A Signaling Pathway Linking Nitric Oxide Production to Heterotrimeric G Protein and Hydrogen Peroxide Regulates Extracellular Calmodulin Induction of Stomatal Closure in Arabidopsis

Extracellular calmodulin (ExtCaM) regulates stomatal movement by eliciting a cascade of intracellular signaling events including heterotrimeric G protein, hydrogen peroxide (H₂O₂), and Ca²⁺. However, the ExtCaM-mediated guard cell signaling pathway remains poorly understood. In this report, we show that Arabidopsis (Arabidopsis thaliana) NITRIC OXIDE ASSOCIATED1 (AtNOA1)-dependent nitric oxide (NO) accumulation plays a crucial role in ExtCaM-induced stomatal closure. ExtCaM triggered a significant increase in NO levels associated with stomatal closure in the wild type, but both effects were abolished in the Atnoa1 mutant. Furthermore, we found that ExtCaM-mediated NO generation is regulated by GPA1, the Gα-subunit of heterotrimeric G protein. The ExtCaM-dependent NO accumulation was nullified in gpa1 knockout mutants but enhanced by overexpression of a constitutively active form of GPA1 (cGα). In addition, cGα Atnoa1 and gpa1-2 Atnoa1 double mutants exhibited a similar response as did Atnoa1. The defect in gpa1 was rescued by overexpression of AtNOA1. Finally, we demonstrated that G protein activation of NO production depends on H₂O₂. Reduced H₂O₂ levels in guard cells blocked the stomatal response of cGα lines, whereas exogenously applied H₂O₂ rescued the defect in ExtCaM-mediated stomatal closure in gpa1 mutants. Moreover, the atrbohD/F mutant, which lacks the NADPH oxidase activity in guard cells, had impaired NO generation in response to ExtCaM, and H₂O₂-induced stomatal closure and NO accumulation were greatly impaired in Atnoa1. These findings have established a signaling pathway leading to ExtCaM-induced stomatal closure, which involves GPA1-dependent activation of H₂O₂ production and subsequent AtNOA1-dependent NO accumulation.Plant guard cells control opening and closure of the stomata in response to phytohormones (e.g. abscisic acid [ABA]) and various environmental signals such as light and temperature, thereby regulating gas exchange for photosynthesis and water status via transpiration (Schroeder et al., 2001). Cytosolic calcium ([Ca²⁺]_i) has been shown to be a key second messenger that changes in response to multiple stimuli in guard cells (McAinsh et al., 1995; Grabov and Blatt, 1998; Wood et al., 2000). A large proportion of Ca²⁺ is localized in extracellular space. It has been shown that external Ca²⁺ concentration ([Ca²⁺]_o) promotes stomatal closure and induces oscillation in [Ca²⁺]_i in guard cells (MacRobbie, 1992; McAinsh et al., 1995; Allen et al., 2001). However, how the guard cells perceive [Ca²⁺]_o concentration and convert [Ca²⁺]_o changes into [Ca²⁺]_i changes was not understood until a calcium-sensing receptor (CAS) in the plasma membrane of guard cells in Arabidopsis (Arabidopsis thaliana) was identified (Han et al., 2003). The external Ca²⁺ (Ca²⁺_o)-induced [Ca²⁺]_i increase is abolished in CAS antisense lines (Han et al., 2003). Both [Ca²⁺]_o and [Ca²⁺]_i show diurnal oscillation that is determined by stomatal conductance, whereas the amplitude of [Ca²⁺]_i oscillation is reduced in CAS antisense lines (Tang et al., 2007). The reduced amplitude of [Ca²⁺]_i diurnal oscillation in response to Ca²⁺_o treatment suggests the potential existence of other [Ca²⁺]_o sensor(s) that may transmit [Ca²⁺]_o information into the [Ca²⁺]_i response in coordination with CAS. Extracellular calmodulin (ExtCaM) could be such an additional [Ca²⁺]_o sensor.Calmodulin is a well-known Ca²⁺ sensor that is activated upon binding of Ca²⁺. It has been shown that calmodulin exists