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Transcript of The guard cell as a single-cell model towards understanding drought tolerance and abscisic acid...
Journal of Experimental Botany, Vol. 60, No. 5, pp. 1439–1463, 2009Perspectives on Plant Development Special Issuedoi:10.1093/jxb/ern340 Advance Access publication 30 January, 2009
REVIEW PAPER
The guard cell as a single-cell model towards understandingdrought tolerance and abscisic acid action
Caroline Sirichandra, Aleksandra Wasilewska, Florina Vlad, Christiane Valon and Jeffrey Leung*
Institut des Sciences du Vegetal, Centre National de la Recherche Scientifique, UPR2355, 1 Avenue de la Terrasse, Bat. 23, 91190Gif-sur-Yvette, France
Received 26 September 2008; Revised 28 November 2008; Accepted 2 December 2008
Abstract
Stomatal guard cells are functionally specialized epidermal cells usually arranged in pairs surrounding a pore.
Changes in ion fluxes, and more specifically osmolytes, within the guard cells drive opening/closing of the pore,allowing gas exchange while limiting water loss through evapo-transpiration. Adjustments of the pore aperture to
optimize these conflicting needs are thus centrally important for land plants to survive, especially with the rise in
CO2 associated with global warming and increasing water scarcity this century. The basic biophysical events in
modulating membrane transport have been gradually delineated over two decades. Genetics and molecular
approaches in recent years have complemented and extended these earlier studies to identify major regulatory
nodes. In Arabidopsis, the reference for guard cell genetics, stomatal opening driven by K+ entry is mainly through
KAT1 and KAT2, two voltage-gated K+ inward-rectifying channels that are activated on hyperpolarization of the
plasma membrane principally by the OST2 H+-ATPase (proton pump coupled to ATP hydrolysis). By contrast,stomatal closing is caused by K+ efflux mainly through GORK, the outward-rectifying channel activated by
membrane depolarization. The depolarization is most likely initiated by SLAC1, an anion channel distantly related to
the dicarboxylate/malic acid transport protein found in fungi and bacteria. Beyond this established framework, there
is also burgeoning evidence for the involvement of additional transporters, such as homologues to the multi-drug
resistance proteins (or ABC transporters) as intimated by several pharmacological and reverse genetics studies.
General inhibitors of protein kinases and protein phosphatases have been shown to profoundly affect guard cell
membrane transport properties. Indeed, the first regulatory enzymes underpinning these transport processes
revealed genetically were several protein phosphatases of the 2C class and the OST1 kinase, a member of theSnRK2 family. Taken together, these results are providing the first glimpses of an emerging signalling complex
critical for modulating the stomatal aperture in response to environmental stimuli.
Key words: Abscisic acid, drought, guard cells, light, protein phosphorylation.
Introduction
A stone tablet, roughly 114 cm in height, 72 cm in width,
and 28 cm thick, weighing 760 kg, created a sensation in
1799 when it was unearthed at the Mediterranean harbour
Rashid, or Rosetta, during Napoleon Bonaparte’s cam-
paign in Egypt. The text on this stele dates back to 196 BC,
and part of the excitement was due to the fact that the
single passage was written in hieroglyphic, demontic, and in
classical Greek. This turned out to be very fortunate, as
comparative translation of the three languages by French
and British scholars was instrumental in deciphering many
previously impenetrable principles of hieroglyphic writing.
The term ‘Rosetta stone’ has since pervaded our every day
parlance as synonymous to a critical key to a process of
decryption or breakthrough understanding of a difficult
problem. Every intellectual barrier, regardless of its initial
enormity, has been breached eventually by the studies of
* To whom correspondence should be addressed: [email protected]ª The Author [2009]. Published by Oxford University Press [on behalf of the Society for Experimental Biology]. All rights reserved.For Permissions, please e-mail: [email protected]
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a judiciously chosen ‘Rosetta stone’. In biology, this
actually embodies diverse models, mainly in the guise of
bacteria, yeast, worms, flies, and for our intellectual quest in
plant biology, the model plant Arabidopsis (Simpson and
Dean, 2002). Being unrepentant reductionists in the era of
systems biology, our Rosetta stone—the stomatal guard
cell—that promises to enlighten our understanding of signal
integration between light, drought, and abscisic acid (ABA)measures merely 10–20 lm in its overall dimensions but it
possesses all of its mechanistic ‘languages’ decipherable by
genetics, molecular biology, and biophysics. The successful
cross-translation of these three ‘languages’ (i.e. as a multi-
disciplinary approach) will be needed to completely un-
derstand the syntax of each key component in the signalling
chain and how the guard cell turgor is dynamically adjusted
according to the environmental and hormonal cues. At itscrux, this is no more than a fundamental problem of the
signal transduction genre (on reversible cell expansion), but
this field has always held a special appeal to the collective
imagination of biologists, plant breeders, and policy mak-
ers alike because of the need to improve agricultural
productivity—for food, construction, medicine, etc.—in
view of diminishing fresh water supplies, population
growth, and global warming this century. The beckoningquestion for all of us who are intensely engaged in this
cross-disciplinary research area is how soon can these three
‘languages’ be articulated into a coherent model and how
many generalities can flow from the particularities of this
single cell. The limited results that allow a comparison of
similar work conducted in the guard cell and in cell culture
so far strongly suggest shared principles in stress signalling
(Jeannette et al., 1999; Brault et al., 2004).Genetics have revolutionized biology since the turn of the
20th century with the re-discovery of Mendel’s laws on
heredity. When molecular biology joined forces in the
1970s, it began more and more to be appreciated how the
life of a cell depends on the subtle details of the molecules
from which it is built. The small thale cress Arabidopsis
thaliana was ushered in the 1980s as the new plant model
precisely because of its accessibility to genetics and molec-ular probing. To this day, genetics screens—applicable in
both the forward and reverse modes—have been instrumen-
tal in identifying hundreds of mutations that altered
responses of the plant to drought and ABA. In addition to
such gene-by-gene approaches, high throughput tools that
allow monitoring gene expression across the whole genome
in the last decade have revealed networks of co-expressed
genes encoding elements of such diverse nature as todefy—at least at present—any reasonable effort to propose
a unifying signalling scheme. It is not clear why ABA
signalling and its link to drought-adaptive responses require
such complicated mechanistic schemes. This may be due to
the fact that drought adaptation has a large quantitative
component which can be influenced by the intensity of the
experimental drought, the method of drought application
(e.g. in vitro by mannitol, hair dryer on detached plants,etc.) and that the nature of the signalling networks may also
be modified by the cell’s particular developmental state. The
guard cell was developed as a simpler model system
(Armstrong et al., 1995) with the decided aim of decoding
the signalling network in which the membrane transport
system operates in a tight relationship with components in
ABA signalling (Wasilewska et al., 2008). Indeed, stomatal
closure in response to progressive drought has all of the
attributes for an excellent genetic model. Particularly
salutary, is the cell autonomy of the physiological responsedue to the absence of plasmodesmata (Wille and Lucas,
1984), the extreme robustness, and the all important virtue
of reducing the quantitative aspect of drought response into
an all-or-none phenotype (opening/closing).
The guard cells are specialized epidermal cells, located in
pairs on the aerial organs of the plant. Each pair of cells
forms the boundary of a small pore, or stoma, in the
epidermis. Due to the impermeable wax layer on theepidermal surface, the stomatal complex therefore plays
a major role in controlling gas exchange (photosynthetic
carbon dioxide uptake) between plant and the surrounding
atmosphere (Fig. 1a). The stomata are important regulators
of the global atmospheric environment (Hetherington and
Woodward, 2003), and, in fact, the developmental fate of
epidermal cells to differentiate or not into a pair of mature
guard cells—and therefore stomatal density—is intimatelylinked to environmental cues (Gray et al., 2000; Hether-
ington and Woodward, 2003; Masle et al., 2005). The
opening and closing of the stomatal pore are regulated by
osmotic pressure of the guard cells, brought about by the
dynamic changes in the intracellular concentrations of
inorganic and organic ions (K+ and malate2–) and sugars.
These events require interplay between ion channels,
vacuolar and membrane transporters, and metabolite con-versions (Roelfsema and Hedrich, 2005; Wasilewska et al.,
2008). The variations in the transpirational fluxes caused by
stomatal movements can alter leaf temperatures, the ampli-
tudes of which are sufficiently large to be semi-quantifiable
by remote infrared thermography (Raskin and Ladyman,
1988). This technology has therefore been applied to
identify mutants of Arabidopsis impaired in stomatal re-
sponse to experimental drought that is closer to fieldconditions than those based on rapid or chemical de-
hydration stress (Vartanian et al., 1994; Merlot et al., 2002)
(Fig. 1a). Below, first guard cell signalling as established by
biophysical and pharmacological approaches will be de-
scribed, followed by the more recent progress by genetics
and molecular biology in identifying the major components
that link guard cell functions to light and ABA signalling.
The biophysical framework of stomatalmovement
Throughout the 1980s and 1990s, a large body of physiolog-ical data showed that hyperpolarization of the plasma
membrane is stimulated by the activities of H+-ATPases
(proton pumps coupled to ATP hydroylsis), which then
initiates stomatal opening by allowing entry of K+ through
the voltage-dependent K+ inward-rectifying channels. In
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conditions of water stress, the increase in either cellular
ABA, or apoplastic ABA at the surface of guard cells,
triggers a reduction in turgor pressure caused by K+ efflux
and release of anions such as organic acids necessary forstomatal closure. The two distinct sites of ABA accumulation,
either in the cell or in the apoplast, correlate with the presence
of physiologically detectable perception sites or receptors
inside the cell, as well as on its surface. The enhanced
transpiration of ABA-biosynthetic mutants (Koornneef
et al., 1982; Leon-Kloorsterziel et al., 1996; Marin et al.,
1996; Merlot et al., 2002), transgenic plants expressing an
anti-ABA antibody (Artsaenko et al., 1995), and recentgenetic screens for mutants of Arabidopsis sensitive to
progressive drought, based solely on stomatal movement as
the phenotype (Merlot et al., 2002), have provided converg-
ing and incontrovertible evidence for this critical role of
endogenous ABA. As alluded to above, the reduction in
turgor pressure is achieved by the net efflux of both K+ and
release of anionic organic acids from the vacuole to the
cytoplasm and from the cytoplasm to the outside of the cells.One of the earliest responses to ABA frequently, but not
always, is a rise in cytosolic free Ca2+ ([Ca2+]i). The source of
Ca2+ required to elevate [Ca2+]i in response to ABA
originates from both voltage-activated influx across the
plasma membrane and release from internal stores as de-
duced by the use of pharmacological agents and Ba2+ (which
acts as a competitor of Ca2+ influx, internal release as well asthe transient) (MacRobbie, 2000). The uptake and release of
Ca2+ from internal stores, corresponding to various endo-
membranes and, particularly, the endoplasmic reticulum
(ER), are triggered by the intermediates cyclic ADP-ribose
(Allen et al., 1995; McAinsh et al., 1997; Wu et al., 1997),
inositol 1,4,5-trisphosphate (IP3) (Blatt et al., 1990; Gilroy
et al., 1990; Allen et al., 1995; Lee et al., 1996), hyperpolar-
ization of the plasma membrane in Vicia (Grabov and Blatt,1999) and, more recently, myo-inositol hexakisphosphate
(InsP6), which is about 1003 more effective than IP3 based
on inactivation of the K+ inward-rectifying channel (Lemtiri-
Chlieh et al., 2003) (Fig. 1b). The regulation of the Ca2+
signal relay seems highly redundant, as the changes in 32P
labelling of both inositol lipids and inositol phosphates argue
for ABA-induced phosphoinositide turnover in the guard cell
(Lee et al., 1996). However, the changes in label in putativeIP3 observed in these studies were surprisingly small if this
were the major activator of ABA-triggered Ca2+ release. The
aminosteroid, U73122, an inhibitor of phospholipase C, can
Fig. 1. Genetic screen of Arabidopsis mutants sensitive to progressive drought. (a) Closing (ABA, drought) and opening (light) of the
stomatal pore alter the transpirational flux (top) with amplitudes sufficiently large to be visualized by remote infrared thermography
(bottom). In comparison to wild-type plants, mutants that are impaired in stomatal closure in conditions of water deficit are therefore
cooler (plants noted by circles in the infrared images). Figures are modified from those in Merlot et al. (2002) and Roelfsema and Hedrich
(2005). (b) Summary of transport events at the plasma membrane of the guard cell. In responding to drought or ABA, the anion channel
(SLAC) is activated, which drives depolarization of the plasma membrane, while the activity of the proton pump ATPase (OST2), needed
for plasma membrane hyperpolarization, is inhibited. Both of these membrane transporters are regulated by Ca2+, and, in the case of
OST2, the inhibition is most likely mediated, at least in part, by the calcium-sensitive PSK5 kinase. Membrane depolarization also leads
to activation of the K+-outward-rectifying channel (GORK) to expel K+ and inhibition of the K+-inward-rectifying channels (KAT1 and
KAT2) for K+ influx, both of these events are coordinated in opposing fashion by a pH-sensitive pathway that is in part membrane limited.
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modify the form of the cytosolic Ca2+ oscillation induced by
ABA, but not externally applied Ca2+ (Staxen et al., 1999).
Accordingly, U73122 also only partially inhibits stomatal
closure by ABA but not by external Ca2+ (Jacob et al., 1999;
Staxen et al., 1999). Injection of 8-NH2-cADPR (a compet-
itive antagonist of cADPR) or blocking cADPR synthesis by
the addition of nicotinamide can also inhibit ABA-induced
stomatal closure, but again only partially (Leckie et al., 1998;MacRobbie, 2000).
In Arabidopsis, hyperpolarization of the guard cell
plasma membrane can lead to increased Ca2+ influx only in
the presence of applied H2O2, a by-product of superoxides
(Pei et al., 2000). Moreover, applied ABA can also induce
elevation of endogenous H2O2, and blocking the production
of such reactive oxygen species by diphenylene iodonium
chloride impairs the stomatal closing response (Pei et al.,2000). There are multiple sources of H2O2; perhaps the
most relevant to general ABA signalling is that originating
from the catalytic activities of two plasma membrane-
bound NADPH oxidase subunits, AtrbohD and AtrbohF
(Kwak et al., 2003). It is noteworthy though, that about
45% of the guard cells in the double mutant AtrbohD/F still
showed elevated Ca2+ signal in response to applied H2O2
(Kwak et al., 2003), indicating that there are additional andprobably equally important sources. Likewise, the range of
possible cellular targets of H2O2 is unknown, but, in vitro,
the protein phosphatase activities of both ABA-INSENSI-
TIVE1 (ABI1) and ABI2 can be inhibited by this radical
(Meinhard and Grill, 2001; Meinhard et al., 2002). On the
other hand, both the open stomata1 (ost1) (Mustilli et al.,
2002) and growth control by ABA2 (gca2) (Pei et al., 2000)
mutants, insensitive to stomatal closing in ABA, are eitherseverely deficient in H2O2 production or its perception,
respectively (Wang and Song, 2008).
Nitric oxide (NO), first discovered in 1978 as a gaseous
substance in endothelial cells that relaxes blood vessels,
turns out to function as an intermediate in ABA signal-
ling as well. NO—usually supplied in the form of NO
donors such as sodium nitroprusside or S-nitroso-N-
acetyl-penacillamine—was first shown to induce stomatalclosure and reduce transpiration in many plant species,
including Vicia faba, Salpichroa organifolia, Tradescantia
spp., pea, and Arabidopsis thaliana (Neill et al., 2008). NO
promotes intracellular Ca2+ release via cGMP-dependent
cyclic ADP-ribose synthesis (Garcia-Mata et al., 2003),
and this process can be blocked by large spectrum kinase
inhibitors such as K252A and staurosporine (Sokolovski
et al., 2005). The precise sources of NO production are stilldebatable but it is generally thought that nitrate reductase,
especially the isoform encoded by NIA1, may contribute to
this step (Neill et al., 2008).
The Ca2+ signal then triggers a network of effects,
including K+ efflux by vacuolar and plasmalemma K+
channels, release of anionic organic acids by the slow (S)-
type anion channels (Schroeder and Hagiwara, 1989;
Hedrich et al., 1990), while at the same time, inhibits theactivity of K+ inward-rectifying channels (Schroeder and
Hagiwara, 1989; Kelly et al., 1995).
Several observations suggest that Ca2+-independent path-
ways also exist. The physiological state of the guard cell
(e.g. in intact plants versus isolated protoplasts) or the
particular plant species require different rations of Ca2+ to
relay the ABA signal (Levchenko et al., 2005; Marten et al.,
2007). This had led to the alternative proposal of a pH-
sensitive pathway. The concept of pH as a second messen-
ger in ABA signalling has been parlayed from two relatedobservations made in the Blatt laboratory: (i) exposure to
ABA led to a 0.1–0.3 unit rise in pHi of guard cells (Irving
et al., 1992; Blatt and Armstrong, 1993); and (ii) artificially
decreasing the pHi by loading a weak organic acid (usually
butyric acid) suppressed potassium efflux (Blatt, 1992; Blatt
and Armstrong, 1993). pHi acts independently of Ca2+,
based on their effects on K+ influx as well as the differential
sensitivities of the K+ inward- and K+ outward-rectifiers(Grabov and Blatt, 1997). Miedema and Assmann (1996)
have shown that the effect of pHi was the result of proton
interaction with sites associated with the membrane, per-
haps K+ outward-rectifying channel or auxiliary proteins.
The action of pHi also extended to the control of K+ influx,
which was activated by acidity, opposite to that of the K+
efflux (Blatt, 2000). Although these electrophysiological
studies suggested membrane-delimited pathways, they didnot exclude the possibility that there might also be pH-
sensitive cytosolic regulators (see below in the discussion on
the sharp pH sensitivity of the protein phosphatase ABI1).
