS16 is known to be a Gαiinteracting RGS protein24 and was found by SPR to bind
equivalently to immobilized wild-type Gαi1 and Gαi1(R178M/
A326S) proteins (Fig. 6). This equivalence included RGS16
only interacting with high affinity to the Gα subunits in their
transition state-mimetic form (namely, Gα in complex with
GDP and aluminum tetrafluoride31). These binding results
Journal of Biomolecular Screening 14(10); 2009
Fluorescent Steady-State RGS Protein GAP Assay
FIG. 6. RGS16 binds equivalently to wild-type Gαi1 and the rate-altered Gαi1(R178M/A326S) mutant. (A,B) Sensorgrams derived from 600-s
injections of various concentrations (3 nM to 10 µM) of RGS16 over surface plasmon resonance (SPR) biosensors of immobilized (A) wild-type
Gαi1⋅GDP⋅AlF4– or (B) Gαi1(R178M/A326S)⋅GDP⋅AlF4–. SPR experiments were also conducted with both Gαi1 subunits in their inactive, guanosine diphosphate (GDP)–bound state (data not shown). (C,D) Resultant sensorgrams were used in equilibrium saturation binding analyses (as
previously described24) to derive dissociation constants (KD values). RGS16 bound to wild-type Gαi1⋅GDP⋅AlF4– with a dissociation constant of
124 nM (95% confidence interval of 76-174 nM; panel C), whereas RGS16 bound to Gαi1(R178M/A326S)⋅GDP⋅AlF4– with a dissociation constant of 115 nM (64-166 nM; panel D). Note that interactions were not observed (for either Gα subunit) when the Gα was GDP bound (as
expected; Soundararajan et al.24 and Tesmer et al.31) or when RGS2 was injected (data not shown).
suggest that no long-range perturbations have been made to the
RGS domain interaction sites on Gαi1 by the 2 rate-altering
mutations of R178M and A326S.
Using the Transcreener GDP assay, we performed an additional test of the Gαi1(R178M/A326S) variant to control for
any unintended changes the 2 point mutations could have
engendered within Gα to alter its interaction specificity with
various RGS proteins. With the same RGS protein spectrum
used in the SPR binding experiments, we found that RGS2
(highly selective for Gαq over Gαi substrates) had no effect on
increasing steady-state GTPase activity of Gαi1(R178M/
A326S), whereas RGS16 increased steady-state GTPase activity 12-fold over the basal rate (Fig. 7).
Pilot screen for inhibitors of RGS4 GAP
activity on Gαi1(R178M/A326S)
Given the robust performance of the Transcreener GDP
assay in the control screen for potential compound interference
Journal of Biomolecular Screening 14(10); 2009
(Fig. 3D) and evidence that the 2 mutations to Gαi1 affected
neither the affinity nor specificity of the Gα/RGS domain interaction (Figs. 6, 7), we proceeded to a pilot screen with
Gαi1(R178M/A326S) and RGS4 using the GenPlus library of
960 bioactive molecules (Fig. 8). The screening window was
first optimized by varying the concentrations of Gα and RGS
protein inputs; at 50 nM Gαi1(R178M/A326S) and 250 nM
RGS4, a maximal signal-to-background difference of 112 mP
units was obtained after 120 min of elapsed reaction time before
fluorescence polarization (FP) measurement. The thiol-reactive
compound CCG-4986 was used in the screen as a positive control for RGS4 inhibition.13,33 The GenPlus library screen was
conducted with Gαi1(R178M/A326S) and RGS4 (Fig. 8A); a
separate counterscreen of the library was performed with
Gαi1(R178M/A326S) and no RGS4 (Fig. 8B) to identify compounds having either nonspecific effects or modifying Gαi1
GTPase activity (rather than RGS4 GAP activity per se).
Z′ factors of 0.60, 0.83, 0.83, and 0.82 were obtained at 60,
90, 120, and 180 min elapsed reaction time, as calculated based
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FIG. 7. The steady-state GTPase activity of Gαi1(R178M/A326S) is
increased by RGS4 and RGS16 but not by the Gαq-selective RGS2.
Transcreener guanosine diphosphate (GDP) assays were performed
as in Figure 4, using 250 nM of the indicated RGS protein. Moles of
GDP produced per mol input Gαi1(R178M/A326S) protein were first
plotted over time using GraphPad Prism and linear regression performed to determine steady-state GTPase rates. Presented bar graph
denotes GTPase-accelerating protein (GAP) factors derived from
these steady-state GTPase rates.