not only intracellularly but also extracellularly in many plant species (Biro et al., 1984; Sun et al., 1994, 1995; Cui et al., 2005). ExtCaM has been implicated in several important biological functions, such as the promotion of cell proliferation, pollen germination, and tube growth (Sun et al., 1994, 1995; Ma and Sun, 1997; Ma et al., 1999; Cui et al., 2005; Shang et al., 2005). ExtCaM is found in the cell wall of guard cells in Vicia faba and in the epidermis of Arabidopsis by immunogold labeling/electron microscopy and western-blot analyses, respectively, and the endogenous CaM in the extracellular space has been shown to regulate stomatal movements (Chen et al., 2003; Xiao et al., 2004). Under natural conditions, once the activity of ExtCaM has been inhibited by its membrane-impermeable antagonist W7-agrose or CaM antibody, stomatal opening under light is enhanced and stomatal closure in darkness is inhibited in V. faba and Arabidopsis (Chen et al., 2003; Xiao et al., 2004). [Ca²⁺]_i and cytosolic hydrogen peroxide (H₂O₂) changes, two events involved in ExtCaM-regulated stomatal movement (Chen et al., 2004), are likely regulated by light/darkness (Chen and Gallie, 2004; Tang et al., 2007), suggesting that ExtCaM plays an important physiological role in the regulation of stomatal diurnal rhythm. Calmodulin-binding proteins have been found in the protoplast of suspension-cultured Arabidopsis cells, supporting the idea that ExtCaM functions as a peptide-signaling molecule (Cui et al., 2005). Furthermore, ExtCaM triggers [Ca²⁺]_i elevation in guard cells of V. faba and Arabidopsis and in lily (Lilium daviddi) pollen (Chen et al., 2004; Xiao et al., 2004; Shang et al., 2005). These observations support the notion that ExtCaM could be a potential [Ca²⁺]_o sensor for external calcium, and this external calcium sensing could subsequently regulate the [Ca²⁺]_i level through a signaling cascade.It is interesting that ExtCaM and ABA induce some parallel changes in second messengers in guard cell signaling. Our previous studies show that ExtCaM induces [Ca²⁺]_i increase and H₂O₂ generation through the Gα-subunit (GPA1) of a heterotrimeric G protein, and increased H₂O₂ further elevates [Ca²⁺]_i (Chen et al., 2004). G protein, Ca²⁺, and H₂O₂ are well-known second messengers in ABA-induced guard cell signaling (McAinsh et al., 1995; Grabov and Blatt, 1998; Pei et al., 2000; Wang et al., 2001; Zhang et al., 2001; Liu et al., 2007). However, the signaling cascade triggered by ExtCaM in guard cells is poorly understood. New ABA signaling components in guard cells could provide a clue in the study of the molecular mechanism of ExtCaM guard cell signaling.Recently, nitric oxide (NO) has been shown to serve as an important signal molecule involved in many aspects of developmental processes, including floral transition, root growth, root gravitropism, adventitious root formation, xylogenesis, seed germination, and orientation of pollen tube growth (Beligni and Lamattina, 2000; Pagnussat et al., 2002; He et al., 2004; Prado et al., 2004; Gabaldón et al., 2005; Stohr and Stremlau, 2006). Increasing evidence points to a role for NO as an essential component in ABA signaling in guard cells (Garcia-Mata and Lamattina, 2001, 2002; Neill et al., 2002). It has been shown that nitrate reductase (NR) reduces nitrite to NO, and the nia1, nia2 NR-deficient mutant in Arabidopsis showed reduced ABA induction of stomatal closure (Desikan et al., 2002; Bright et al., 2006). Although animal nitric oxide synthase (NOS) activity has been detected in plants and inhibitors of mammalian NOS impair NO production in plants (Barroso et al., 1999; Corpas et al., 2001), the gene(s) encoding NOS in