Merging biophysics with genetics andmolecular biology on stomatal opening: theroles of blue-light photoreceptor kinases,proton pumps, and K+ uptake channels
Light is captured by plants as a source of energy critical for
photosynthesis. But it also doubles as a trigger in signal
transduction pathways directing growth and development(photomorphogenesis). In particular, wavelengths in the blue
and UV-A regions of the electromagnetic spectrum control
phototropism, cotyledon and leaf expansion, stomatal open-
ing, and chloroplast movements in response to changes in
light intensity. Light in the blue spectral range is captured by
receptor kinases, known as phototropins, which then imple-
ment many of the above responses, including stomatal
opening for CO2 assimilation (Shimazaki et al., 2007). Bycontrast, photosynthetically active radiation seems unimpor-
tant for stomatal opening as guard cells that lack functional
green chloroplasts could still respond to blue light, CO2, and
ABA (Roelfsema et al., 2006). Phototropins are ubiquitous
among higher plants and Arabidopsis contains two: PHOT1
and PHOT2. Light sensing is mediated by two flavin-binding
motifs, known as LOV1 and LOV2 (for light, oxygen,
voltage), located at the N-terminal photosensory region ofthe proteins. Photoexcitation leads to activation of the C-
terminal kinase domain and, as a result, receptor autophos-
phorylation. The PHOT1 and PHOT2 are both required for
the activation of the H+-ATPases by blue light and mediate
stomatal opening in a redundant manner (Kinoshita et al.,
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2001). Although the signals from the blue-light receptors are
ultimatedly transduced to the H+-ATPases (see below), there
is no evidence that these proton pumps are direct phosphor-
ylation targets. In fact, their partially redundant functions in
stomatal opening via blue light may belie the actual complex
roles of PHOT1 and PHOT2. Both are critical for blue-light
stimulation of stomatal opening as the double mutant
phot1,phot2—but not their respective single mutants—iscompletely insensitive to blue light (Kinoshita et al., 2001).
These two photoreceptor kinases, however, also assume
distinct functions. PHOT1, but not PHOT2, can interact
directly with NON PHOTOTROPIC HYPOCOTYL3
(NPH3) and ROOT PHOTOTROPISM2 (RPT2), which are
plant-specific novel proteins required for PHOT1-
dependent phototropism (Motchoulski and Liscum, 1999;
Sakai et al., 2000; Inada et al., 2004). A protein interactingwith the N-terminal domain of the Vicia phot1a, but not
phot1b, was also isolated from guard cells (Emi et al., 2005).
It is therefore likely that PHOT1 and PHOT2 may in fact
process both common and separate information in the
transduction chain.
H+-ATPases, upon activation by the phototropin-mediated
signals, hyperpolarize the plasma membrane to ultimately
drive stomatal opening. Depending on the plant species, theplasma membrane potentials are hyperpolarized to different
potentials, but the important point is that they are always
slightly more negative than the activation potential of the K+
uptake channels (about –120 to –180 mV) (Dietrich et al.,
2001). This voltage gradient is therefore sufficient to account
for K+ uptake from the apoplastic space via the K+ inward-
rectifying channels (Blatt, 1991; Thiel et al., 1992; Roelfsema
and Prins, 1998). The functions of the H+-ATPases and theK+ inward-rectifying channels are therefore coupled electri-
cally. In addition to this electric coupling between the two
membrane transporters, other modes of regulations through
pump-driven apoplastic acidification are equally important in
assuring optimal K+ uptake capacity. Measurements on
guard cells in situ within epidermal strips and protoplasts
derived thereof have detected activation of K+ uptake
channels by low pH (Blatt, 1992; Ilan et al., 1996; Dietrichet al., 1998; Bruggemann et al., 1999). Functional coupling
between H+-ATPases and K+ inward-rectifying channels
underlying stomatal opening is therefore subjected to
selective control mechanisms relying on both voltage and
pH. Apoplastic acidication not only changes the voltage-
sensitivity, but also the number of K+ uptake channels as well
(Blatt, 1992; Ilan et al., 1996; Hoth et al., 1997; Dietrich et al.,
1998) (see below). Assuming one titratable pH-sensitive site,a maximum pH sensitivity (pKa) value of 5.3 was obtained
for K+ uptake channels in Vicia faba (Ilan et al., 1996). At
variance, a pKa value of 6.3 was instead obtained by Grabov
and Blatt (1997); with respect to pHi regulation of the K+
inward-rectifier, the central question may be the effective pH
within the fixed-acid matrix of the cell wall at the membrane
surface, rather than the apoplastic space. The pKa value of
K+ uptake channels in Arabidopsis thaliana was about pH4.8, whereas pH 6.2 was obtained for Solanum tuberosum and
Nicotiana tabacum (Dietrich et al., 1998; Bruggemann et al.,
1999). K+ uptake in the guard cell is therefore contingent on
the rate of the proton pump and the apoplastic pH buffering
capacity of the individual plant species.
Although K+ provides the major osmoticum, investiga-
tions have also reported that sucrose accumulates in guard
cells and replaces K+ in the afternoon to maintain stomatal
apertures (Tallman and Zeiger, 1988). Sugars are some of the
breakdown products from starch, but it is unlikely that theentire source of sucrose is derived from photosynthetic CO2
fixation within guard cell chloroplasts because the chloro-
phyll content in guard cells is <2% of that of mesophyll cells
on a cell basis and Rubisco activity is low on a chlorophyll
basis (Outlaw et al., 1979; Shimazaki et al., 1983; Gotow
et al., 1988; Shimazaki, 1989; Reckmann et al., 1990).
Because sucrose and hexose can accumulate to high levels in
the apoplast during the day, it is reasonable to assume thatthe source of sucrose originates mostly from import of this
reserve (Lu et al., 1997; Vavasseur and Raghavendra, 2004).
Consistent with this notion is that sucrose uptake by guard
cells was indeed detected when epidermal peels were over-
layed onto mesophyll tissues (Dittrich and Raschke, 1977);
moreover, the activation of H+-ATPase by the fungal toxin
fusicoccin was found to stimulate sucrose uptake in guard
cell protoplasts (Reddy and Das, 1986; Ritte et al., 1999).This suggests that H+-ATPase activity is also coupled to
sugar transporters, besides K+ channels. The sucrose trans-
porter AtSUC3 is expressed in Arabidopsis guard cells, and
also the AtSTP1 H+/monosaccharide symporter could con-
tribute to guard-cell specific accumulation of sucrose (Stadler
et al., 2003; Meyer et al., 2004).
Forward genetic screens for mutants in Arabidopsis with
enhanced transpiration under mild drought conditions haveidentified two allelic mutations, open stomata2 (ost2)-1 and
ost2-2, at the AHA1 locus encoding a proton pump (Merlot
et al., 2007) (Fig. 1a, b). Both of these mutations rendered
the AHA1 H+-ATPase constitutively activated. The family
of H+-ATPases is composed of 11 genes (and one likely
pseudogene) in the Arabidopsis genome, and their corre-
sponding transcripts are all detectable in guard cell proto-
plasts, whereas only four of them are detectable inmesophyll cells (Ueno et al., 2005). Arguably, identifying
two allelic mutations in the same gene out of 11 possible
targets could still be statistically fortuitous but it is nonethe-
less noteworthy that the genetic screens were accomplished
independently using Arabidopsis plants of different genetic
backgrounds and also under slightly varying experimental
drought conditions. Alternatively, the bias in only identify-
ing AHA1 could reflect the relatively dominant role of thisproton pump in regulating membrane hyperpolarization in
response to progressive water depletion and to ABA. In any
event, the fact that only constitutively activating mutations
have been recovered at this locus so far also indicates that
at least one other H+-ATPase in the gene family could
assume partially overlapping functions. Functional overlap
is consistent with the fact that an insertion mutation in the
AHA1 locus causes no obvious phenotype (data notshown). A candidate gene that functionally overlaps with
AHA1 might be the closest homologue AHA2.
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The current model on regulation of proton pump activity
suggests that an H+-ATPase is kept in an inactive state
by intramolecular contact between its autoinhibitory
C-terminal domain with certain critical amino acids in the
rest of the protein (Palmgren, 2001). This model is indeed
consistent with the data generated by the yeast two-hybrid
interaction system based on the split ubiquitin reporter
(Merlot et al., 2007) and by bimolecular fluorescencecomplementation (BiFC) in co-infiltrated living tobacco
epidermal cells (Fig. 2a) that these two domains can
interact, even in trans. When activated, the H+-ATPase is
phosphorylated on its penultimate threonine residue, and
the tight interaction of the C-terminal autoinhibitory
domain is released from the rest of the protein. Phosphor-
ylation by itself is not sufficient to activate the H+-ATPase,
but it requires the further binding of 14-3-3 proteins to thephosphorylated C-terminus (Kinoshita and Shimazaki,
1999; Emi et al., 2001). The kinase(s) that is critical for the
phosphorylation of the penultimate threonine residue has
not been identified, but, in Vicia, it is insensitive to general
protein kinase inhibitors (Kinoshita and Shimazaki, 2001),
and this upstream kinase in spinach has been demonstrated
to be associated with the plasma membrane (Svennelid
et al., 1999). The crystallization of the full AHA2 H+-ATPase monomer at a resolution of 5.5 A has been
achieved and the results suggested that the C-terminal
autoinhibitory domain assumed no particular structure
(Pedersen et al., 2007). In plant cells, however, the
physiologically quiescent form of an H+-ATPase may not
be a monomer but a dimer, with the C-terminal domains
arranged in a probable antiparallel configuration main-
tained by contacts between residues in the so-called RIIsubregion of the inhibitory domain (Ottmann et al., 2007).
Once activated, the dimer is said to be converted into
a wheel-like hexamer in a higher-order complex with three
14-3-3 dimers (Kanczewska et al., 2005; Ottmann et al.,
2007). The mechanisms by which interconversion between
these higher-order structures are mediated are not known.
ABA partially blocks the activation of H+-ATPases by blue
light. Reduction of this proton pumping activity in the plasmamembrane of the guard cell is necessary for subsequent
membrane depolarization leading ultimately to stomatal
closure. Our knowledge concerning how ABA inhibits the
proton pump remains fragmentary, but part of the effect
might be exerted indirectly through nitric oxide and H2O2
triggered by ABA (Zhang et al., 2004, 2007). The inhibitory
effect of ABA on proton pumping, H+-ATPase phosphoryla-
tion, and stomatal opening can be rescued by applying2-carboxyphenyl-4,4,5,5-tetramethylimidazoline-1-oxyl-3-oxide
(c-PTIO), a scavenger of NO (Zhang et al., 2007), but not by
H2O2. Instead, the stimulatory effect evoked by H2O2 to close
stomates may be directed through another yet-to-defined
pathway that implicates the histidine kinase AHK5 (Desikan
et al., 2008). This other pathway is thought to be divergent
from that of ABA despite the consistent observation of the
tight association of ABA and H2O2 production. An earlierobservation that the protein phosphatase inhibitor calyculin
was relatively more effective than okadaic acid in blocking
stomatal opening in response to blue light led to the
speculation, based on the known partial specificities of these
protein phosphatase inhibitors, that protein phosphatases 1
(PP1) might represent a key element in part of the blue-light
signalling chain (Kinoshita and Shimazaki, 1997). Transient
overexpression of a dominant negative form of the catalytic
subunit of a protein phosphatase 1 (VfPP1c) in the guard cells
of Vicia faba by bombardment was found to indeed blockstomatal opening in response to blue light, but only weakly so
to red light. The step inhibited appeared to be upstream of the
plasma membrane H+-ATPase, because the inhibition can be
circumvented by applied fusicoccin (which activates H+-
ATPases). That a PP1 is a key positive regulator in blue-light
signalling is reinforced by the treatment with the cell-perme-
able inhibitor tautomycin, which has a 10-fold higher potency
for PP1 than PP2A. Phototropins and H+-ATPases arephosphorylated when guard cells are exposed to blue light;
yet, only the phosphorylation of the proton pumping, but not
that of the phototropins, was observed to be reduced
dramatically in the presence of tautomycin (Takemiya et al.,
2006). There have been no corresponding mutants identified in
Arabidopsis because the PP1c is encoded by nine isogenes with
between 90% and 99% amino acid sequence homology. It
appears that a severe reduction in their gene expression byreverse genetic methods may also cause lethality as recovery of
this class of mutant has been problematic (Takemiya et al.,
2006). In addition, the inhibitory effect of ABA on H+-
ATPase is considerably lessened by mutations affecting
a homologous pair of protein phosphatases, 2C ABSCISIC
ACID-INSENSITIVE 1 and 2 (ABI1 and ABI2) (Roelfsema
et al., 1998), and that the C-terminus of AHA2 can complex
with PP2A scaffold subunits (Fuglsang et al., 2006). There is,however, no knowledge on whether these protein phospha-
tases directly inactivate the proton pumps. The most direct
evidence for a negative regulator of H+-ATPases comes from
the demonstration of a specific calcium-stimulated kinase,
PKS5 (a member of the SnRK3 kinase family), in phosphor-
ylating Ser931 of AHA2, which interfered with the binding of
a 14-3-3 protein to the penultimate threonine (Fuglsang et al.,
2007). In a functional assay based on yeast, AHA2 alone cancomplement the growth defect of a mutant disrupted in its
endogenous H+-ATPase. However, co-transformation of
AHA2 with PKS5 alone or PSK5 together with its calcium-
binding subunit SCaBP1 led to poor complementation of this
growth defect, consistent with the notion that the kinase and
its cognate calcium-binding subunit conjointly down-regulate
AHA2. Since the Ser931 is in a highly conserved block of
amino acid residues, phosphorylation by PSK5 (or homolo-gous SnRK3) has been proposed to represent a general mode
of negative regulation of H+-ATPases.
Dynamic regulation of the K+ inward-rectifying channels by changing itsactivation state
As mentioned above, the hyperpolarization of the plasma mem-
brane activates the voltage-dependent K+ inward-rectifying
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channels. K+ is in fact a macronutrient essential not only for
adjusting osmotic potential (as in the case of stomatal opening
through cell expansion), but it is also vital for the activity of
a large number of cytosolic enzymes, and for controlling
the membrane potential of cells. It is therefore not
surprising that the plant has elaborate uptake and
distribution systems for this cation (Very and Sentenac,
2003; Amtmann et al., 2004; Dreyer et al., 2004; Gierth and
Maser, 2007; Lebaudy et al., 2007). The functional form of
these channels is composed of four a-subunits (Daram
et al., 1997). In the guard cells of Arabidopsis, KAT1 and
KAT2 encode the majority of the a-subunits which proba-
bly assemble into homotetramers or heterotetramers at
different stoichiometric ratios (and with other minor iso-
forms) presumably to increase functional flexibility (Pilot
et al., 2001; Lebaudy et al., 2008a). Mutants disrupted for
Fig. 2. Confirmation of protein interaction by biomolecular fluorescence complementation (BiFC) based on reconstitution of the split
yellow fluorescent protein (YFP). (a) To test intramolecular interaction of the H+-ATPase OST2 in live plant cells, the N-terminal domain of
the proton pump (aa 1–842) was fused in-frame to the C-terminal half of the fluorescent protein YFP (YFc). Similarly, the C-terminal
autoinhibitory domain of OST2 (aa 838–949) was tagged with the N-terminal half of YFP (YFn) as a translational fusion. These fusion
constructs, along with the suppressor of transgene silencing HcPro, were propagated separately in the Agrobacterium tumefaciens
strain AGL0 and then the proteins were transiently and simultaneously expressed in the leaves of Nicotiana tabacum by co-infiltration.
Infiltrated plants were maintained in greenhouse conditions (22 �C, 60% humidity, 16 h light/8 h dark cycles) for 48–72 h. Infiltrated areas
from leaves were excised and examined by confocal microscopy (Leica TCS SP2). When the spectrum of the fluorescence was
measured, the reconstituted YFP emits a diagnostic frequency between 500 nm and 535 nm (a–c). (b) The well-characterized KAT1 was
served as the positive control in this protein interaction test based on BiFC. KAT1 is convenient because this K+ inward-rectifying a-
subunit can homotetramerize and form the characteristic aggregates of ;0.25–0.5 lm in the plane of the plasma membrane, which is
recapitulated here with the split YFP. (c) Like the yeast Snf1, the ABA-activated kinase OST1 can also homodimerize (as shown by the
particular strong fluorescence from the reconstituted YFP in the nuclei). The YFP fluorescence following the contour of the epidermal
cells most likely reflects cytoplasmic localization which is currently being pursued in detail (C Sirichandra, unpublished results) but it is
consistent with it being the target of negative regulation of ABI1, which is localized in both the nucleus and cytoplasm (Moes et al., 2008).
(d) Negative control based on co-infiltration of chimeric constructs expressing the C-terminal autoinhibitory domain of OST2 fused
translationally in-frame to YFPn and another unrelated transporter fragment similarly fused to YFPc (A Wasilewska, unpublished results).
Negative control interactions in most cases gave no fluorescence. For the purpose of illustration, however, the panel shown here
represents the highest level of background fluorescence that has been encountered in the entire series of experments. These occasional
irregularly shaped and randomly distributed spots are most likely due to autofluorescence. Although the background fluorescence is
visually also yellow, its peak emission frequency from these spots is ;600 nm, which distinguishes it from that of the reconstituted YFP.
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either one or a combination of both genes displayed hardly
perceptible K+ uptake defect. Increasingly severe pheno-
types were obtained, however, when dominant-negative
forms of these channels were introduced into the plants in
either the wild-type (as for the experiments reported for
KAT1) (Baizabal-Aguirre et al., 1999; Kwak et al., 2001)
or the corresponding null genetic background (as for
KAT2) (Lebaudy et al., 2008b). These combined resultsindicate that KAT1 and KAT2 are largely functionally
equivalent and are extremely efficient in K+ uptake to
assure an abundant supply of this macroelement esential
for plant development. The activity of the KAT1 seems to
be modulated by phosphorylation. A 48 kDa calcium-
independent kinase activity was detected in extracts of Vicia
guard cell protoplasts, but not in mesophyll cells, that can
phosphorylate in vitro a peptide containing the C-terminal356 amino acids of KAT1 (Mori et al., 2000). Interestingly,
this kinase was rapidly but transiently activated by exoge-
nous ABA in a dose- and time-dependent manner (Mori
et al., 2000). Since the KAT1 current is suppressed by
depolarization of the guard cell plasma membrane and
elevated Ca2+ triggered by ABA, these observations suggest
that phosphorylation of the C-terminus may bring about
a change in the voltage-dependent activation kinetics of thisK+ channel (Tang and Hoshi, 1999). The exact kinase from
Vicia that phosphorylated KAT1 is not known, but the
obvious candidate, AAPK, purified from ABA-treated
guard cell protoplasts (Li and Assmann, 1996; Li et al.,
2000) apparently did not support phosphorylation of KAT1
(Li et al., 1998). It has also been reported that a 57 kDa
calcium-dependent kinase activity from both guard cell
protoplast membrane and soluble fractions can phosphory-late KAT1 produced in a coupled transcription–translation
system (Li et al., 1998).