on data from control wells containing either Gαi1(R178M/
A326S) only or Gαi1(R178M/A326S) plus RGS4. Note that
these Z′ factor values reflect only the RGS4-dependent increase
in GTPase activity and not the total observed GTPase activity
relative to no-enzyme controls. The Z factor for the GenPlus
library screen at the 120-min time point (shown in Fig. 8A) was
0.73, which was calculated by excluding values from wells
containing hit compounds. Of the 960 compounds in the
GenPlus library, 17 were initially considered hits in the RGS4/
Gα screen (i.e., those data points that fell outside the µ ± 3σ
range). However, 10 of these 17 hits also resulted in a greater
than ±3σ change in the mean signal within the Gα-only counterscreen and thus were excluded because these compounds are
likely either to affect the Gα subunit or to otherwise interfere
with the assay. Thus, the RGS4-specific hit rate was 0.7%: 7
compounds from the 960-compound library exhibited an modulatory effect on GDP production that was specific to RGS4stimulated GTPase activity (Fig. 8A vs. 8B). Six compounds
(id # 62, 63, 244, 413, 524, 812) exhibited an RGS4-specific
inhibitory effect (i.e., a change in polarization greater than the
[mean + 3 SD] signal threshold), and 1 compound (#596)
exhibited an RGS4-specific activating effect on GDP production (i.e., a change in polarization less than the [mean – 3 SD]
signal threshold). This hit rate may be artificially high in this
pilot screen given that the collection of compounds surveyed
(GenPlus library) is not a diverse sampling of chemical space
but a collection of US-, European-, and Japanese-approved
drugs and other bioactive compounds. As expected,13,33 the
thiol-reactive RGS4 inhibitor CCG-4986 consistently exhibited
inhibition of RGS4-stimulated GDP production (Fig. 8A).
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FIG. 8. Pilot screen and counterscreen using the 960-compound
GenPlus library. Transcreener guanosine diphosphate (GDP) assay
components were added to wells containing 50 nM Gαi1 (R178M/
A326S) with (A) or without (B) 250 nM RGS4 protein and 10 µM
compound (in 0.5% [v/v] final concentration of DMSO), 150 µM of
reactive RGS4 inhibitor CCG-4986, or 0.5% DMSO only, as indicated
in the legends. The range of signal observed (3 standard deviations [σ]
about the mean [µ]) is denoted by the dashed lines for the 960-compound library screen using RGS4 and Gαi1 (R178M/A326S) (black;
panel A, coefficient of variation [CV%] = 8.8%) and library counterscreen using Gαi1 (R178M/A326S) alone (gray; panel B, CV% = 3.0%).
Data in panel A were obtained at 120 min of elapsed reaction time; data
in panel B were obtained after 210 min of elapsed reaction time, given
the slower GTPase (and GDP production) rate of Gαi1 (R178M/A326S)
in the absence of RGS4 GTPase-accelerating protein (GAP) activity.
To our knowledge, the combined use of a GDP detection assay
with a rate-altered Gα subunit represents a unique strategy to
detect RGS protein GAP activity. Even though the 2 primary
components of Gα catalysis, GTP hydrolysis rate and product
release, were altered significantly by mutation, the resultant
Gα subunits still served as functional substrates for the GTPaseaccelerating activity of RGS proteins. Using this doublemutation strategy to develop a steady-state RGS protein GAP
Journal of Biomolecular Screening 14(10); 2009
Fluorescent Steady-State RGS Protein GAP Assay
assay that is easy for the nonspecialist to perform and is well
suited for HTS removes a major technical barrier preventing the
exploration of RGS proteins as therapeutic targets. Moreover,
Gαi1 is a substrate for the GAP activity of several RGS protein
family members24 in addition to those we have tested here;
thus, the reagents and methods that we have described should
have broad applicability across the protein family. Employing
the rate-altered Gαi1(R178M/A326S) mutant in a homogeneous, endpoint-based, enzymatic HTS assay will be useful in
screening for RGS protein inhibitors, and unlike existing
assays based on the RGS domain/Gα binding interaction,11-13
this enzymatic assay should also facilitate identification of
small-molecule activators of RGS domain-mediated GAP
activity. The lipid moiety phosphatidylinositol-3,4,5-trisphophate (PIP3) has been shown to bind to and thereby inhibit, in
an allosteric fashion, the GAP activity of select RGS domains
such as that of RGS423; Ca2+/calmodulin reverses this PIP3mediated inhibition by competing for the PIP3 binding site.23 A
small molecule targeting this site of allosteric modulation over
RGS domain GAP activity could potentially be quite valuable
therapeutically in pathophysiological situations that may arise
from a loss of RGS protein activity, such as RGS2 in hypertension34 and RGS4 in schizophrenia.35
ACKNOWLEDGMENTS
Thanks to Drs. Christopher Johnston and Francis Willard
(UNC) for initial discussions regarding rate-altering Gα mutations and Dr. Steve Hayes (BellBrook Labs) for discussion and
critical appraisal of the manuscript. Work at BellBrook Labs
was supported by NIH SBIR grant R43 NS059082, and work
in the Siderovski lab was funded by National Institutes of
Health (NIH) grant R01 GM082892. A.J.K. acknowledges early
support from NIH training grant T32 GM008719 and current
support from NIH fellowship F30 MH074266.
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17.
18.
19.
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Address correspondence to:
David P. Siderovski, Ph.D.
UNC–Chapel Hill
4073 Genetics Medicine Bldg, 120 Mason Farm Road,
CB#7365
Chapel Hill, NC 27599-7365
E-mail: dsiderov@med.unc.edu
Journal of Biomolecular Screening 14(10); 2009