plants is still not clear. AtNOS1 in Arabidopsis was initially reported to encode a protein containing NOS activity (Guo et al., 2003). However, recent studies have raised critical questions regarding the nature of AtNOS1 and suggested that AtNOS1 appears not to encode a NOS (Crawford et al., 2006; Zemojtel et al., 2006). However, the originally described Atnos1 mutant is deficient in NO accumulation (Crawford et al., 2006). Consequently, AtNOS1 was renamed AtNOA1 (for NITRIC OXIDE ASSOCIATED1; Crawford et al., 2006). Therefore, the Atnoa1 mutant provides a useful tool for dissecting the function of NO in plants. At present, the molecules that regulate NO generation in ABA-mediated guard cell signaling are not clear. Evidence suggests that H₂O₂, a second messenger important for the regulation of many developmental processes and stomatal movement (Pei et al., 2000; Zhang et al., 2001; Coelho et al., 2002; Demidchik et al., 2003; Kwak et al., 2003), regulates NO generation in guard cells (Lum et al., 2002; He et al., 2005; Bright et al., 2006).Given the parallel signaling events induced by ABA and ExtCaM, we investigated whether NO is involved in the regulation of ExtCaM-induced stomatal closure in Arabidopsis and whether it is linked to G protein and H₂O₂, two key regulators of both ExtCaM and ABA regulation of stomatal movements. Using Arabidopsis mutants (e.g. GPA1 null mutants, the NO-producing mutant Atnoa1, and the guard cell H₂O₂ synthetic enzymatic mutant atrbohD/F) combined with pharmacological analysis, we present compelling evidence to establish a linear functional relationship between Gα, H₂O₂, and NO in ExtCaM guard cell signaling.     

Evolution of Conifer Diterpene Synthases: Diterpene Resin Acid Biosynthesis in Lodgepole Pine and Jack Pine Involves Monofunctional and Bifunctional Diterpene Synthases

Abscisic acid (ABA) induces stomatal closure and inhibits light-induced stomatal opening. The mechanisms in these two processes are not necessarily the same. It has been postulated that the ABA receptors involved in opening inhibition are different from those involved in closure induction. Here, we provide evidence that four recently identified ABA receptors (PYRABACTIN RESISTANCE1 [PYR1], PYRABACTIN RESISTANCE-LIKE1 [PYL1], PYL2, and PYL4) are not sufficient for opening inhibition in Arabidopsis (Arabidopsis thaliana). ABA-induced stomatal closure was impaired in the pyr1/pyl1/pyl2/pyl4 quadruple ABA receptor mutant. ABA inhibition of the opening of the mutant’s stomata remained intact. ABA did not induce either the production of reactive oxygen species and nitric oxide or the alkalization of the cytosol in the quadruple mutant, in accordance with the closure phenotype. Whole cell patch-clamp analysis of inward-rectifying K⁺ current in guard cells showed a partial inhibition by ABA, indicating that the ABA sensitivity of the mutant was not fully impaired. ABA substantially inhibited blue light-induced phosphorylation of H⁺-ATPase in guard cells in both the mutant and the wild type. On the other hand, in a knockout mutant of the SNF1-related protein kinase, srk2e, stomatal opening and closure, reactive oxygen species and nitric oxide production, cytosolic alkalization, inward-rectifying K⁺ current inactivation, and H⁺-ATPase phosphorylation were not sensitive to ABA.The phytohormone abscisic acid (ABA), which is synthesized in response to abiotic stresses, plays a key role in the drought hardiness of plants. Reducing transpirational water loss through stomatal pores is a major ABA response (Schroeder et al., 2001). ABA promotes the closure of open stomata and inhibits the opening of closed stomata. These effects are not simply the reverse of one another (Allen et al., 1999; Wang et al., 2001; Mishra et al., 2006).A class of receptors of ABA was identified (Ma et al., 2009; Park et al., 2009; Santiago et al., 2009; Nishimura et al., 2010). The sensitivity of stomata to ABA was strongly decreased in quadruple and sextuple mutants of the ABA receptor genes PYRABACTIN RESISTANCE/PYRABACTIN RESISTANCE-LIKE/REGULATORY COMPONENT OF ABSCISIC ACID RECEPTOR (PYR/PYL/RCAR; Nishimura et al., 2010; Gonzalez-Guzman et al., 2012). The PYR/PYL/RCAR receptors are involved in the early ABA signaling events, in which a sequence of interactions of the receptors with PROTEIN PHOSPHATASE 2Cs (PP2Cs) and subfamily 2 SNF1-RELATED PROTEIN KINASES (SnRK2s) leads to the activation of downstream ABA signaling targets in guard cells (Cutler et al., 2010; Kim et al., 2010; Weiner et al., 2010). Studies of Commelina communis and Vicia faba suggested that the ABA receptors involved in stomatal opening are not the same as the ABA receptors involved in stomatal closure (Allan et al., 1994; Anderson et al., 1994; Assmann, 1994; Schwartz et al., 1994). The roles of PYR/PYL/RCAR in either stomatal opening or closure remained to be elucidated.Blue light induces stomatal opening through the activation of plasma membrane H⁺-ATPase in guard cells that generates an inside-negative electrochemical gradient across the plasma membrane and drives K⁺ uptake through voltage-dependent inward-rectifying K⁺ channels (Assmann et al., 1985; Shimazaki et al., 1986; Blatt, 1987; Schroeder et al., 1987; Thiel et al., 1992). Phosphorylation of the penultimate Thr of the plasma membrane H⁺-ATPase is a prerequisite for blue light-induced activation of the H⁺-ATPase (Kinoshita and Shimazaki, 1999, 2002). ABA inhibits H⁺-ATPase activity through dephosphorylation of the penultimate Thr in the C terminus of the H⁺-ATPase in guard cells, resulting in prevention of the opening (Goh et al., 1996; Zhang et al., 2004; Hayashi et al., 2011). Inward-rectifying K⁺ currents (I_Kin) of guard cells are negatively regulated by ABA in addition to through the decline of the H⁺ pump-driven membrane potential difference (Schroeder and Hagiwara, 1989; Blatt, 1990; McAinsh et al., 1990; Schwartz et al., 1994; Grabov and Blatt, 1999; Saito et al., 2008). This down-regulation of ion transporters by ABA is essential for the inhibition of stomatal opening.A series of second messengers has been shown to mediate ABA-induced stomatal closure. Reactive oxygen species (ROS) produced by NADPH oxidases play a crucial role in ABA signaling in guard cells (Pei et al., 2000; Zhang et al., 2001; Kwak et al., 2003; Sirichandra et al., 2009; Jannat et al., 2011). Nitric oxide (NO) is an essential signaling component in ABA-induced stomatal closure (Desikan et al., 2002; Guo et al., 2003; Garcia-Mata and Lamattina, 2007; Neill et al., 2008). Alkalization of cytosolic pH in guard cells is postulated to mediate ABA-induced stomatal closure in Arabidopsis (Arabidopsis thaliana) and Pisum sativum and Paphiopedilum species (Irving et al., 1992; Gehring et al., 1997; Grabov and Blatt, 1997; Suhita et al., 2004; Gonugunta et al., 2008). These second messengers transduce environmental signals to ion channels and ion transporters that create the driving force for stomatal movements (Ward et al., 1995; MacRobbie, 1998; Garcia-Mata et al., 2003).In this study, we examined the mobilization of second messengers, the inactivation of I_Kin, and the suppression of H⁺-ATPase phosphorylation evoked by ABA in Arabidopsis mutants to clarify the downstream signaling events of ABA signaling in guard cells. The mutants included a quadruple mutant of PYR/PYL/RCARs, pyr1/pyl1/pyl2/pyl4, and a mutant of a SnRK2 kinase, srk2e.     