Evidence from earlier work shows that K+in channel
activities are regulated by GTP-regulatory proteins (G-
proteins) (Fairley-Grenot and Assmann, 1991). Similar to
the pH-sensitive pathway discussed above, at least part of
that regulated by G-proteins seems to be associated directly
with the plasma membrane as well because various GTPanalogues can alter K+
in channel opening/closing activities
in membrane patches isolated from Vicia faba guard cell
protoplasts (Wu and Assmann, 1994). Furthermore, toxins
such as pertusis and cholera, which covalently modify the
a-subunits of many G-proteins by catalysing the transfer of
ADP-ribose from NAD+ to specific amino acid residues can
also inhibit K+in channel activity (Wu and Assmann, 1994).
The precise mechanistic link between G-proteins and K+in
channels is still not known, however.
Controlling K+ inward current and H+-ATPase activity by endo- and exocytosis
As has been described, stomatal opening and closing are
reflected in the swelling and shrinking, respectively, of the
pair of stomatal guard cells. The volume changes can alter
the surface area by up to 40% (Raschke, 1979) but it was
not clear how the guard cell could achieve such dramatic
changes, especially in nature where fluctuation of micro-
environments is the norm that will demand continual but
small adjustments of the cell surface. Studies combining
biophysics and cell biology within the last few years have
shown that the guard cell can be surprisingly resourceful:
cell expansion can be driven by excursion and removal of
equivalent portions of plasma membrane material withremarkable rapidity (Homann, 1998; Homann and Thiel,
2002; Hurst et al., 2004). In Vicia guard cells, moreover,
a simultaneous measurement of membrane capacitance and
ionic currents suggested that the surface increase was
associated with insertion of both K+ inward- and K+
outward-rectifying channels (Homann and Thiel, 2002).
Parallels of this kind of mechanism of cell volume control
exist in animals, including the cAMP-induced insertion ofthe cystic fibrosis transmembrane conductance regulator
(CFTR, an ABC transporter with channel characteristics)
(Kleizen et al., 2000) and the delivery of epithelial Na+
channels to the apical membrane promoted by aldosterone
and insulin (Erlij et al., 1994; Blazer-Yost et al., 1998).
Further detailed studies on KAT1 by transient expression of
the protein tagged with the fluorescent protein GFP in Vicia
guard cell protoplasts (Hurst et al., 2004) or tobacco leafepidermal cells (Sutter et al., 2006) showed that the fusion
protein was organized as microdomains of ;0.25–0.5 lm in
diameter equivalent to clusters of roughly 50 tetrameric
channels (Hurst et al., 2004; Sutter et al., 2006) that were
positionally stable within the plane of the plasma membrane
(Sutter et al., 2006). A reservoir of KAT1 is therefore
available in the form of a vesicular pool in the cytoplasm,
and the channels are delivered into the plasma membraneon demand by vesicle exocytosis. Targeting KAT1 to the
plasma membrane was found to depend on SPY121,
a member of the Q-SNARE (soluble N-ethylmaleimide-
sensitive factor attachment protein receptor) subclass of
syntaxins. A fragment of SNARE derived from its cleavage
by Clostridum neurotoxin was shown to block, presumably
in a dominant-negative manner, responses of K+ and Cl–
channels to ABA (Leyman et al., 1999) and to have causednoticeable changes in the KAT1 distribution in the plane of
the plasma membrane (Sutter et al., 2006).
Insertion of KAT1 into the plasma membrane requires
exocytosis that is also encrypted by intrinsic sequence
signatures and structural contexts. Di-acidic motifs, D/E-X-
D/E, have been found to function as ER export signals in
plasma membrane proteins in yeast and animal cells
(Nishimura and Balch, 1997; Votsmeier and Gallwitz,2001), and this molecular cryptogram seems conserved in
plants. There are four similar di-acidic motifs (DXE/DXD)
in the C-terminal domain of KAT1, but only one of them
(DAE394–396 localized to the nucleotide-binding domain),
which also conserved in other plant K+in rectifiers, was
found to be required for export from the ER to the plasma
membrane, as mutation in this motif (to AAA) caused
nearly complete retention of KAT1 in ER-like endomem-branes in transfected guard cell protoplasts and human
embryonic kidney cells (Mikosch et al., 2006). These results
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would imply that ER export may constitute an important
mechanism in regulating channel density—and therefore
total K+ transport activity—in conjunction with cell volume
control. Conversely, inactivation of KAT1 by ABA was
accompanied by selective endocytosis from the plasma
membrane leading to their sequestration within an endo-
somal pool (Sutter et al., 2007). Although sequestration was
initiated in concert with detectable changes in K+ channelactivities evoked by ABA (Homann and Thiel, 2002;
Meckel et al., 2004; Homann et al., 2007), this process alone
is several orders of magnitude too slow to account for the
short-term control of K+ flux by this hormone. Remark-
ably, enodocytosis can still occur despite a high osmotic
pressure (Meckel et al., 2004).
By contrast to KAT1, less is known about trafficking of
the proton pump. In the same studies that examined KAT1transport by transient expression in tobacco epidermal cells,
the endogenous H+-ATPase PMA2 of tobacco was also
tracked but it seemed to be stationary during these same
studies (Sutter et al., 2006, 2007). However, the insertion of
H+-ATPases—exemplified by PMA2 (Lefebvre et al.,
2004)—into the plasma membrane was not by default, but
required cytosolic factors interacting with the nucleotide
binding site of the proton pump. In maize coleoptile,application of the auxin analogue 3-indole acetic acid can
stimulate ER exocytosis and, within minutes, an increase in
the number of H+-ATPases can be detected immunologi-
cally (Hager et al., 1991). Treatment of the coleoptile with
the protein synthesis inhibitor cyclohexamide suggested that
the half-life of an H+-ATPase in this fast-growing tissue was
;12 min. Thus, an increase in H+ extrusion necessary for
growth (the ‘acid-growth’ theory) can be accomplished incertain tissues by enhanced delivery of the proton pump
from the ER to the plasma membrane. Whether there might
be equally dynamic transport of certain H+-ATPases, apart
from PMA2, in the guard cell is not known.
ABA stimulation of stomatal closure:nuclear- and chloroplast-located receptors
Contrary to the effect of light, ABA is synthesized in
conditions of water deficit to trigger stomatal closure, thereby
limiting transpiration. It has already been mentioned above
that the activity of H+-ATPases can be inhibited, at leastpartially (to about 60%), by 10 lM exogenous ABA
(Roelfsema et al., 1998; Zhang et al., 2004). Multiple sites of
ABA perception, inside the cell as well as on the outside of
the cell surface, have been detected by electrophysiological
means for over 15 years (Leung and Giraudat, 1998;
MacRobbie, 1995). The possibility of multiple sites of ABA
perception seems to also correlate with the phenotypic
characterization of two tomato mutants, tos1 and tss2
(Borsani et al., 2002). The mutant tss2 was shown to be
hypersensitive to growth inhibition by exogenous ABA
(Borsani et al., 2001), while tos1, insensitive to ABA,
behaved in a rather similar way to the wild type when grown
on an alkaline medium buffered at pH 8 (Borsani et al.,
2002), which prevents almost completely the entry of ABA
into the cell (Jeannette et al., 1999). Alternatively, the
addition of ABA–BSA conjugate in the medium, which was
too large to penetrate the plasma membrane (Jeannette et al.,
1999), also reduced growth of the tos1 mutant as in the wild
type. The similar results obtained either with ABA–BSA
conjugate or by using pH 8 showed that the insensitivity
phenotype disappears when the ABA is kept extracellularly.The argument by the authors is that tos1 is altered in
intracellular ABA perception or signalling, but the nature of
their corresponding proteins is not known.
In the last few years, several serious candidate intracellu-
lar receptors, some with surprising characteristics, have
been proposed, based on their ability to bind ABA in vitro.
The first reported ABA-binding protein is the homologue of
the H subunit of the larger trimeric Mg2+-chelatase complex(CHLH) protein in Vicia faba (Zhang et al., 2002). The
Arabidopsis homologue is encoded by the ABAR gene which
turns out to be identical to GENOME UNCOUPLED5
(GUS5) (Shen et al., 2006), discovered earlier as being
essential for plastid–nucleus communication and, more
specifically, in the control of chlorophyll synthesis by either
the metabolism or sensing of the tetrapyrrole signal Mg2+-
protoporphyrin-IX. The GUS5/CHLH subunit has there-fore a dual function that generates independent downstream
physiological consequences: in binding to Mg2+-protopor-
phyrin in chlorophyll synthesis and binding to ABA during
adaptive response to dehydration. The knock-down abar
mutant (Shen et al., 2006) has normal chlorophyll content,
but the ABA-inducible genes were down-regulated except
for the the two homologous negative regulators of ABA
signalling, ABI1 and ABI2, which were up-regulatedinstead. Exogenously applied ABA stimulated ABAR ex-
pression, increased Mg2+-chelatase activity and Mg2+-
protoporphyrin content, but suppressed chlorophyll and
protoporphyrin synthesis.
Another candidate came from the biochemical character-
ization of a 52-kDa plasma membrane-localized protein
with a WW-domain from barley aleurone. This protein,
named ABAP1 has been shown to physically bind ABAin vitro (Razem et al., 2004) and this can be weakened by
the presence of H2O2 (Razem and Hill, 2007). Because there
is no detectable change in the overall protein structure
induced by H2O2, the authors have suggested that the
inhibitory effect may represent some form of feedback
regulation directly on the local ABA binding site of the
protein. The search for ABAP1 homologues in Arabidopsis
by the same research group turned up FCA as the closest(Razem et al., 2006), which is rather surprising considering
that this protein has long been recognized for its prominent
role in the control of flowering time by the so-called
autonomous pathway. In contrast to ABAP1 of barley, the
Arabidopsis FCA is not a plasma membrane-localized
protein, but rather a single-stranded RNA-binding protein
that is constitutively nuclear-localized (Macknight et al.,
1997). Binding of ABA to as yet undefined amino acidsinterfered with its interaction, via its WW domain, with
another RNA-binding protein FY, which is similar in
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sequence to the yeast polyadenylation and 3#-end processing
factor PsF2p (Simpson et al., 2003). Interaction of FCA with
FY is obligatory for the correct splicing of the FCA
transcript in a negative feedback loop. The disruption of this
interaction by ABA would thus correlate with a previous
observation that this hormone can cause delays in flowering
(Levy and Dean, 1998). Nonetheless, the purported inhibi-
tory effect of (+)ABA on the in vitro interaction of FCA-FY,and also their homologous rice counterparts has been
questioned recently (Jang et al., 2008). The mutant fca, in
addition, showed no substantial alteration in most of the
classical ABA responses (such as seed germination or
transpiration), except at the level of the lateral roots, which
were found to be reduced in sensitivity to the inhibitory
effects of applied ABA (Razem et al., 2006). There was also
no dramatically altered expression of genes related todrought nor ABA signalling in fca as ascertained by tran-
scriptome analysis (Marquardt et al., 2006). Lastly, there are
still the cell-surface receptors to account for the typical
physiological responses elicited by externally applied ABA on
guard cells (Anderson et al., 1994) and on cell cultures
(Jeannette et al., 1999). Although additional candidates have
surfaced, none possesses all of the characteristics expected of
a cognate ABA receptor, and, in recent months, a so-calledGCR2 has been particularly controversial (Gao et al., 2007;
Johnston et al., 2007; Liu et al., 2007a, b; Chen and Ellis,
2008; Illingworth et al., 2008).
The calcium signal coordinates membranetransporters in stomatal closure
ABA, at least in the guard cell, regulates repetitive cytosolic
free Ca2+ ([Ca2+]cyt) elevations (Mori and Muto, 1997). As
described above, this Ca2+ signal is likely to be responsible
for the inhibition of H+-ATPases possibly via the calcium-
sensitive kinase PKS5 (Fig. 1b). In addition, experimentallyimposed [Ca2+]cyt transients had previously revealed two
distinctive Ca2+-dependent stomatal closing responses:
a rapid so-called ‘Ca2+-reactive’ stomatal closing response,
and a long-lasting ‘Ca2+-programmed’ stomatal response,
which prevailed even after Ca2+ transients have been
terminated (Israelsson et al., 2006). The long-lasting Ca2+-
programmed response, but not the rapid Ca2+-reactive
stomatal closing response, was found to depend on theCa2+ transient pattern. In guard cells, the [Ca2+]cyt elevation
activated the slow- or S-type anion channels by reversible
protein phosphorylation (Schmidt et al., 1995), implying
that calcium-regulated kinases may also be involved in
decoding the Ca2+ signal. Two of such kinases, CPK3 and
CPK6, whose expressions are enriched in guard cells and
are induced by ABA, appear to be excellent candidates.
Indeed, disruption of either one or both of the kinasesimpaired the up-regulation of anion channel currents by
ABA, thereby confirming them as key transducers of the
Ca2+ signal in the guard cell (Mori et al., 2006). When
guard cell protoplasts were incubated in low extracellular
Ca2+, the S-type anion channels only responded moderately
to 2 mM Ca2+ in the pipette. This response can be enhanced
in the wild-type, but not in the mutant, cpk protoplasts by
the addition of ABA. The authors’ interpretation is that
ABA as a stomatal closing signal, mediates by an undefined
mechanism of ‘priming’ of guard cell Ca2+ sensors (among
them, CDPK) such that they can respond to an elevated
Ca2+ signal. These two CDPKs may also have other roles in
the ABA regulation of Ca2+-permeable channels (Israelssonet al., 2006; Mori et al., 2006).
Whether anion channels are direct targets of these Ca2+-
dependent kinases is not yet known. The hunt for the actual
slow anion channels that might be placed squarely in the
ABA signalling pathway itself had also been a long and
torturous quest until recently. The first ‘chloride’ channel
CLC reported turned out to be a nitrate/proton exchanger
(De Angeli et al., 2006). Earlier, there was some evidencebased on pharmacological tests that the anion channel
might correspond to an ATP-binding cassette (ABC) trans-
porter similar to the animal proteins, based on their
sensitivity to the known blocker glibenclamide (Leonhardt
et al., 1999). The mutant Atmrp5 affected in an ABC
transporter has been reported to show impaired Ca2+
signalling and partial ABA-induced anion current activity
as components of its pleiotropic phenotype (Klein et al.,2003; Suh et al., 2007). It is indeed very exciting to note that
independent direct genetic screens for mutants impaired in
stomatal response to either elevated CO2 (Negi et al., 2008)
and ozone (Vahisalu et al., 2008) have converged on slow
anion channel-associated 1 (slac1) as the closest candidate to
the long awaited S-type anion channel. These allelic
mutants turned out to be pleiotropic, being strongly di-
minished not only in anion current and in responding toCO2, ozone, but also to ABA, light/dark transition, Ca2+,
H2O2, and NO, but retained wild-type Ca2+ channel activity
(Vahisalu et al., 2008). Interestingly, slac1 did not affect
rapid (R)-type anion channel current. This observation is
important because it also clarifies the position as to whether
the slow and rapid anion channels are distinct entities or
alternate states of the same channel protein (Vahisalu et al.,
2008). The protein was specifically localized to the plasmamembrane of guard cells and loosely resembled the bacterial
and fungal C4-dicarboxylate/malic acid transporters. One
member of this family in Schizosaccharomyces pombe,
Mae1, had been functionally characterized as a malate
uptake transporter, although the amino acid identity is only
20% to that of SLAC1 (Grobler et al., 1995). Guard cell
protoplasts prepared from slac1 contained higher content of
not only malate, but also fumarate, K+, and Cl– ascompared with those of the wild type. This suggests a broad
default directly or indirectly caused by slac1 in the
homeostasis of organic and inorganic ions.
GORK is the major guard cell outward-rectifying K+ channel
By reverse genetics, a T-DNA insertion was identified in the
GORK gene encoding a potassium inward-rectifying
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channel (Hosy et al., 2003), which has been previously
shown to be highly expressed in the guard cell (Pilot et al.,
2001). Patch-clamp experiments on guard cell protoplasts
derived from gork showed only about 10% residual K+
outward current as compared with the native K+out channel.
A dominant-negative form of gork was produced by
replacing the hallmark motif GYGD (or gly-tyr-gly-asp),
expected to play a pivotal role in the formation of thechannel-conducting pathway (Nakamura et al., 1997), by
introducing the positively charged amino acid arginine (or
R) resulting in RRGD. The dominant-negative behaviour
of this channel was confirmed by heterologous expression in
Xenopus oocytes. These experiments, which involved in-
jection of cRNA produced in vitro, showed that the mutant
channel was electrically silent, and co-injection in parity
with the mutant and wild-type cRNA resulted in >76%inhibition of the GORK current. Similarly, expression of
this gene bearing the dominant negative mutation in stable
transgenic Arabidopsis blocked K+out current in the guard
cells by >90%. Stomatal movement assays in response to
ABA and light-to-darkness transition revealed that both the
disrupted GORK or its dominant negative counterpart
expressed in transgenic Arabidopsis led to reduced closing
response and higher transpirational fluxes in both excisedrosettes and intact plants submitted to progressive drought.
These observations provide clear genetic evidence for the
important function of this K+out channel in regulating
stomatal closure. Note that the knock-out and, particularly,
the dominant-negative form of the gene led to only partial
disruption of this response. This is likely due to the fact that
K+ channel current activities in guard cells are approxi-
mately an order of magnitude larger than physiological K+
fluxes during stomatal movements (Schroeder et al., 1987).
There might also be additional and perhaps more minor K+
efflux mechanisms. For example, the transiently activated
outward-rectifying K+ current IAP might contribute to K+
efflux, which is down-regulated by elevated Ca2+(Pei et al.,
1998).
ABA transport and distribution: theemergence of ABC transporters
Delivering ABA, like other hormones, to the right place
and at the right time is undoubtedly important inoptimizing plant growth in fluctuating environmental
constraints (e.g. light intensity and quality). As has been
epitomized by several excellent studies into auxin redistri-
bution, its gradients and maxima are orchestrated by the
PIN efflux carriers. PIN proteins direct this cell-to-cell
auxin transport, and orient plant development through
their asymmetric subcellular distribution (Robert and
Offringa, 2008). PIN polarity itself is regulated byPINOID and, surprisingly, by the phototropins as well, all
of which are members of the AGC protein serine/threonine
kinase family. In addition to the PIN efflux carriers, there
is also a wealth of evidence for the participation of several
ATP-binding cassette (ABC) proteins. Mutations in the
AtABCB19 locus have recently been found to release the
inhibitory effect of N-1-naphthylphthalamic acid (NPA)
on hypocotyl tropism (Nagashima et al., 2008). Also,
mutations in AtMDR1 and AtPGP1 have provided evi-
dence that relates auxin polar transport to photomorpho-
genesis and root development (Lin and Wang, 2005).
Unlike auxin, the mechanisms by which ABA is trans-
ported have not been extensively explored, probablyhindered by the lack of appropriate chemical inhibitors.
The enzymes that convert xanthoxin eventually into ABA
are expressed in the vascular parenchyma cells of roots and
shoots (Cheng et al., 2002; Koiwai et al., 2004), suggesting
that the vascular system constitutes the major conduit of
long-distance transport. Because not all cells express all
of the biosynthetic and modification enzymes of ABA
(Marion-Poll and Leung, 2006; Wasilewska et al., 2008),the intermediates in the synthetic pathway might be escorted
from one cell type to another for the successive maturation
of the hormone molecule. Using the luciferase gene driven
by promoters sensitive to ABA as a reporter, in vivo
imaging revealed that in transgenic Arabidopsis under ‘non-
stress’ conditions, the hormone is highly concentrated in the
apical meristem and in the guard cells (Christmann et al.,
2004). It is likely that these tissues are more than passivehormone repositories; rather, these observations compel the
question: does ABA have more subtle physiological func-
tions other than in abiotic stress? In responding to drought,
the ABA content increases ;10-fold, most of which will
likely come from de novo synthesis, as the delivery from
enzymatic release of the small pre-existing pool of inactive
ABA conjugate would not be significant to the overall
contribution (Neill et al., 1983; Priest et al., 2006). In fieldconditions, as the soil dries, ABA had been proposed to be
the long-distance messenger that spreads the alarm of water
deficit by moving from root to shoot, and to also play
a major role in orchestrating the subsequent physiological
responses, particularly reducing transpiration by stomatal
closure (Wilkinson and Davis, 2002). The argument in
favour of this root-to-shoot re-distribution of ABA was
inspired by split-root experiments with whole plants, inwhich only part of the root system was exposed to water
deficit. This is also consistent with results from experiments
in which the water status in leaves was maintained by
pressurization of drought-exposed roots that failed to
prevent stomatal closure in herbaceous species (Wilkinson
and Davis, 2002). Evidence to the contrary, however, also
exists. As noted above, the apical meristem and guard cells
in leaves, being the major detectable sites of ABA, alreadyhint at the incongruence with the strict view of root-to-
shoot transport in the moment of stress. Secondly, grafting
of tomato shoots onto root stocks deficient in ABA
biosynthesis indicated root-generated ABA was not re-
quired (Holbrook et al., 2002). Lastly, based on theoretical
considerations, the transport of a chemical signal from
roots to the canopy of tall trees may take >1 d if taking into
account the transpirational streaming speed of 2 m h�1 inconifer xylem (Zimmermann and Brown, 1971). Recently,
through a series of simple but elegant experiments,
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Christmann et al. (2008) tendered the provocative possibil-
ity that the drought alarm is more likely to be a hydraulic
signal instead. They showed that when water was directly
delivered to leaves, even a decrease in soil water potential
sufficient to elicit a strong loss of cell turgor pressure
(expected to be at or near 0 MPa) now proved to be
ineffective. Under these conditions, mesophyll cells
remained turgid (0.3 MPa), with cellular osmotic pressurescomparable to those from well-watered plants (0.38 MPa)
and, in particular, this response was dependent of neither
de novo ABA biosynthesis nor signalling (Christmann
et al., 2008).
What might be the ABA transporters? At this juncture,
we can only speculate. As described above, mutations
affecting certain ABC proteins lead to altered response to
auxin. They are also emerging as prominent integrators ofdiverse signalling pathways in guard cell physiology. These
transporters are encoded by large gene families with
memberships around 100, exist in eukaryotes and prokar-
yotes, and are structurally very diverse. They consist of
mechanochemically coupled integral membrane protein
complexes in which ATP binding and hydrolysis drive
solute transport across membranes. ABC proteins were first
discovered in animals owing to their capacity to exportxenobiotic substances such as toxic drugs, and hence, they
are also known as Multiple Drug Resistance (MDR) trans-
porters. A class of antidiabetic agents, collectively known as
sulphonylureas, are potent inhibitors of ABC transporters
and ATP-sensitive K+ channels in animal tissues (Higgins,
1995). Sulphonylureas can stimulate stomatal opening and
partially inhibit both outward K+ (Leonhardt et al., 1997)
and slow anion currents (Leonhardt et al., 1999) in Vicia
and Commelina. This inhibition is released by vasodilator
agents (e.g. cromakalin) collectively known as KCO which
open K+ channels in animals, or, alternatively, by ABA
treatment which can partially restore the slow anion current
(Leonhardt et al., 1999). In humans, the ABC transporter
CFTR functions as a chloride channel, thereby also blurring
the distinction between transporters and channels (Higgins,
1992, 1995).Three Arabidopsis mutants that are disrupted in genes
encoding specific ABC proteins leading to perturbed
stomatal physiology have been identified so far. Atmrp4 has
wider stomatal aperture as compared with the wild type, but
the mutant phenotype can be restored by ABA, indicating
that the phenotype is not due to a lesion in ABA signalling
(Klein et al., 2004). More recently, a screen of ;20,000 gene
trap lines designed to identify genes preferentially expressedin the guard cells led to the discovery of AtPDR3
(Pleiotropic Drug Resistance 3). Preliminary evidence
showed that disruption of this gene led to reduced
sensitivity of guard cells to ABA (Galbiati et al., 2008).
The relationship between the ATMRP5 and ABA signal-
ling in the guard cell is complex. The stomata of Atmrp5 are
insensitive to several stimuli, including auxin, Ca2+, and
ABA (Klein et al., 2003); more precisely, the mutationappears to impair activation of the anion channels by Ca2+
and ABA (Suh et al., 2007). The average stomatal aperture
of the mutant, despite de-regulated anion channels, is
unexpectedly smaller when compared with that of the wild
type (Klein et al., 2003). The Atmrp5 mutation is rather
pleiotropic (Gaedeke et al., 2001; Klein et al., 2003) and it
might be difficult to distinguish primary and indirect
phenotypic consequences.
Another ABC transporter has been recently reported to
play a role in CO2 sensing through malate transport. Ascompared with the wild type, guard cells on detached leaves
isolated from mutants AtABCB14 were shown to close
more rapidly in responding to high CO2 (800 ppm) and,
conversely, transgenic Arabidopsis plants overexpressing the
gene displayed the opposite phenotype (Lee et al., 2008). By
contrast, the mutant responded normally to light-to-
darkness transition, ABA, and Ca2+. The mutant guard
cells on isolated epidermal strips also close their stomatamore rapidly in malate (20 mM), while the overexpressors
not at all. The phenotype of the Atabcb14 mutant is
therefore roughly opposite to those in slac1. High CO2 has
been shown to increase apoplastic malate from 1 mM to
3 mM, and it was hypothesized that a default in malate
uptake (needed to maintain high osmotic pressure and
stomatal opening) in the mutant might be responsible for
the phenotype. AtABCB14 can partially restore growth ofthe dicarboxylate transporter mutant CBT315 of Escher-
ichia coli, which cannot use malate as a carbon source.
Similarly, expression of this ABC transporter in HeLa cells
can increase malate uptake by 80%. These results reinforce
the hypothesis that AtABCB14 controls stomatal movement
by importing malate from the apoplastic space into guard
cells, thereby increasing their osmotic pressure.
Reversible protein phosphorylation-basedpathways underpin rapid regulation ofstomatal movements: mechanistic insightsderived from genetic and molecular analysis
Correct interpretation of mutant phenotypes can sometimes
provide invaluable molecular insights into signalling or
developmental events. Recessive mutations are, as a general
rule, much easier to interpret because they must entail
a partial or full loss of function (usually catalytic activity).
Dominant mutations are, by comparison, more open todebate because their underlying causes can be multiple in
origin. One of the first regulators in ABA signal trans-
duction was identified by a single dominant mutation abi1-1
(Koornneef et al., 1984), which rendered the mutant highly
insensitive to exogenous ABA, reduced seed dormancy, and
hypersensitive to mild water deficit. The gene encodes a 2C-
type protein phosphatase (Leung et al., 1994; Meyer et al.,
1994; Bertauche et al., 1996; Leube et al., 1998) that canstably exist in monomeric forms (Leube et al., 1998).
Because the PP2C catalytic activity of the ABI1 is acutely
sensitive to pH and a shift from 7.2 (in prevailing cytosolic
condition) to pH 7.5 (during ABA signalling) would be
expected to double the ABI1 activity (Leube et al., 1998),
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this PP2C might be one of the important cytosolic factors
in the pH-dependent pathway in modulating K+ fluxes
(Blatt, 1992, 2000; Blatt and Armstrong, 1993) (see above).
ABI1 might also be the target of inactivation by the
second messenger H2O2 produced during ABA signalling,
thus implying the existence of a negative feedback loop
(Meinhard and Grill, 2001).
An important and intriguing publication has recentlyrevealed that the manifestation of the various ABA-
insensitivity phenotypes required nuclear localization of the
protein, and that the abi1-1 mutation resulted in the
preferential accumulation of the protein in the nucleus
(Moes et al., 2008). Application of the proteasome inhibitor
MG-132 led to both a preferential nuclear accumulation of
the wild-type ABI1 and an enhancement of PP2C-
dependent inhibitory action of the ABA responses. Theseobservations indeed contribute critically towards an under-
standing—admittedly still partial—of the ABI1 regulatory
function. At the whole plant level, numerous genetic
analyses had already defined a negative regulatory role for
the wild-type ABI1 in ABA signalling, and this function is
not altered but rather reinforced by the mutation abi1-1 in
that the mutant protein also blocks ABA sensitivity—even
constitutively. At the molecular level, the mutation renderedthe nuclear form of the PP2C more stable, which can be
recapitulated by MG-132 treatment of the wild-type ABI1
protein. A first conclusion is that the ABI1 is dynamically
regulated by proteolysis (and perhaps also inactivation by
H2O2, as mentioned above). That this dominant mutation
has a stabilizing effect against ubiquitin-mediated proteoly-
sis on the protein is indeed in accordance with an earlier
report of an extragenic revertant of abi1-1, named sleepy1
or sly1 (Steber et al., 1998). SLY1 encodes an F-box subunit
of an SCF E3 ubiquitin ligase complex (McGinnis et al.,
2003). Here, we further venture the prediction that the
mutant sly1 subunit in the E3 ligase complex might be more
efficient that its wild-type counterpart in promoting abi1-1
destruction, thereby relieving constitutive inhibition by this
mutated PP2C on the ABA signalling pathway. In survey-
ing the current literature on hormone signalling for clues, itwas found that this predicted mechanism bears striking
resemblance to the case of another sly allelic mutant (gar2-
1) E3 ligase subunit which, as compared with its wild-type
counterpart, has a higher affinity towards its substrates
which are certain members of the so-called DELLA
proteins, especially when they are phosphorylated (GAI
and RGA). These proteins function in growth restraints
during GA signalling. Presumably the mutant slygar2-1
promotes a much more efficient degradation of the phos-
phorylated DELLA proteins by the ubiquitin-proteasome
complex (Fu et al., 2004). A second and more tentative
conclusion drawing from GA signalling as an analogy is
that the Asp replacement in abi1-1, being more negatively
charged and mimicking a phosphorylated amino acid near
the catalyic site (Das et al., 1996), may increase its
degradation as it would be targeted more efficiently by themutant sly E3 ligase (this is why the mutant sly1 was
isolated as an extragenic suppressor of abi1-1). The simple
but elegant demonstration of Moes et al. (2008) portends
that the unbiquitin-mediated proteolysis, a rather common
mechanism in regulating other hormone signals up to now,
might also be an integral part of the ABI1 pathway.
Whether the mutation abi1-1 in itself causes an absolute
excess of catalytic activity in vivo as compared with its wild-
type counterpart—independent of the gain in protein
stability—is not clear, although this dominant mutationhas also been alternatively interpreted as ‘hypermorphic’
(Robert et al., 2006; Moes et al., 2008). This interesting
possibility is nonetheless entertained by the identification of
a particular 2A-type protein phosphatase, PP2Ac-2, that
when disrupted, can also partially suppress the various
elementary ABA-insensitivity phenotypes caused by the
abi1-1 mutation (Pernas et al., 2007). This possibility of
excess protein phosphatase activity is also corroborated bya second independent observation that numerous second-
site loss-of-function mutations dispersed within the mutant
abi1-1 gene (i.e. intragenic suppressor mutations) all re-
versed the ABA-insensitivity phenotype towards that of the
wild-type and, in some cases, even causing mild ABA
hypersensitivity (Gosti et al., 1999). Importantly, recombi-
nant abi1-1 proteins containing these intragenic second site
substitutions expressed in E. coli are enzyme-dead, or nearlyso, towards casein as the in vitro substrate (Gosti et al.,
1999). Thus any hypothetical excess PP2C activity caused
by abi1-1 is completely neutralized by either mutating
another phosphatase (PP2Ac-2) or second-site intragenic
mutations dispersed elsewhere in the same protein.
One major problem associated with the hypothesis
privileging excess PP2C activity caused by the abi1-1
mutation is that it has never been detected by the currentavailable in vitro biochemical tests. In fact, all these tests
used commercial casein as the classical surrogate substrate
and, paradoxically, a consistent partial loss of phosphatase
catalytic activity was rather observed (Bertauche et al.,
1996; Leube et al., 1998; Sheen, 1998). One could perhaps
reconcile that the presumed excess phosphatase activity
engendered by abi1-1 could not have been detected because
all phosphatase tests had relied on an animal protein as thesubstrate. The alternative possibility is that the presumed
excess of catalytic activity and the gain in protein stability is
in fact one and the same phenomenon. That is, the
dominant mutation might in fact cause: (i) a partial loss of
in vivo catalytic activity relative to that of the wild-type
counterpart, but at the same time (ii) this deficit is more
than offset by the gain in stability that it bestows on the
protein against ubiquitin-mediated proteolysis, as suggestedby the combined results of Steber et al. (1998), McGinnis
et al. (2003), and Moes et al. (2008).
In plants, the phenotype provoked by the loss-of-function
revertant alleles of abi1 (including those caused by T-DNA
insertions) is mild and hardly distinguishable from that of
the wild type. This can be explained readily by the largely
overlapping functions of at least three other homologous
PP2Cs in ABA signalling (Schweighofer et al., 2004),including the closest homologue ABI2, initially identified
through the same dominant mutation as that found in
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abi1-1 (Koornneef et al., 1984; Leung et al., 1997;
Rodriguez et al., 1998) that can compensate for one
another. Thus, a third conclusion based on analysis of these
loss-of-function alleles is that the ABI1-regulated part of
the signalling chain must be critical, as it is assured by at
least four functionally redundant PP2C, in addition to the
aforementioned one controlled by PP2Ac-2 (Pernas et al.,
2007). This is attested by the fact that a surprisingly largenumber of mutations affecting ABA perception, including
the putative receptor abar (see above), lead to perturbed
expression of the ABI1 gene, but presumably, any impact
would be largely buffered by genic redundancy. These
observations further suggest that these parallel protein
phosphatase pathways have common downstream targets.
The abi1-1 (as well as abi2-1) mutation impairs the rise in
Ca2+ (Allen et al., 1999) which blocks ABA responses of K+
and anion channels (Armstrong et al., 1995; Grabov et al.,
1997; Pei et al., 1997). The homologous AtPP2CA, one of
the redundant negative regulators of ABA signalling
(Sheen, 1998), has been shown to bind directly to the
potassium channel AKT2 in yeast, and the K+ channel
characteristics can be influenced by AtPP2CA observable by
co-expression in Xenopus oocytes (Cherel et al., 2002).
Similar interaction and functional tests with membranetransporters have not been carried out with ABI1. It is thus
not clear whether the impact of the abi1-1 mutation on ion
transport is direct or not.
One of the in planta cognate targets of the ABI1 is almost
certainly to be the ABA-activated kinase OPEN STO-
MATA1 (OST1), as these two proteins can interact in
a directed yeast two-hybrid assay (Yoshida et al., 2006).