Loss of Halophytism by Interference with SOS1 Expression

The contribution of SOS1 (for Salt Overly Sensitive 1), encoding a sodium/proton antiporter, to plant salinity tolerance was analyzed in wild-type and RNA interference (RNAi) lines of the halophytic Arabidopsis (Arabidopsis thaliana)-relative Thellungiella salsuginea. Under all conditions, SOS1 mRNA abundance was higher in Thellungiella than in Arabidopsis. Ectopic expression of the Thellungiella homolog ThSOS1 suppressed the salt-sensitive phenotype of a Saccharomyces cerevisiae strain lacking sodium ion (Na⁺) efflux transporters and increased salt tolerance of wild-type Arabidopsis. thsos1-RNAi lines of Thellungiella were highly salt sensitive. A representative line, thsos1-4, showed faster Na⁺ accumulation, more severe water loss in shoots under salt stress, and slower removal of Na⁺ from the root after removal of stress compared with the wild type. thsos1-4 showed drastically higher sodium-specific fluorescence visualized by CoroNa-Green, a sodium-specific fluorophore, than the wild type, inhibition of endocytosis in root tip cells, and cell death in the adjacent elongation zone. After prolonged stress, Na⁺ accumulated inside the pericycle in thsos1-4, while sodium was confined in vacuoles of epidermis and cortex cells in the wild type. RNAi-based interference of SOS1 caused cell death in the root elongation zone, accompanied by fragmentation of vacuoles, inhibition of endocytosis, and apoplastic sodium influx into the stele and hence the shoot. Reduction in SOS1 expression changed Thellungiella that normally can grow in seawater-strength sodium chloride solutions into a plant as sensitive to Na⁺ as Arabidopsis.Accompanying the production and accumulation of osmolytes and other protective molecules, an important aspect of plant responses leading to salt stress tolerance is the regulation of uptake, reexport, and control over the distribution of sodium ions (Na⁺; Hasegawa et al., 2000; Tester and Davenport, 2003). Na⁺ appear to enter the root by several pathways (Essah et al., 2003; Pardo et al., 2006), although the nature of participating genes and their interaction in pathways require further investigation. Once Na⁺ has entered the root endodermis, a tissue that represents a barrier to ions (Peng et al., 2004), it is generally assumed that the ion enters the xylem following the movement of water to aerial parts of the plant. Despite substantial efflux of Na⁺ across the plasma membrane of root cells, the net flux of Na⁺ is unidirectional from soil to roots and then to the shoot, except for possible recirculation via the phloem (Tester and Davenport, 2003). In a range of species, the severity of damaging symptoms is positively correlated with the content of Na⁺ reaching photosynthetic tissues (Davenport et al., 2005; Ren et al., 2005; Munns et al., 2006). However, halophytic species can accumulate very high amounts of Na⁺ in vacuoles, such that Na⁺ may account for most of the total cellular osmotic potential (Tester and Davenport, 2003), and the presence of Na⁺ accelerates growth in euhalophytes to some degree (Adams et al., 1998). Emerging as the major advantage of halophytes appears to be their exceptional control over Na⁺ influx combined with export mechanisms, the ability to coordinate its distribution to various tissues, and efficient sequestration of Na⁺ into vacuoles. These characteristics are of particular advantage when plants are subjected to a sudden increase of Na⁺ salts in their environment (Hasegawa et al., 2000), whereas gradual increases in Na⁺ may be tolerated even by plants that are not halophytic in nature.Na⁺-ATPases, major Na⁺ export systems in organisms such as fungi and the moss Physcomitrella patens, have not been found in higher plants (Lunde et al., 2007). In Arabidopsis (Arabidopsis thaliana), transporters of monovalent (alkali) cations, such as HKT1 (Berthomieu et al., 2003; Rus et al., 2004), members of the NHX family (Yamaguchi et al., 2005; Pardo et al., 2006), and SOS1 (for Salt Overly Sensitive 1; Shi et al., 2000, 2002, 2003), have been shown to play roles in the movement and distribution of Na⁺ ions. Studies have shown the involvement of nonselective ion channels with roles in the transport of Na⁺ ions, but the genes encoding such function(s) have not been identified (Demidchik and Maathuis, 2007). SOS1, whose deletion resulted in a strong salt-sensitivity phenotype in Arabidopsis, encodes a plasma membrane Na⁺/H⁺ antiporter involved in removing Na⁺ ions from cells (Shi et al., 