Mutations in the OST1 locus led to guard cells that areunresponsive to the ABA signal and low humidity (Merlot
et al., 2002; Mustilli et al., 2002; Yoshida et al., 2002; Xie
et al., 2006), similar to some of the vegetative phenotypes
engendered by the abi1-1 mutation. As referred to earlier in
the section dealing with the Ca2+ signal, the ost1 mutation
blocks the production of the second messenger H2O2
(Mustilli et al., 2002). The OST1 belongs to the SnRK2
family with a membership of 10 in the Arabidopsis genome(Hrabak et al., 2003). The OST1 kinase (also known as
Srk2e and SnRK2.6) has a relatively conserved N-terminal
catalytic domain and a more divergent regulatory C-
terminal domain. A small stretch of amino acids, known as
domain II, localized to the extreme end of the C-terminus is
functionally required for ABA activation of the kinase
activity and, incidentally, is the docking site for the ABI1
(Yoshida et al., 2006). Although the biological consequen-ces of this interaction between ABI1 and OST1 have not
been pursued in these studies, examples abound in the
animal field that have shown PP2Cs to be negative
regulators of AMP-activated kinases (Moore et al., 1991;
Hardie, 2007) (which are homologues of Sucrose Non-
Fermenting kinase or Snf1 of yeast, and Snf1-Related
Kinases or SnRKs of plants). Moreover, these kinases in
yeast and animals assume important roles as energy sensorsto switch off ATP-consuming anabolic pathways in times of
stress while switching on ATP-producing catabolic path-
ways (Hardie, 2007). Since ABI1 has been defined as
a negative regulator of ABA signalling by genetics and by
in vitro reconstitution assays (Sheen, 1998; Gosti et al.,
1999), combining with the obvious parallel with the animal
systems, it is almost certain that ABI1 negatively regulates
OST1. There seems to be, however, an additional surprising
layer of negative regulation of the OST1, as suggested by
the crystal structure of the yeast homologue Snf1. Duringthe earlier directed yeast two-hybrid test between OST1 and
certain heteronuclear RNA-binding proteins as potential
substrates (Riera et al., 2006), it had been found that OST1
itself can homodimerize. It has been possible subsequently
to confirm this dimer formation in living plant cells by
BiFC analysis as well (Fig. 2c), although the meaning of the
homodimerization in the functional context was not obvi-
ous at the time. The crystal structure of the kinase domainof the Snf1 had been determined recently and, surprisingly,
it revealed a novel dimer (Nayak et al., 2006). These Sfn1
dimers exist in cells as determined by co-immunoprecipita-
tion using antibodies that could selectively recover one or
the other epitope-tagged Snf1. The particular conformation
of the conserved aC helix harbouring phosphate-binding
residues, and the masking of the activation segment, as well
as the substrate binding site within the groove formed bythe dimer, suggest that dimerization is a new mechanism
that maintains the inactive state of the kinase. Strikingly,
the interface was formed by the most-conserved residues
of the Snf1/AMPK kinases, being predominantly in the
T-loop activation segment and the loop-aG region of the
kinase domain. This implies that dimer formation is
a conserved feature of the Snf1/AMPK kinases and could
extend to OST1.In plants, the SnRK2 kinases have been characterized in
terms of their biochemical activities in most detail in
Arabidopsis and rice (Hrabak et al., 2003; Boudsocq et al.,
2004; Kobayashi et al., 2004). These kinases phosphor-
ylate context-dependent serine and threonine residues, and
representative members from Arabidopsis (OST1/Srk2e,
SnRK2.2, 2.3, 2.8) and from rice (SAPK 8, 9, 10) that have
been tested can all phosphorylate peptides derived from theconstant (C) domain in the b-ZIP class of transcription
factors containing the motif Arg–3–X–2–X–1–pSer/pThr
(where the pSer/pThr denotes phosphorylated serine or
threonine arbitrarily fixed at position ‘0’ in the degenerate
peptide, and the positions of the other amino acids in the
motif are denoted with a ‘–’ relative to this serine/threonine)
(Kobayashi et al., 2005; Furihata et al., 2006; Chae et al.,
2007). Thus, based on the in vitro phosphorylation of thesepeptides, SnRK2 kinases are thought to target b-ZIP
proteins to regulate gene transcription (Kobayashi et al.,
2005; Furihata et al., 2006; Chae et al., 2007). Physical
interaction between homologues of an SnRK kinase and
b-ZIP proteins from wheat has also been detected in yeast
two-hybrid screens (Johnson et al., 2002). Some b-ZIP
transcription factors have been shown to bind with avidity
in vitro to the core ABA-Responsive Element (ABRE,PyACGTGGC), enriched in certain promoters up-regulated
by ABA.
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On the basis of quantitative phosphorylation of an array
of semi-degenerate peptides using SnRK2-10 as test kinase,
the consensus sequence Leu–5–X–4–Arg–3–X–2–X–1–pSer/
pThr was derived (Vlad et al., 2008). The importance of the
Arg–3 was therefore independently confirmed (Furihata
et al., 2006; Vlad et al., 2008); moreover, this kinase also
has preference for hydrophobic amino acids at the –5
position, particularly Leu. The importance of Leu–5 can bein fact retrospectively confirmed from the study by others:
this amino acid was consistently present in the peptides
derived from Arabidopsis and rice b-ZIP transcription
factors that were phosphorylated efficiently by the SnRK2
(Kobayashi et al., 2005; Furihata et al., 2006), and was
absent from the single test peptide derived from a so-called
C3 domain that was also inefficiently phosphorylated
(Furihata et al., 2006). An undeniable advantage conferredby the technology of phosphorylation of soluble peptide
arrays (Hutti et al., 2004) is that it allows the prediction of
preferred or disfavoured amino acids at the variable
(denoted as X in the motifs) positions based on their
quantitative influence on the phosphorylation of the central
serine/threonine. This in turn allows the generation of
theoretical peptide sequences, ranked in hierarchical prefer-
ences, which can be used to match against proteins annotedin a given genome. The dehydrins, in addition to b-ZIP
transcription factors, stand out as another major category
of potential direct targets (Vlad et al., 2008), whose
functions are often attributed to be in osmotic adjustments
by binding ions or protection of membranes during re-
sponse to environmental stresses (Puhakainen et al., 2004;
Kariola et al., 2006).
A proteomics approach had also been used to identifytargets of SnRK2.8 in planta (Shin et al., 2007) by
comparing the profiles of the phosphoproteins in transgenic
plants ectopically expressing SnRK2.8 with those of a corre-
sponding insertion mutant. These experiments targeted
phosphoproteins migrating between pI values of 3.9–5.1
and pI 4.7–5.9 representing ;70% of the total phosphopro-
teins set by these defined limits of isoelectric points. Nine
candidate target proteins were retained, and further testsrevealed that seven of these were phosphorylatable in vitro
by SnRK2.8. Among the seven candidates, three were 14-3-
3 isoforms, and, by comparing their sites of phosphoryla-
tion, the deduced motifs were DYRPSKVE on 14-3-3j and
DYRPSKIE on 14-3-3v (Shin et al., 2007). Note that
SnRK2.8 was the identical test kinase in two of the above
independent studies carried out by Furihata et al. (2006)
and Shin et al. (2007), and yet no conservation in the motifswas observed between the 14-3-3 proteins and those in the
b-ZIP transcription factors or dehydrins. Particularly in-
congruent is Asp rather than Arg at position –3 in the 14-3-
3 proteins, because Asp had been predicted to be a very
disfavoured residue for this type of kinase (Vlad et al.,
2008). Perhaps the sample sizes are still too small to draw
any conclusion concerning a ‘consensus’ or ‘preferred’
phosphorylation site of SnRK2 and, moreover, the possibil-ity cannot be excluded that the two different experimental
approaches may have cryptic technical biases.
Transcription factors in regulating guard cellmovements
Transcriptional control in stomatal movement is a burgeon-
ing field of inquiry into ABA signalling, which will be
a valuable complement to the wealth of knowledge already
gleaned from that on volume control of guard cell through
active membrane transport mechanisms. Gene expression
has been traditionally considered as a relatively late event in
the unfolding sequence of guard cell signalling but, in
nature, where guard cells are exposed to continual fluctua-
tions of micro-meteological changes, the processes of cell
volume control by membrane transport and transcriptional
events are probably much more tightly integrated. There is
indirect but nonetheless tantalizing evidence for changes
in RNA composition in the guard cells that might be link-
ed to stomatal movements in response to environmental
stimuli. In brief, up-regulation of mRNA, particularly one
encoding the AtPP2CA (see above) that can be detected in
Arabidopsis guard cell protoplasts upon treatment with
ABA (Leonhardt et al., 2004), and a number of mutations
affecting guard cell response to drought as part of
their pleiotropic affects are impaired in RNA metabolism
(Wasilewska et al., 2008).
We have already alluded to the prominent role of some b-
ZIP domain proteins in ABA signalling by their affinity
towards promoters containing the ABRE motif to trigger
transcription. Very recently, the activity of several MYB
transcription factors has also been shown to influence
stomatal movements in response to environmental stimuli.
The name MYB is attributed to their structural similarity to
cellular proto-oncogenes in animals (Lipsick, 1996). The
MYB family in Arabidopsis comprises 163 genes, making it
one of the largest transcription factor families (Chen et al.,
2006). Three in the so-called R2R3 subclass, which has
a membership of 126, have been shown to influence stomatal
movements in response to different environmental stimuli.
The diagnostic feature in this subclass of MYB transcription
factors is the two to three 50- to 53-amino-acid imperfect
repeats that form the helix-turn-helix motifs R1, R2, and R3
(Rosinsky and Atchley, 1998). In plants, two-repeat (R2-
R3) MYB family members predominate. The transcript of
AtMYB44 was shown to be rapidly induced (within 30 min)
by dehydration, low temperature, high salinity, exogenous
JA, ethylene, and ABA (Jung et al., 2008). Overexpression
of the gene led to an overall hypersensitivity to ABA and
a more rapid stomatal response to ABA than the wild type.
However, there were pleiotropic effects as well, such as
smaller stomatal structures, but no difference in stomatal
density was noted, suggesting that AtMYB44 plays a role in
development. These transgenic plants showed reduced
activation of several key negative regulators of ABA signal-
ling, including ABI1 and ABI2 by stress conditions, most
notably high salt, and conversely, the transcript levels of
these key regulators were enhanced in the knock-out
Atmyb44 mutant.
Two other R2R3–MYB transcription factors were found
to participate in light/dark sensing of guard cells, and these
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results have been reviewed recently (Gray, 2005). Again in
brief, the two transcription factors, AtMYB60 and
AtMYB61, play opposing roles in response to light. The
expression of AtMYB60 is environmentally regulated, being
reduced by darkness and ABA, which are signals that
stimulate stomatal closure. There was no absolute correla-
tion with expression levels of this gene with stomatal closure
per se because CO2, while effective in inducing stomatalclosure, has no effect on gene expression. By contrast,
AtMYB60 was up-regulated by light (which stimulates
stomatal opening) (Cominelli et al., 2005). The other,
AtMYB61, seemed to be expressed only in darkness (closed
stomata), and not at all in the light. Very interestingly, this
expression seemed ‘specific’ to darkness, as neither ABA
nor drought exerted any impact and, in accordance,
darkness-induced stomatal closure, but not that from ABA,was also impaired in the Atmyb61 insertion mutant (Liang
et al., 2005). These findings thus provide additional evidence
that transcriptional activity in the guard cell is linked to cell
volume control via membrane transport.
Concluding remarks
Guard cells and their attendant mechanisms to withstand
bouts of water deficit have no doubt contributed to the
successful terrestrial adaptation of plants from their former
aquatic confines. The appropriate and continual ajustment
of stomatal aperture by these cells in land plants are vitalfor optimal CO2 uptake necessary for photosynthesis, yet
preventing excessive water loss by transpiration. Engineer-
ing guard cells to be more sensitive to low humidity has
proven successful in reducing water consumption of a crop
plant without noticeable sacrifice in seed yield (Wang et al.,
2005). Because guard cells have no plasmadesmata, the
adaptive responses are thus cell-autonomous, rendering
them essentially a biological ‘test tube’. These properties,and the indissociable link between stomatal closure and low
humidity, make the stomatal complex an ideal system for
inquisitive probing into drought-adaptative mechanisms by
biophysics, genetics, and molecular biology. The membrane
voltage in guard cells can undergo large (>100 mV) and
rapid (10 s period) oscillations between hyperpolarized
and depolarized values allowing K+ uptake and release,
respectively (Gradmann et al., 1993; Gradmann andHoffstadt, 1998). This led to the hypothesis that the control
of stomatal movement and steady-state aperture depends on
variations in the pattern of these oscillations, enabling the
net guard cell K+ content to increase or decrease as a result
of changes in the balance of, respectively, K+ uptake
through hyperpolarization-activated, and K+ release
through depolarization-activated channels (Gradmann
et al., 1993; Gradmann and Hoffstadt, 1998). As summa-rized in Fig. 1b, in Arabidopsis guard cells, K+ uptake is
mainly through KAT1 and KAT2, while K+ release is
largely mediated by GORK. In the last two years, the
identification of a specific H+-ATPase (OST2) and an anion
channel (SLAC1) has also been witnessed. These newer
additions complete the major categories of plasma mem-
brane transporters, whose existence in the guard cell plasma
membrane had been inferred from biophysics for more than
a decade. The next obvious challenge is to work out the
mechanistic details on how these transporters are individ-
ually regulated, as well as how their activities are globally
coordinated to bring about rapid membrane hyper- and
de-polarization. For instance, the activation mechanismsof H+-ATPases by structural conversion from a dimer to
a hexamer remain unclear. Crystallographic data based on
PMA2 of tobacco showed that the C-terminal inhibitory
domain can be further divided into ‘R’ subdomains
(Ottmann et al., 2007). There are still many open questions
concerning the function of the RI subdomain, to which
some mutations have been mapped (Merlot et al., 2007). It
remains unclear how RI can influence the phosphorylationat the penultimate Thr in the RII subdomain. Ottmann
et al. (2007) speculated that RI influences inter-RII in-
teraction between the two H+-ATPase units in the dimer
(the inactive form) to facilitate hexamer formation (the
active form). It seems, beyond the well-established model
of intramolecular interaction between the C-termini and
the rest of the protein (Palmgren, 2001), there may be
other parallel activation mechanisms. It is also unclearhow the mutation ost2-1D, predicted to locate in the first
transmembrane domain (Merlot et al., 2007), could in-
fluence accessibility to the penultimate Thr for phosphor-
ylation. On the other hand, the exact deactivation
mechanisms of H+-ATPases are also not completely
known, with the exception of the PSK5 kinase which
phosphorylates Ser931 of AHA2 to block 14-3-3 protein
binding. Whether this is the critical amino acid that alsodirectly governs the structural conversion of the complex
from hexamer to dimer is not clear.
It is also likely that more refined genetics screens will
reveal other novel types of transporters (and their regu-
lators) as they are encoded by large families in Arabidopsis.
The few ABC transporter mutants that are affected in
stomatal function display pleiotropic phenotypes and this
fact may reflect the possibility that each transporter iscapable of transporting a large spectrum of substances,
which is the hallmark property that contrasts them with
selective channels. Pinpointing the precise substance(s)
transported by each of individual ABC protein would thus
be an arduous task. Furthermore, these substances could
range from simple organic and inorganic ions to complex
macromolecules like lipids, or even nucleic acids. For
example, in Caenorhabditis elegans, 10 of the 60 ABCtransporters are required to propagate gene silencing by
RNA interference, suggesting that they may transport RNA
(Timmons, 2007). Even identification of the transported
substance(s) does not automatically give clues about their
specific physiological functions in a cellular context. Many
of the ABC proteins are said to be bifunctional; that is,
independent of the substance(s) transported, ABC proteins
can also impose specific regulatory functions, most likely bycomplexing with other structurally diverse proteins in the
membrane (Higgins, 1992).
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A partial reversion of the mutant phenotype of abi1-1 by
the presence of the pp2ac-2 mutation would strongly imply
that the overall and absolute amount of catalytic activities
contributed by members of these two protein phosphatase
families must be tightly balanced to down-regulate ABA
signalling properly. Also, although the immediate down-
stream cognate targets of the PP2Ac-2 and the PP2Cs might
be distinct, the genetic observations do suggest that theircorresponding sub-branches of the signalling pathways are
most likely to later converge. The fact that ABI1 exerts its
important physiological functions relevant to ABA signal-
ling in the nucleus suggests that the post-translational
modification in the nucleus is different from that in the
cytoplasm. One such modification would render the protein
a selective target of ubiquitin-mediated proteolysis. The
nuclear localization of ABI1 has been interpreted to meanthat transcription is required for the observable phenotypic
events, including stomatal closure to limit transpiration
evoked by ABA (Moes et al., 2008). Indeed, there had been
tantalizing evidence in the past that transcriptional activity
in the guard cell is important for volume control. For
example, the activities of the K+in channels are curtailed by
ABA, and this is also paralleled by the down-regulation of
the KAT1 transcript level (Leonhardt et al., 2004). Manytranscripts in guard cell protoplasts are also stimulated by
ABA, and are driven by promoters enriched in the ABRE
motif. Besides the b-ZIP domain transcription factors,
which have been known for almost 20 years to be involved
in ABA-mediated gene transcription (Guiltinan et al., 1990),
some members of the R2R3 MYB class have now surfaced.
How membrane transport and nuclear events are wedded to
execute stomatal responses to a variety of environmentalconstraints is not obvious, and this problem will have to be
solved if we are to procure a more integrated vision.
Membrane transport mechanisms and transcriptional events
in the guard cell have been treated traditionally as distinct
temporal events. For instance, the stimulatory effects on ion
transport in the plasma membrane of the guard cell that
lead ultimately to stomatal closure can be detected within
seconds upon ABA application (Levchenko et al., 2005).These rapid physiological responses at the plasma mem-
brane are thus unlikely to be a direct consequence of the
presumably time-consuming transcriptional events. A guard
cell in a laboratory setting, however, is invariably chal-
lenged by such sudden and high doses of applied hormones
(or other pharmaceutical agents). In a natural setting, the
guard cell is rather continually exposed to micro-meteolog-
ical fluctuations in CO2, light intensities, and ambianttemperatures. Gene transcription, mRNA translation, and
ion transport across endo- and plasma membranes are most
likely to be integrated events, at least in time if not in space.
Acknowledgements
The authors appreciate the thoughtful comments from the
two anonymous reviewers. We are also grateful to Alejan-
dro Ferrando Monleon for the unconditional use of his
unpublished vectors and sound advice in the BiFC experi-
ments, and Marie-Noelle Soler of the Imaging and Cell
Biology facility of the IFR87 for expert support with
confocal microscopy. Work carried out in the authors’
laboratory was generously funded by the Ministere de la
Recherche Doctoral Fellowship (CS, Universite Paris XI),
European Union Marie-Curie Early Stage Training Fellow-
ships MEST-CT-2005-020232-2 ADONIS (AW and FV),Genoplante GNP05037G ABRUPT (JL), and the Centre
National de la Recherche Scientifique (JL and CV).
References
Allen GI, Muir SR, Sanders D. 1995. Release of Ca2+ from individual
plant vacuoles by both InsP3 and cyclic ADP-ribose. Science 268,
735–737.
Allen GJ, Kuchitsu K, Chu SP, Murata Y, Schroeder JI. 1999.
Arabidopsis abi1-1 and abi2-1 phosphatase mutations reduce absci-
sic acid-induced cytoplasmic calcium rises in guard cells. The Plant
Cell 11, 1785–1798.
Amtmann A, Armengaud P, Volkov V. 2004. Potassium nutrition
and salt stress. In: Blatt MR, ed. Membrane transport in plants.
Oxford: Blackwell, 316–346.
Anderson BE, Ward JM, Schroeder JI. 1994. Evidence for an
extracellular reception site for abscisic acid in Commelina guard cells.
Plant Physiology 104, 1177–1183.
Armstrong F, Leung J, Grabov A, Brearley J, Giraudat J,
Blatt MR. 1995. Sensitivity to abscisic acid of guard-cell K+ channels
is suppressed by abi1-1, a mutant Arabidopsis gene encoding
a putative protein phosphatase. Proceedings of the National Academy
of Sciences, USA 92, 9520–9524.
Artsaenko O, Peisker M, Mieden UZ, Fiedler U, Weiler EW,
Muntz K, Conrad U. 1995. Expression of a single-chain Fv antibody
against abscisic acid creates a wilty phenotype in transgenic tobacco.
The Plant Journal 8, 745–750.
Baizabal-Aguirre VM, Clemens S, Uozumi N, Schroeder JI. 1999.
Suppression of inward-rectifying K+ channels KAT1 and AKT2 by
dominant negative point mutations in the KAT1 a-subunit. Journal of
Membrane Biology 167, 119–125.
Bertauche N, Leung J, Giraudat J. 1996. Protein phosphatase
activity of abscisic acid insensitive 1 (ABI1) protein from Arabidopsis
thaliana. European Journal of Biochemistry 241, 193–200.
Blatt MR. 1991. Ion channel gating in plants: physiological implica-
tions and integration for stomatal function. Journal of Membrane
Biology 124, 95–112.
Blatt MR. 1992. K+ channels of stomatal guard cells: characteristics
of the inward rectifier and its control by pH. Journal of General
Physiology 99, 615–644.
Blatt MR. 2000. Cellular signaling and volume control in stomatal
movements in plants. Annual Review of Cell Developmental Biology
16, 221–241.
Blatt MR, Armstrong F. 1993. K+ channels of stomatal guard cells:
abscisic-acid evoked control of the outward rectifier mediated by
cytoplasmic pH. Planta 191, 330–341.
The guard cell as a single-cell model | 1455 by guest on Septem
ber 12, 2016http://jxb.oxfordjournals.org/
Dow
nloaded from
Blatt MR, Thiel G, Trentham DR. 1990. Reversible inactivation of K+
channels of Vicia stomatal guard cells following the photolysis of
caged inositol 1,4,5-trisphosphate. Nature 346, 766–771.
Blazer-Yost BL, Liu X, Helman SI. 1998. Hormonal regulation of
ENaCs: insulin and aldosterone. American Journal of Physiology – Cell
Physiology 274, C1373–C1379.
Borsani O, Cuartero J, Fernandez JA, Valpuestra V, Botella MA.
2001. Identification of two loci in tomato reveals distinct mechanisms
for salt tolerance. The Plant Cell 13, 873–888.
Borsani O, Cuartero J, Valpuestra V, Botella MA. 2002. Tomato
tos1 mutation identifies a gene essential for osmotic tolerance and
abscisic acid sensitivity. The Plant Journal 32, 905–914.
Boudsocq M, Barbier-Brygoo H, Lauriere C. 2004. Identification of
nine SNF1-related protein kinases 2 activated by hyperosmotic and
saline stresses in Arabidopsis thaliana. Journal of Biological Chemistry
279, 41758–41766.
Brault M, Amiar Z, Pennarun A-M, Montstiez M, Zhang Z,
Cornel D, Dellis O, Knight H, Bouteau F, Rona J-P. 2004. Plasma
membrane depolarization induced by abscisic acid in Arabidopsis
suspension cells involves reduction of proton pumping in addition to
anion channel activation, which are both Ca2+ dependent. Plant
Physiology 135, 231–243.
Bruggemann L, Dietrich P, Dreyer I, Hedrich R. 1999. Pro-
nounced differences between the native K+ channels and KAT1 and
KST1 alpha-subunit homomers of guard cells. Planta 207, 370–376.
Chae MJ, Lee JS, Nam MH, Cho K, Hong JY, Yi SA, Suh SC,
Yoon IS. 2007. A rice dehydration-inducible SNF1-related protein
kinase 2 phosphorylates an abscisic acid responsive element binding
factor and associates with ABA signalling. Plant Molecular Biology 63,
151–169.
Chen J, Ellis BE. 2008. GCR2 is a new member of the eukaryotic
lanthionine synthase component C-like protein family. Plant Signaling
and Behavior 3, 307–310.
Chen Y, Yang X, He K, et al. 2006. The MYB transcription factor
superfamily of Arabidopsis: expression analysis and phylogenetic
comparison with the rice MYB family. Plant Molecular Biology 60,
107–124.
Cheng WH, Endo A, Zhou L, et al. 2002. A unique short-chain
dehydrogenase/reductase in Arabidopsis glucose signaling and absci-
sic acid biosynthesis and functions. The Plant Cell 14, 2723–2743.
Cherel I, Michard E, Platet N, Mouline K, Alcon C, Sentenac H,
Thibaud J-B. 2002. Physical and functional interaction of the
Arabidopsis K+ channel AKT2 and phosphatase AtPP2CA. The Plant
Cell 14, 1133–1146.
Christmann A, Hoffmann T, Teplova I, Grill E, Muller A. 2004.
Generation of active pools of abscisic acid revealed by in vivo imaging
of water-stressed Arabidopsis. Plant Physiology 137, 209–219.
Christmann A, Weiler EW, Steudle E, Grill E. 2008. A hydraulic
signal in root-to-shoot signalling of water shortage. The Plant Journal
52, 167–174.
Cominelli E, Galbiati M, Vavasseur A, Conti L, Sala T,
Vuylsteke M, Leonhardt N, Dellaporta S, Tonelli C. 2005. A
guard-cell specific MYB transcription factor regulates stomatal move-
ments and plant drought tolerance. Current Biology 15, 1196–1200.
Daram P, Urbach S, Gaymard F, Sentenac H, Cherel I. 1997.
Tetramerization of the AKT1 plant potassium channel involves its C-
terminal cytoplasmic domain. EMBO Journal 16, 3455–3463.
Das AK, Helps NR, Cohen PTW, Barford D. 1996. Crystal structure
of the protein serine/threonine phosphatase 2C at 2.0 A resolution.
EMBO Journal 15, 6798–6809.
De Angeli A, Monachello D, Ephitikhine G, Frachisse JM,
Thomine S, Gambale F, Barbier-Brygoo H. 2006. The nitrate/
proton antiporter AtCLCa mediates nitrate accumulation in plant
vacuoles. Nature 442, 939–942.
Desikan R, Horak J, Chaban C, et al. 2008. The histidine kinase
AHK5 integrates endogenous and environmental signals in Arabidop-
sis guard cells. Public Library of Science One 3, e2491.
Dietrich P, Dreyer I, Wiesner P, Hedrich R. 1998. Cation sensitivity
and kinetics of guard cell potassium channels differ among species.
Planta 205, 277–287.
Dietrich P, Sanders D, Hedrich R. 2001. The role of ion channels in
light-dependent stomatal opening. Journal of Experimental Biology 52,
1959–1967.
Dittrich P, Raschke K. 1977. Uptake and metabolism of carbohy-
drates by epidermal tissue. Planta 134, 83–90.
Dreyer I, Mueller-Roeber B, Kohler B. 2004. Voltage-gated ion
channels. In: Blatt MR, ed. Membrane transport in plants. Oxford:
Blackwell, 150–192.
Emi T, Knoshita T, Sakamoto K, Mineyuki Y, Shimazaki K-i.
2005. Isolation of a protein interacting with Vfphot1a in guard cells of
Vicia faba. Plant Physiology 138, 1615–1626.
Emi T, Kinoshita T, Shimazaki K. 2001. Specific binding of vf14-3-
3a isoform to the plasma membrane H+-ATPase in response to blue
light and fusicoccin in guard cells of broad bean. Plant Physiology 125,
1115–1125.
Erlij D, de Smet P, van Dreissche W. 1994. Effect of insulin on area
and Na+ channel activity of apical membrane of cultured toad kidney
cells. Journal of Physiology 481, 533–542.
Fairley-Grenot K, Assmann S. 1991. Evidence for G-protein
regulation of inward K+ channel current in guard cells of Fava Bean.
The Plant Cell 3, 1037–1044.
Fu X, Richards DE, Fleck B, Xie D, Burton N, Harberd NP. 2004.
The Arabidopsis mutant sleepygar2-1 protein promotes plant growth by
increasing the affinity of the SCFSLY1 E3 ubiquitin ligase for DELLA
protein substrates. The Plant Cell 16, 1406–1418.
Fuglsang AT, Guo Y, Cuin TA, et al. 2007. Arabidopsis
protein kinase PKS5 inhibits the plasma membrane H+-ATPase
by preventing interaction with 14-3-3 protein. The Plant Cell 19,
1617–1634.
Fuglsang AT, Tulinius G, Cui N, Palmgren MG. 2006. Protein
phosphatase 2A scaffolding subunit A interacts with plasma mem-
brane H+-ATPase C-terminus in the same region as 14-3-3 protein.
Physiologia Plantarum 128, 334–340.
Furihata T, Maruyama K, Fujita Y, Umezawa T, Yoshida R,
Shinozaki K, Yamaguchi-Shinozaki K. 2006. Abscisic acid-
dependent multisite phosphorylation regulates the activity of a tran-
scription activator AREB1. Proceedings of the National Academy of
Sciences, USA 103, 1988–1993.
1456 | Sirichandra et al. by guest on Septem
ber 12, 2016http://jxb.oxfordjournals.org/
Dow
nloaded from
Gaedeke N, Klein M, Kolukisaoglu U, et al. 2001. The Arabidopsis
thaliana ABC transporter AtMRP5 controls root development and
stomata movement. EMBO Journal 20, 1875–1887.
Galbiati M, Simoni L, Pavesi G, Cominelli E, Francia P,
Vavasseur A, Nelson T, Bevan M, Tonelli C. 2008. Gene trap lines
identify Arabidopsis genes expressed in stomatal guard cells. The
Plant Journal 53, 750–762.
Gao Y, Zeng Q, Guo J, Cheng J, Ellis BE, Chen J-G. 2007.
Genetic characterization reveals no role for the reported ABA receptor,
GCR2, in ABA control of seed germination and early seedling
development in Arabidopsis. The Plant Journal 52, 1001–1013.
Garcia-Mata C, Gay R, Slkolovski S, Hills A, Lamattina L, Blatt MR.
2003. Nitric oxide regulates K+ and Cl– channels in guard cells through
a subset of abscisic acid-evoked signaling pathways. Proceedings of the
National Academy of Sciences, USA 100, 11116–11121.
Gierth M, Maser P. 2007. Potassium transporters in plants –
involvement in K+ acquisition, redistribution and homeostasis. FEBS
Letters 581, 2348–2356.
Gilroy S, Read ND, Trewavas AJ. 1990. Elevation of cytoplasmic
calcium by caged calcium or caged inositol trisphosphate initiates
stomatal closure. Nature 346, 769–771.
Gosti F, Beaudoin N, Serizet C, Webb AAR, Vartanian N,
Giraudat J. 1999. ABI1 protein phosphatase 2C is a negative
regulator of abscisic acid signaling. The Plant Cell 11, 1897.
Gotow K, Taylor S, Zeiger E. 1988. Photosynthetic carbon fixation
in guard cell protoplasts of Vicia faba L.: evidence from radiolabel
experiments. Plant Physiology 86, 700–705.
Grabov A, Blatt MR. 1997. Parallel control of the inward-rectifier K+
channel by cytosolic free Ca2+ and pH in Vicia guard cells. Planta 201,
84–95.
Grabov A, Blatt MR. 1999. A steep dependence of inward-rectifying
potassium channels on cytosolic free calcium concentration increase
evoked by hyperpolarization in guard cells. Plant Physiology 119,
277–287.
Grabov A, Leung J, Giraudat J, Blatt MR. 1997. Alteration of anion
channel kinetics in wild-type and abi1-1 transgenic Nicotiana ben-
thamiana guard cells by abscisic acid. The Plant Journal 12, 203–213.
Gradmann D, Blatt MR, Thiel G. 1993. Electrocoupling of ion
transporters in plants. Membrane Biology 136, 327–332.
Gradmann D, Hoffstadt J. 1998. Electrocoupling of ion transporters
in plants: interaction with internal ion concentrations. Journal of
Membrane Biology 166, 51–59.
Gray J. 2005. Guard cells: transcription factors regulate stomatal
movements. Current Biology 15, R593–R595.
Gray JE, Holroyd GH, van der Lee FM, Bahrami AR, Sijmons PC,
Woodward FI, Schuch W, Hetherington AM. 2000. The HIC
signalling pathway links CO2 perception to stomatal development.
Nature 408, 713–716.
Grobler J, Bauer F, Subden RE, van Vuuren HJ. 1995. The mae1
gene of Schizosaccharomyces pombe encodes a permease for malate
and other C4 dicarboxylic acids. Yeast 11, 1485–1491.
Guiltinan MJ, Marcotte WR, Quatrano RS. 1990. A plant leucine
zipper protein that recognizes an abscisic acid response element.
Science 250, 267–271.
Hager A, Debus G, Edel H-G, Stansky H, Serrano R. 1991. Auxin
induced exocytosis and the rapid synthesis of a high-turnover pool of
plama membrane H+-ATPase. Planta 185, 527–537.
Hardie DG. 2007. AMP-activated/SNF1 protein kinases: conserved
guardians of cellular energy. Nature Reviews of Molecular Cellular
Biology 8, 774–785.
Hedrich R, Busch H, Raschke K. 1990. Ca2+ and nucleotide
dependent regulation of voltage dependent anion channels in the
plasma membrane of guard cells. EMBO Journal 9, 3889–3892.
Hetherington AM, Woodward FI. 2003. The role of stomata in
sensing and driving environmental change. Nature 424, 901–908.
Higgins CF. 1992. ABC transporter: from microorganisms to man.
Annual Review of Cell Biology 8, 67–113.
Higgins CF. 1995. The ABC of channel regulation. Cell 82, 693–696.
Holbrook NM, Shashidhar VR, James RA, Munns R. 2002.
Stomatal control in tomato with ABA-deficient roots: response of
grafted plants to soil drying. Journal of Experimental Botany 53,
1503–1514.
Homann U. 1998. Fusion and fission of plasma membrane material
accommodates for osmotically induced changes in surface area in
guard-cell protoplasts. Planta 206, 329–333.
Homann U, Meckel T, Hewing J, Hutt M-T, Hurst AC. 2007.
Distinct fluorescent pattern of KAT1:GFP in the plasma membrane
of Vicia faba guard cells. European Journal of Cell Biology 86,
489–500.
Homann U, Thiel G. 2002. The number of K+ channels in the plasma
membrane of guard cell protoplasts changes in parallel with the
surface area. Proceedings of the National Academy of Sciences, USA
99, 10215–10220.
Hosy E, Vavasseur A, Mouline K, et al. 2003. The Arabidopsis
outward K+ channel GORK is involved in regulation of stomatal
movements and plant transpiration. Proceedings of the National
Academy of Sciences, USA 100, 5549–5554.
Hoth S, Dreyer I, Dietrich P, Becker D, Muller-Rober B,
Hedrich R. 1997. Molecular basis of plant-specific acid activation of
K+ uptake channel. Proceedings of the National Academy of Sciences,
USA 94, 4806–4810.
Hrabak EM, Chan CWM, Gribskov M, et al. 2003. The Arabidopsis
CDPK-SnRK superfamily of protein kinases. Plant Physiology 132,
666–680.
Hurst AC, Meckel T, Tayefeh S, Thiel G, Homann U. 2004.
Trafficking of the plant potassium inward rectifying KAT1 in guard cell
protoplasts of Vicia faba. The Plant Journal 37, 391–397.
Hutti JE, Jarrell ET, Chang JD, Abbott DW, Storz P, Toker A,
Cantley LC, Turk BE. 2004. A rapid method for determining protein
kinase phosphorylation specificity. Nature Methods 1, 27–29.
Ilan N, Schwartz A, Moran N. 1996. External protons enhance the
activity of the hyperpolarization-activated K+ channels in the guard
cell protoplasts of Vicia faba. Journal of Membrane Biology 154,
168–181.
Illingworth CJ, Parkes KE, Snell CR, Mullineaux PM,
Reynolds CA. 2008. Criteria for confirming sequence periodicity
identified by Fourier transform analysis: application to GCR2, a candi-
date plant GPCR? Biophysical Chemistry 133, 28–35.
The guard cell as a single-cell model | 1457 by guest on Septem
ber 12, 2016http://jxb.oxfordjournals.org/
Dow
nloaded from
Inada S, Ohgishi M, Mayama T, Okada K, Sakai T. 2004. RPT2 is
a signal transducer involved in phototropic response and stomata
opening by association with phototropin 1 in Arabidopsis thaliana. The
Plant Cell 16, 887–896.
Irving HR, Gehring CA, Parish RW. 1992. Changes in cytosolic pH
and calcium of guard cells precede stomatal movements. Proceedings
of the National Academy of Sciences, USA 89, 1790–1794.
Israelsson M, Siegel RS, Young J, Hashimoto M, Iba K,
Schroeder JI. 2006. Guard cell ABA and CO2 signaling network
updates and Ca2+ sensor priming hypothesis. Current Opinions in
Plant Biology 9, 654–663.
Jacob T, Ritchie S, Assmann SM, Gilroy S. 1999. Abscisic acid
signal transduction in guard cells is mediated by phospholipase D
activity. Proceedings of the National Academy of Sciences, USA 96,
12192–12197.
Jang YH, Lee JH, Kim J-K. 2008. Abscisic acid does not disrupt
either the Arabidopsis FCA-FY interaction or its rice counterpart
in vitro. Plant and Cell Physiology DOI: 10.1093/pcp/pcn1151.
Jeannette E, Ronna J-P, Bardat F, Cornel D, Sotta B,
Miginiac E. 1999. Induction of RAB18 gene expression and
activation of K+ outward rectifying channels depend on an
extracellular perception of ABA in Arabidopsis thaliana suspension
cells. The Plant Journal 18, 13–22.
Johnson RR, Wagner RL, Verhey SD, Walker-Simmons MK.
2002. The abscisic acid-responsive kinase PKABA1 interacts with
a seed-specific abscisic acid response element-binding factor, TaABF,
and phosphorylates TaABF peptide sequences. Plant Physiology 130,
837–846.
Johnston CA, Temple BR, Chen JG, Gao Y, Moriyama EN,
Jones AM, Siderovski DP, Willard FS. 2007. Comment on ‘A G
protein-coupled receptor is a plasma membrane receptor for the plant
hormone abscisic acid’. Science 318, 914c.
Jung C, Seo JS, Han SW, Koo YJ, Kim CH, Song SI, Nahm BH,
Choi YD, Cheong J-J. 2008. Overexpression of AtMYB44 enhances
stomatal closure to confer abiotic stress tolerance in transgenic
Arabidopsis. Plant Physiology 146, 623–635.
Kanczewska J, Marco S, Vandermeeren C, Maudoux O,
Rigaud J-L, Boutry M. 2005. Activation of the plant plasma
membrane H+-ATPase by phosphorylation and binding of 14-3-3
proteins converts a dimer into a hexamer. Proceedings of the National
Academy of Sciences, USA 102, 11675–11680.
Kariola T, Brader G, Helenius E, Li J, Heino P, Palva ET. 2006.
EARLY RESPONSIVE TO DEHYDRATION 15, a negative regulator of
abscisic acid responses in Arabidopsis. Plant Physiology 142, 1559–
1573.
Kelly WB, Esser JE, Schroeder JI. 1995. Effects of cytosolic
calcium and limited, possible dual, effects of G protein modulators on
guard cell inward potassium channels. The Plant Journal 8, 479–489.
Kinoshita T, Doi M, Suetsugu N, Kagawa T, Wada M,
Shimazaki K. 2001. phot1 and phot2 mediate blue light regulation of
stomatal opening. Nature 414, 656–660.
Kinoshita T, Shimazaki K. 1997. Involvement of calyculin A- and
okadaic acid-sensitive protein phosphatase in blue light response of
stomatal guard cells. Plant and Cell Physiology 38, 1281–1285.
Kinoshita T, Shimazaki K. 2001. Analysis of the phosphorylation
level in guard-cell plasma membrane H+-ATPase in response to
fusicoccin. Plant and Cell Physiology 42, 424–432.
Kinoshita T, Shimazaki K-i. 1999. Blue light activates the plasma
membrane H+-ATPase by phosphorylation of the C-terminus in
stomatal guard cells. EMBO Journal 18, 5548–5558.
Klein M, Geisler M, Suh SJ, et al. 2004. Disruption of AtMRP4,
a guard cell plasma membrane ABCC-type ABC transporter, leads to
deregulation of stomatal opening and increased drought susceptibility.
The Plant Journal 39, 219–236.
Klein M, Perfus-Barbeoch L, Frelet A, Gaedeke N, Reinhardt D,
Mueller-Roeber B, Martinoia E, Forestier C. 2003. The plant
multidrug resistance ABC transporter AtMRP5 is involved in guard
cell hormonal signalling and water use. The Plant Journal 33,
119–129.
Kleizen B, Braakman I, de Jong HR. 2000. Regulated trafficking of
the CFTR chloride channel. European Journal of Cell Biology 79,
544–556.
Kobayashi Y, Murata M, Minami H, Yamamoto S, Kagaya Y,
Hobo T, Yamamoto A, Hattori T. 2005. Abscisic acid-activated
SNRK2 protein kinases function in the gene-regulation pathway of
ABA signal transduction by phosphorylation ABA response element-
binding factors. The Plant Journal 44, 939–949.
Kobayashi Y, Yamamoto S, Minami H, Kagaya Y, Hattori T.
2004. Differential activation of the rice sucrose nonfermenting1-related
protein kinase2 family by hyperosmotic stress and abscisic acid. The
Plant Cell 16, 1163–1177.
Koiwai H, Nakaminami K, Seo M, Mitsuhashi W, Toyomasu T,
Koshiba T. 2004. Tissue-specific localization of an abscisic acid
biosynthetic enzyme, AAO3, in Arabidopsis. Plant Physiology 134,
1697–1707.
Koornneef M, Jorna ML, Brinkhorst-van der Swan DLC,
Karssen CM. 1982. The isolation of abscisic acid (ABA) deficient
mutants by selection of induced revertants in non-germinating
gibberellin sensitive lines of Arabidopsis thaliana (L.) Heynh. Theoretical
and Applied Genetics 61, 385–393.
Koornneef M, Reuling G, Karssen CM. 1984. The isolation and
characterization of abscisic acid-insensitive mutants of Arabidopsis
thaliana. Physiologia Plantarum 61, 377–383.
Kwak JM, Mori IC, Pei ZM, Leonhardt N, Torres MA, Dangl JL,
Bloom RE, Bodde S, Jones JD, Schroeder JI. 2003. NADPH
oxidase AtrbohD and AtbohF genes function in ROS-dependent ABA
signaling in Arabidopsis. EMBO Journal 22, 2623–2633.
Kwak JM, Murata Y, Baizabal-Aguirre VM, Merrill J, Wang M,
Kemper A, Hawke SD, Tallman G, Schroeder JI. 2001. Dominant
negative guard cell K+ channel mutants reduce inward-rectifying K+
currents and light-induced stomatal opening in Arabidopsis. Plant
Physiology 127, 473–485.
Lebaudy A, Hosy E, Simonneau T, Sentenac H, Thibaud J-B,
Dreyer I. 2008a. Heteromeric K+ channels in plants. The Plant Journal
54, 1076–1082.
Lebaudy A, Vavasseur A, Hosy E, Dreyer I, Leonhardt N,
Thibaud J-B, Very A-A, Simmoneau T, Sentenac H. 2008b. Plant
adaptation to fluctuating environment and biomass production are
1458 | Sirichandra et al. by guest on Septem
ber 12, 2016http://jxb.oxfordjournals.org/
Dow
nloaded from
strongly dependent on guard cell potassium channels. Proceedings of
the National Academy of Sciences, USA 105, 5271–5276.
Lebaudy A, Very A-A, Sentenac H. 2007. K+ channel activity in
plants: genes, regulations and functions. FEBS Letters 581, 2357–
2366.
Leckie CP, McAinsh MR, Allen GJ, Sanders D,
Hetherington AM. 1998. Abscisic acid-induced stomatal closure
mediated by cyclic ADP-ribose. Proceedings of the National Academy
of Sciences, USA 95, 15837–15842.
Lee M, Choi YB, Burla B, Kim Y-Y, Jeon B, Maeshima M,
Yoo J-Y, Martinoia E, Lee Y. 2008. The ABC transporter AtABCB14
is a malate importer and modulates stomatal response to CO2. Nature
Cell Biology DOI: 10.1038/ncb1782.
Lee YS, Choi YB, Suh S, Lee J, Assmann S, Joe CO, Kelleher JF,
Crain RC. 1996. Abscisic acid-induced phosphoinositide turnover in
guard cell protoplasts of Vicia faba. Plant Physiology 110, 987–996.
Lefebvre B, Batoko H, Duby G, Boutry M. 2004. Targeting of
a Nicotiana plumbaginifolia H+-ATPase to the plasma membrane is not
by default and requires cytosolic structural determinants. The Plant
Cell 16, 1772–1789.
Lemtiri-Chlieh F, MacRobbie EAC, Webb AAR, Manison NF,
Brownlee C, Skepper JN, Chen J, Prestwich GD, Brearley CA.
2003. Inositol hexakisphosphate mobilizes an endomembrane store of
calcium in guard cells. Proceedings of the National Academy of
Sciences, USA 100, 10091–10095.
Leonhardt N, Kwak JM, Robert N, Waner D, Leonhardt G,
Schroeder JI. 2004. Microarray expression analyses of Arabidopsis
guard cells and isolation of a recessive abscisic acid hypersensitive
protein phosphatase 2C mutant. The Plant Cell 16, 596–615.
Leonhardt N, Marin E, Vavasseur A, Forestier C. 1997. Evidence
for the existence of a sulfonylurea-receptor-like protein in plants:
modulation of stomatal movements and guard cell potassium
channels by sulfonylureas and potassium channel openers. Proceedings
of the National Academy of Sciences, USA 94, 14156–14161.
Leonhardt N, Vavasseur A, Forestier C. 1999. ATP binding
cassette modulators control abscisic acid-regulated slow anion
channels in guard cells. The Plant Cell 11, 1141–1151.
Leon-Kloorsterziel KM, Gil MA, Ruijs GJ, Jacobsen SE,
Olszewski NE, Schwartz SH, Zeevaart JAD, Koornneef M. 1996.
Isolation and characterisation of abscisic acid-deficient Arabidopsis
mutants at two new loci. The Plant Journal 10, 655–661.
Leube MP, Grill E, Amrhein N. 1998. ABI1 of Arabidopsis is
a protein serine/threonine phosphatase highly regulated by the proton
and magnesium ion concentration. FEBS Letters 424, 100–104.
Leung J, Bouvier-Durand M, Morris P-C, Guerrier D, Chefdor F,
Giraudat J. 1994. Arabidopsis ABA response gene ABI1: features
of a calcium-modulated protein phosphatase. Science 264, 1448–
1452.
Leung J, Giraudat J. 1998. Abscisic acid signal transduction. Annual
Review of Plant Physiology and Plant Molecular Biology 49, 199–222.
Leung J, Merlot S, Giraudat J. 1997. The Arabidopsis ABSCISIC
ACID-INSENSITIVE 2 (ABI2) and ABI1 genes encode homologous
protein phosphatases 2C involved in abscisic acid signal transduction.
The Plant Cell 9, 759–771.
Levchenko V, Konrad KR, Dietrich P, Roelfsema MRG,
Hedrich R. 2005. Cytosolic abscisic acid activates guard cell anion
channels without preceding Ca2+ signals. Proceedings of the National
Academy of Sciences, USA 102, 4203–4208.
Levy Y, Dean C. 1998. The transition to flowering. The Plant Cell 10,
1973–1990.
Leyman B, Geelen D, Quintero FJ, Blatt MR. 1999. A tobacco
syntaxin with a role in hormonal control of guard cell ion channels.
Science 283, 537–540.
Li J, Assmann SM. 1996. An abscisic acid-activated and calcium-
independent protein kinase from guard cells of Fava bean. The Plant
Cell 8, 2359–2368.
Li J, Lee Y-RJ, Assmann SM. 1998. Guard cells possess a calcium-
dependent protein kinase that phosphorylates the KAT1 potassium
channel. Plant Physiology 116, 785–795.
Li J, Wang X-Q, Watson MB, Assmann SM. 2000. Regulation of
abscisic acid-induced stomatal closure and anion channels by guard
cell AAPK kinase. Science 287, 300–303.
Liang Y-K, Dubois C, Dodd IC, Holroyd GH, Hetherington AM,
Campbell MM. 2005. AtMYB61, an R2R3-MYB transcription factor
controlling stomatal aperture in Arabidopsis thaliana. Current Biology
15, 1201–1206.
Lin R, Wang H. 2005. Two homologous ATP-binding cassette
transporter proteins, AtMDR1 and AtPGP1, regulate Arabidopsis
photomorphogenesis and root development by mediating polar
auxin transport. Plant Physiology 138, 949–964.
Lipsick JS. 1996. One billion years of Myb. Oncogene 13, 223–235.
Liu X, Yue Y, Li B, Nie Y, Li W, Wu W-H, Ma L. 2007a. A G protein-
coupled receptor is a plasma membrane receptor for the plant
hormone abscisic acid. Science 315, 1712–1716.
Liu X, Yue Y, Li W, Ma L. 2007b. Response to comments on ‘A G-
protein-coupled receptor is a plasma membrane receptor for the plant
hormone abscisic acid’. Science 318, 914d.
Lu P, Outlaw WHJ, Smith BG, Freed GA. 1997. A new mechanism
for the regulation of stomatal aperture size in intact leaves (accumula-
tion of mesophyll-derived sucrose in the guard-cell wall of Vicia faba).
Plant Physiology 114, 109–118.
Macknight R, Bancroft I, Page T, et al. 1997. FCA, a gene
controlling flowering time in Arabidopsis, encodes a protein
containing RNA-binding domains. Cell 99, 737–745.
MacRobbie EAC. 1995. ABA-induced ion efflux in stomatal guard
cells: multiple actions of ABA inside and outside the cell. The Plant
Journal 7, 565–576.
MacRobbie EAC. 2000. ABA activates multiple Ca2+ fluxes in
stomatal guard cells, triggering vacuolar K+ (Rb+) release. Proceedings
of the National Academy of Sciences, USA 97, 12361–12368.
Marin E, Nussaume L, Quesada A, Gonneau M, Sotta B,
Hugueney B, Frey P, Marion-Poll A. 1996. Molecular identifica-
tion of zeaxanthin epoxidase of Nicotiana plumbaginifolia, a gene
involved in abscisic acid biosynthesis and corresponding to
the ABA locus of Arabidopsis thaliana. EMBO Journal 15,
2331–2342.
Marion-Poll A, Leung J. 2006. Abscisic acid synthesis, metabolism
and signal transduction. In: Hedden P, Thomas SG, eds. Plant
The guard cell as a single-cell model | 1459 by guest on Septem
ber 12, 2016http://jxb.oxfordjournals.org/
Dow
nloaded from
hormone signaling. Annual Plant Reviews, Vol. 24. Oxford: Blackwell
Publishing, 1–35.
Marquardt S, Boss PK, Hadfield J, Dean C. 2006. Additional
targets of the Arabidopsis autonomous pathway members, FCA and
FY. Journal of Experimental Botany 57, 3379–3386.
Marten H, Konrad KR, Dietrich P, Roelfsema MRG, Hedrich R.
2007. Ca2+-dependent and -independent abscisic acid activation of
plasma membrane anion channels in guard cells of Nicotiana
tabacum. Plant Physiology 143, 28–37.
Masle J, Gilmore SR, Farquhar GD. 2005. The ERECTA gene regu-
lates plant transpiration efficiency in Arabidopsis. Nature 436, 866–870.
McAinsh MR, Brownlee C, Hetherington AM. 1997. Calcium ions
as second messengers in guard cell signal transduction. Plant
Physiology 100, 16–29.
McGinnis KM, Thomas SG, Soule JD, Strader LC, Zale JM,
Sun T-P, Steber CM. 2003. The Arabidopsis SLEEPY1 gene
encodes a putative F-box subunit of an SCF E3 ubiquitin ligase. The
Plant Cell 15, 1120–1130.
Meckel T, Hurst AC, Thiel G, Homann U. 2004. Endocytosis
against high turgor: intact guard cells of Vicia faba constitutively
endocytose fluorescently labelled plasma membrane and GFP-tagged
K+-channel KAT1. The Plant Journal 39, 182–193.
Meinhard M, Grill E. 2001. Hydrogen peroxide is a regulator of ABI1,
a protein phosphatase 2C from Arabidopsis. FEBS Letters 508,
443–446.
Meinhard M, Rodriguez PL, Grill E. 2002. The sensitivity of ABI2 to
hydrogen peroxide links the abscisic acid-response regulator to redox
signalling. Planta 214, 775–782.
Merlot S, Leonhardt N, Fenzi F, et al. 2007. Constitutive activation
of a plasma membrane H+-ATPase prevents abscisic acid-mediated
stomatal closure. The EMBO Journal 26, 3216–3226.
Merlot S, Mustilli A-C, Genty B, North H, Lefebvre V, Sotta B,
Vavasseur A, Giraudat J. 2002. Use of infrared thermal imaging to
isolate Arabidopsis mutants defective in stomatal regulation. The Plant
Journal 30, 601–609.
Meyer K, Leube MP, Grill E. 1994. A protein phosphatase 2C
involved in ABA signal transduction in Arabidopsis thaliana. Science
264, 1452–1455.
Meyer S, Lauterbach C, Niedermeier M, Barth I, Sjolund RD,
Sauer N. 2004. Wounding enhances expression of ATSUC3, a su-
crose transporter from Arabidopsis sieve elements and sink tissues.
Plant Physiology 134, 684–693.
Miedema H, Assmann SM. 1996. A membrane-delimited effect of
internal pH on the K+-outward rectifier of Vicia faba guard cells.
Journal of Membrane Biology 154, 227–237.
Mikosch M, Hurst AC, Hertel B, Homann U. 2006. Diacidic motif is
required for efficient transport of the K+ channel KAT1 to the plasma
membrane. Plant Physiology 142, 923–930.
Moes D, Himmelbach A, Korte A, Haberer G, Grill E. 2008.
Nuclear localization of the mutant protein phosphatase abi1 is required
for insensitivity towards ABA responses in Arabidopsis. The Plant
Journal 54, 806–819.
Moore F, Weekes J, Hardie DG. 1991. Evidence that AMP triggers
phosphorylation as well as direct allosteric activation of rat liver AMP-
activated protein kinase. European Journal of Biochemistry 199,
691–697.
Mori IC, Murata Y, Yang Y, et al. 2006. CDPKs CPK6 and CPK3
function in ABA regulation of guard cell S-type anion- and Ca2+-
permeable channels and stomatal closure. Public Library of Science
Biology 4, e327. DOI: 310.1371/journal.p bio.0040327.
Mori IC, Muto S. 1997. Abscisic acid activates a 48-kilodalton
protein kinase in guard cell protoplasts. Plant Physiology 113, 883–
839.
Mori IC, Uozumi N, Muto S. 2000. Phosphorylation of the inward-
rectifying potassium channel KAT1 by ABR kinase in Vicia guard cell.
Plant and Cell Physiology 41, 850–856.
Motchoulski AV, Liscum E. 1999. Arabidopsis NPH3: a NPH1
photoreceptor-interacting protein that is essential for phototropism.
Science 286, 961–964.
Mustilli A-C, Merlot S, Vavasseur A, Fenzi F, Giraudat J. 2002.
Arabidopsis OST1 protein kinase mediates the regulation of stomatal
aperture by abscisic acid and acts upstream of reactive oxygen
species production. The Plant Cell 14, 3089–3099.
Nagashima A, Uehara Y, Sakai T. 2008. The ABC subfamily B auxin
transporter AtABCB19 is involved in the inhibitory effects of N-1-
naphthyphthalamic acid on the phototropic and gravitropic responses
of Arabidopsis hypocotyls. Plant and Cell Physiology DOI: 10.1093/
pcp/pcn1092.
Nakamura RL, Anderson JA, Gaber RF. 1997. Determination of key
structural requirements of a K+ channel pore. Journal of Biological
Chemistry 272, 1011–1018.
Nayak V, Zhao K, Wyce A, Schwartz MF, Lo W-S, Berger SL,
Marmostein R. 2006. Structure and dimerization of the kinase
domain from yeast Snf1, a member of the Snf1/AMPK protein family.
Structure 14, 477–485.
Negi J, Matsuda O, Nagasawa T, Oba Y, Takahashi H, Kawai-
Yamada M, Uchimiya H, Hashimoto M, Iba K. 2008. CO2 regulator
SLAC1 and its homologues are essential for anion homeostasis in
plant cells. Nature 452, 483–486.
Neill S, Barros R, Bright J, Desikan R, Hancock J, Harrison J,
Morris P, Ribeiro D, Wilson I. 2008. Nitric oxide, stomatal closure,
and abiotic stress. Journal of Experimental Botany 59, 165–176.
Neill SJ, Horgan R, Heald JK. 1983. Determination of the levels of
abscisic acid-glucose ester in plants. Planta 157, 371–375.
Nishimura N, Balch WE. 1997. A di-acidic signal required for
selective export from the endoplasmic reticulum. Science 277,
556–558.
Ottmann C, Marco S, Jaspert N, et al. 2007. Structure of a 14-3-3
coordinated hexamer of the plant plasma membrane H+-ATPase by
combining X-ray crystallography and electron cryomicroscopy. Molec-
ular Cell 25, 427–440.
Outlaw WHJ, Manchester J, DiCamelli CA, Randall DD, Rapp B,
Veith GM. 1979. Photosynthetic carbon reduction pathway is absent
in chloroplasts of Vicia faba guard cells. Proceedings of the National
Academy of Sciences, USA 76, 6371–6375.
Palmgren MG. 2001. Plant plasma membrane H+-ATPases: power-
houses for nutrient uptake. Annual Review of Plant Physiology and
Plant Molecular Biology 52, 817–845.
1460 | Sirichandra et al. by guest on Septem
ber 12, 2016http://jxb.oxfordjournals.org/
Dow
nloaded from
Pedersen BP, Buch-Pedersen MJ, Morth JP, Palmgren MG,
Nissen P. 2007. Crystal structure of the plasma membrane proton
pump. Nature 450, 1111–1114.
Pei Z-M, Baizabal-Aguirre VM, Allen GI, Schroeder J. 1998. A
transient outward-rectifying K+ channel current down-regulated by
cytosolic Ca2+ in Arabidopsis thaliana guard cells. Proceedings of the
National Academy of Sciences, USA 95, 6548–6553.
Pei Z-M, Kuchitsu K, Ward JM, Schwarz M, Schroeder JI. 1997.
Differential abscisic acid regulation of guard cell slow anion channels in
Arabidopsis wild-type and abi1 and abi2 mutants. The Plant Cell 9,
409–423.
Pei Z-M, Murata Y, Benning G, Thomine S, Klusener B, Allen GJ,
Grill E, Schroeder JI. 2000. Calcium channels activated by hydrogen
peroxide mediate abscisic acid signalling in guard cells. Nature 406,
731–734.
Pernas M, Garcia-Casado G, Rojo E, Solano R, Sanchez-
Serrano JJ. 2007. A protein phosphatase 2A catalytic subunit is
a negative regulator of abscisic acid signaling. The Plant Journal 51,
763–778.
Pilot G, Lacombe B, Gaymard F, Cherel I, Boucherez J,
Thibaud J-B, Sentenac H. 2001. Guard cell inward K+ channel
activity in Arabidopsis involves expression of the twin channel subunits
KAT1 and KAT2. Journal of Biological Chemistry 276, 3215–3221.
Priest DM, Ambrose SJ, Vaistij FE, Elias L, Higgins GS,
Ross AR, Abrams SR, Bowles DJ. 2006. Use of the glucosyltrans-
ferase UGT71B6 to disturb abscisic acid homeostasis in Arabidopsis
thaliana. The Plant Journal 46, 492–502.
Puhakainen T, Hess MW, Makela P, Svensson J, Heino P,
Palva T. 2004. Overexpression of multiple dehydrin genes enhances
tolerance to freezing stress in Arabidopsis. Plant Molecular Biology 54,
743–753.
Raschke K. 1979. Movements of stomata. In: Haupt W, Feinlieb E,
eds. Encyclopaedia of plant physiology. Berlin: Springer, 383–441.
Raskin I, Ladyman JAR. 1988. Isolation and characterization of
a barley mutant with abscisic acid-insensitive stomata. Planta 173,
73–78.
Razem FA, El-Kereamy A, Abrams SR, Hill RD. 2006. The RNA-
binding protein FCA is an abscisic acid receptor. Nature 439,
290–294.
Razem FA, Hill RD. 2007. Hydrogen peroxide affects abscisic acid
binding to ABAP1 in barley aleurones. Biochemistry and Cell Biology
85, 628–637.
Razem FA, Luo M, Liu J-H, Abrams ZR, Hill RD. 2004. Purification
and characterization of a barley aleurone abscisic acid-binding protein.
Journal of Biological Chemistry 279, 9922–9929.
Reckmann U, Sheibe R, Raschke K. 1990. Rubisco activity in
guard cells compared with the solute requirement for stomatal
opening. Plant Physiology 92, 246–253.
Reddy AR, Das VSR. 1986. Stomatal movements and sucrose
uptake by guard cell protoplasts of Commelina bengbalensis L. Plant
and Cell Physiology 27, 1565–1570.
Riera M, Redko Y, Leung J. 2006. Arabidopsis RNA-binding protein
UBA2a relocalizes into nuclear speckles in response to abscisic acid.
FEBS Letters 580, 4160–4165.
Ritte G, Rosenfeld J, Rohrig K, Raschke K. 1999. Rates of sugar
uptake by guard cell protoplasts of Pisum sativum L. related to the
solute requirement for stomatal opening. Plant Physiology 121,
647–656.
Robert HS, Offringa R. 2008. Regulation of auxin transport polarity
by AGC kinases. FEBS Letters 11 DOI: 10.1016/
j.pbi.2008.1006.1004.
Robert N, Merlot S, N’Guyen V, Boisson-Dernier A, Schroeder J.
2006. A hypermorphic mutation in the protein phosphatase 2C HAB1
strongly affects ABA signaling in Arabidopsis. FEBS Letters 580,
4691–4696.
Rodriguez PL, Benning G, Grill E. 1998. ABI2, a second protein
phosphatase 2C involved in abscisic acid signal transduction in
Arabidopsis. FEBS Letters 421, 185–190.
Roelfsema MRG, Hedrich R. 2005. In the light of stomatal opening:
new insights into ‘the Watergate’. New Phytologist 165, 665–691.
Roelfsema MR, Konrad KR, Marten H, Psaras GK, Hartung W,
Hedrich R. 2006. Guard cells in albino leaf patches do not respond to
photosynthetically active radiation, but are sensitive to blue light, CO2
and abscisic acid. Plant, Cell & Environment 29, 1595–1605.
Roelfsema MRG, Prins HBA. 1998. The membrane potential of
Arabidopsis thaliana guard cells: depolarization induced by apoplastic
acidification. Planta 205, 100–112.
Roelfsema MRG, Staal M, Prins HBA. 1998. Blue light-induced
apoplastic acidification of Arabidopsis thaliana guard cells: inhibition by
ABA is mediated through protein phosphatases. Physiologia Planta-
rum 103, 466–474.
Rosinsky JA, Atchley WR. 1998. Molecular evolution of the MYB
family of transcription factors: evidence for polyphyletic origin. Journal
of Molecular Evolution 46, 74–83.
Sakai T, Wada T, Ishiguro S, Okada K. 2000. RPT2: a signal
transducer of the phototropic response in Arabidopsis. The Plant Cell
12, 225–236.
Schmidt C, Schelle I, Liao Y-J, Schroeder JI. 1995. Strong
regulation of slow anion channels and abscisic acid signaling in guard
cells by phosphorylation and dephosphorylation events. Proceedings
of the National Academy of Sciences, USA 92, 9535–9539.
Schroeder J, Hagiwara S. 1989. Cytosolic calcium regulates ion
channels in the plasma membrane of Vicia faba guard cells. Nature
338, 427–430.
Schroeder JI, Raschke K, Neher E. 1987. Voltage dependence of
K+ channels in guard cell protoplasts. Proceedings of the National
Academy of Sciences, USA 84, 4108–4112.
Schweighofer A, Hirt H, Meskienne I. 2004. Plant PP2C phospha-
tases: emerging functions in stress signaling. Trends in Plant Science
9, 236–243.
Sheen J. 1998. Mutational analysis of protein phosphatase 2C
involved in abscisic acid signal transduction in higher plants. Proceed-
ings of the National Academy of Sciences, USA 95, 975–980.
Shen Y-Y, Wang X-F, Wu F-Q, et al. 2006. The Mg2+-chelatase H
subunit is an abscisic acid receptor. Nature 443, 823–826.
Shimazaki K. 1989. Ribulosebisphosphate carboxylase activity and
photosynthetic O2 evolution rate in Vicia guard cell protoplasts. Plant
Physiology 91, 459–463.
The guard cell as a single-cell model | 1461 by guest on Septem
ber 12, 2016http://jxb.oxfordjournals.org/
Dow
nloaded from
Shimazaki K-i, Doi M, Assmann SM, Kinoshita T. 2007. Light
regulation of stomatal movement. Annual Review of Plant Biology 58,
219–247.
Shimazaki K-i, Gotow K, Sakaki T, Kondo N. 1983. High
respiratory activity of guard cell protoplasts from Vicia faba L. Plant
and Cell Physiology 23, 871–879.
Shin R, Alvarez S, Burch AY, Jez JM, Schachtman DP. 2007.
Phosphoproteomic identification of targets of the Arabidopsis sucrose
nonfermenting-like kinase SnRK2.8 reveals a connection to metabolic
processes. Proceedings of the National Academy of Sciences, USA
104, 6460–6465.
Simpson GG, Dean C. 2002. Arabidopsis, the Rosetta stone of
flowering time? Science 296, 793–795.
Simpson GG, Dijkwel PP, Quesada V, Henderson I, Dean C.
2003. FY is an RNA 3# end-processing factor that interacts with FCA
to control the Arabidopsis floral transition. Cell 113, 777–787.
Sokolovski S, Hill A, Gay R, Garcia-Mata C, Lamattina L,
Blatt MR. 2005. Protein phosphorylation is a prerequisite for in-
tracellular Ca2+ release and ion channel control by nitric oxide and
abscisic acid in guard cells. The Plant Journal 43, 520–529.
Stadler R, Buttner M, Ache P, Hedrich R, Ivashikina N,
Melzer M, Shearson SM, Smith SM, Sauer N. 2003. Diurnal and
light-regulated expression of AtSTP1 in guard cells of Arabidopsis.
Plant Physiology 133, 528–537.
Staxen I, Pical C, Montgomery LT, Gray JE, Hetherington AM,
McAinsh MR. 1999. Abscisic acid induces oscillations in guard-cell
cytosolic free calcium that involve phosphoinositide-specific phospho-
lipase C. Proceedings of the National Academy of Sciences, USA 96,
1779–1784.
Steber CM, Cooney SE, McCourt P. 1998. Isolation of the GA-
response mutant sly1 as a suppressor of abi1-1 in Arabidopsis
thaliana. Genetics 149, 509–521.
Suh SJ, Wang YF, Frelet A, Leonhardt N, Klein M, Forestier C,
Mueller-Roeber B, Cho MH, Martinoia E, Schroeder JI. 2007.
The ATP binding cassette transporter AtMRP5 modulates anion and
calcium channel activities in Arabidopsis guard cells. Journal of
Biological Chemistry 282, 1916–1924.
Sutter JU, Campanoni P, Tyrrell M, Blatt MR. 2006. Selective
mobility and sensitivity to SNAREs is exhibited by the Arabidopsis
KAT1 K+ channel at the plasma membrane. The Plant Cell 18,
935–954.
Sutter JU, Sieben C, Hartel A, Eisenach C, Thiel G, Blatt MR.
2007. Abscisic acid triggers the endocytosis of the Arabidopsis KAT1
K+ channel and its recycling to the plasma membrane. Current Biology
17, 1396–1402.
Svennelid F, Olsson A, Piotrowski M, Rosenquist M, Ottmann C,
Larsson C, Oecking C, Sommarin M. 1999. Phosphorylation of
Thr-948 at the C terminus of the plasma membrane H+-ATPase
creates a binding site for the regulatory 14-3-3 protein. The Plant Cell
11, 2379–2391.
Takemiya A, Kinoshita T, Asanuma M, Shimazaki K-i. 2006.
Protein phosphatase 1 positively regulates stomatal opening in re-
sponse to blue light in Vicia faba. Proceedings of the National
Academy of Sciences, USA 103, 13549–13554.
Tallman G, Zeiger E. 1988. Light quality and osmoregulation in Vicia
guard cells: evidence for involvement of three metabolic pathways.
Plant and Cell Physiology 88, 887–895.
Tang XD, Hoshi T. 1999. Rundown of the hyperpolarization-
activated KAT1 channel involves slowing of the opening
transitions regulated by phosphorylation. Biophysical Journal 76,
3089–3098.
Thiel G, MacRobbie EAC, Blatt MR. 1992. Membrane transport in
stomatal guard cells: the importance of voltage control. Journal of
Membrane Biology 126, 1–18.
Timmons LD. 2007. ABC transporters and RNAi in Caenorhabditis
elegans. Journal of Bioenergetics and Biomembrane 39, 459–463.
Ueno K, Kinoshita T, Inoue S-i, Emi T, Shimazaki K-i. 2005.
Biochemical characterization of plasma membrane H+-ATPase activa-
tion in guard cell protoplasts of Arabidopsis thaliana in response to
blue light. Plant and Cell Physiology 46, 955–963.
Vahisalu T, Kollist H, Wang Y-F, et al. 2008. SLAC1 is required for
plant guard cells S-type anion channel function in stomatal signalling.
Nature 452, 487–491.
Vartanian N, Marcotte L, Giraudat J. 1994. Drought rhizogenesis in
Arabidopsis thaliana. Differential responses of hormone mutants. Plant
Physiology 104, 761–767.
Vavasseur A, Raghavendra AS. 2004. Guard cell metabolism and
CO2 sensing. New Phytologist 165, 665–682.
Very A-A, Sentenac H. 2003. Molecular mechanisms and regulation
of K+ transport in higher plants. Annual Review of Plant Biology 54,
575–603.
Vlad F, Turk BE, Peynot P, Leung J, Merlot S. 2008. A versatile
strategy to define phosphorylation preferences of plant protein
kinases and screen for putative substrates. The Plant Journal 55,
104–117.
Votsmeier C, Gallwitz D. 2001. An acidic sequence of a putative
yeast Golgi membrane binds COPII and facilitates ER export. EMBO
Journal 20, 6742–6750.
Wang P, Song C-P. 2008. Guard-cell signalling for hydrogen
peroxide and abscisic acid. New Phytologist 178, 703–718.
Wang Y, Ying J, Kfzma M, et al. 2005. Molecular tailoring of
farnesylation for plant drought tolerance and yield protection.
The Plant Journal 43, 413–424.
Wasilewska A, Vlad F, Sirichandra C, Redko Y, Jammes F,
Valon C, Frei dit Frey N, Leung J. 2008. An update on abscisic
acid signaling in plants and more. Molecular Plant 1, 198–217.
Wilkinson S, Davis WJ. 2002. ABA-based chemical signalling: the
co-ordination of responses to stress in plants. Plant, Cell & Environ-
ment 25, 195–210.
Wille A, Lucas W. 1984. Ultrastructural and histochemical studies of
guard cells. Planta 160, 129–142.
Wu W-H, Assmann SM. 1994. A membrane-delimited pathway of G-
protein regulation of the guard-cell inward K+ channel. Proceedings of
the National Academy of Sciences, USA 91, 6310–6314.
Wu Y, Kuzma J, Marechal E, Graeff R, Lee HC, Foster R,
Chua N-H. 1997. Abscisic acid signaling through cyclic ADP-ribose
in plants. Science 279, 2126–2130.
1462 | Sirichandra et al. by guest on Septem
ber 12, 2016http://jxb.oxfordjournals.org/
Dow
nloaded from
Xie X, Wang Y, Williamson L, et al. 2006. The identification of
genes involved in the stomatal response to reduced atmospheric
relative humidity. Current Biology 16, 882–887.
Yoshida R, Hobo T, Ichimura K, Mizuguchi T, Takahashi F,
Alonso J, Ecker JR, Shinozaki K. 2002. ABA-activated SnRK2
protein kinase is required for dehydration stress signaling in Arabidop-
sis. Plant and Cell Physiology 43, 1473–1483.
Yoshida R, Umezawa T, Mizoguchi T, Takahashi S,
Takahashi F, Shinozaki K. 2006. The regulatory domain of
SRK2E/OST1/SnRK2.6 interacts with ABI1 and integrates
abscisic acid (ABA) and osmotic stress signals controlling
stomatal closure in Arabidopsis. Journal of Biological Chemistry
281, 5310–5318.
Zhang D-P, Wu Z-Y, Li X-Y, Zhao Z-X. 2002. Purification and
identification of a 42-kilodalton abscisic acid-specific-binding protein
from epidermis of broad bean leaves. Plant Physiology 128, 714–725.
Zhang X, Takemiya A, Kinoshita T, Shimazaki K-i. 2007. Nitric oxide
inhibits blue light-specific stomatal opening via abscisic acid signaling
pathways in Vicia guard cells. Plant and Cell Physiology 48, 715–723.
Zhang X, Wang H, Takemiya A, Song C-P, Kinoshita T,
Shimazaki K-i. 2004. Inhibition of blue light-dependent H+ pumping
by abscisic acid through hydrogen peroxide-induced dephosphoryla-
tion of the plasma membrane H+-ATPase in guard cell protoplasts.
Plant Physiology 136, 4150–4158.
Zimmermann MH, Brown CL. 1971. Trees – structure and function.
New York, NY: Springer.
The guard cell as a single-cell model | 1463 by guest on Septem
ber 12, 2016http://jxb.oxfordjournals.org/
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