2000). This efflux strategy, which may be sufficient for the survival of unicellular organisms, must be accompanied by other means of Na⁺ confinement to avoid carryover of Na⁺ between cells in futile cycles. Hence, the physiological role of a plasma membrane Na⁺/H⁺ antiporter must be embedded in the context of tissue, organ, and whole plant distribution of ions and their transporters. A recent discovery on cell layer-specific differential responses to the salt stress of root cells supported this notion (Dinneny et al., 2008).In Arabidopsis, the SOS1 gene is most strongly expressed in the epidermis of the root tip region and in cells adjacent to vascular tissues (Shi et al., 2002). Based on the salt concentration in shoot, root, and xylem sap of wild-type Arabidopsis and its sos1 knockout mutants, the SOS1 antiporter is assumed to function in Na⁺ export under severe salt stress conditions (Shi et al., 2002). However, detailed knowledge about how a Na⁺ excluder achieves salt tolerance in a multicellular eukaryote is still missing. Significantly also, even though SOS1 has been an intensely studied component of the ion homeostasis mechanism, its involvement in the exceptional salt tolerance of halophytes is not known.Thellungiella salsuginea (salt cress), which had before been called T. halophila by us, is a close relative of Arabidopsis, which has become a model to study the genetic basis of this plant''s extreme tolerance to a variety of abiotic stress factors, including salinity (Inan et al., 2004; Gong et al., 2005; Vera-Estrella et al., 2005; Volkov and Amtmann, 2006; Amtmann, 2009). Thellungiella lacks specialized morphological structures, such as salt glands or large sodium storage cells found in other halophytes, making it a useful model for studying stress tolerance mechanisms that could be applicable to further understanding or to embark on engineering of conventional crops (Inan et al., 2004). Recently, it has been reported that Thellungiella had lower net Na⁺ uptake compared with Arabidopsis. The unidirectional influx of Na⁺ ions to roots appeared to be more restricted and/or tightly controlled in Thellungiella than in Arabidopsis. To compensate for greater influx, Arabidopsis roots showed higher Na⁺ efflux (Wang et al., 2006).Here, we wished to explore the role(s) by which ThSOS1, the SOS1 homolog in Thellungiella, could be involved in shaping the halophytic character of the species using ectopic expression of the gene in yeast and in Arabidopsis and Thellungiella SOS1-RNA interference (RNAi) lines. The results identified ThSOS1 as a genetic element whose activity limits Na⁺ accumulation and affects the distribution of Na⁺ ions at high concentration, thus acting as a major tolerance determinant.     

The Gene sml0013 of Synechocystis Species Strain PCC 6803 Encodes for a Novel Subunit of the NAD(P)H Oxidoreductase or Complex I That Is Ubiquitously Distributed among Cyanobacteria

The NAD(P)H oxidoreductase or complex I (NDH1) complex participates in many processes such as respiration, cyclic electron flow, and inorganic carbon concentration in the cyanobacterial cell. Despite immense progress in our understanding of the structure-function relation of the cyanobacterial NDH1 complex, the subunits catalyzing NAD(P)H docking and oxidation are still missing. The gene sml0013 of Synechocystis 6803 encodes for a small protein of unknown function for which homologs exist in all completely known cyanobacterial genomes. The protein exhibits weak similarities to the NDH-dependent flow6 (NDF6) protein, which was reported from Arabidopsis (Arabidopsis thaliana) chloroplasts as a NDH subunit. An sml0013 inactivation mutant of Synechocystis 6803 was generated and characterized. It showed only weak differences regarding growth and pigmentation in various culture conditions; most remarkably, it exhibited a glucose-sensitive phenotype in the light. The genome-wide expression pattern of the Δsml0013::Km mutant was almost identical to the wild type when grown under high CO₂ conditions as well as after shifts to low CO₂ conditions. However, measurements of the photosystem I redox kinetic in cells of the Δsml0013::Km mutant revealed differences, such as a decreased capability of cyclic electron flow as well as electron flow into respiration in comparison with the wild type. These results suggest that the Sml0013 protein (named NdhP) represents a novel subunit of the cyanobacterial NDH1 complex, mediating its coupling either to the respiratory or the photosynthetic electron flow.Cyanobacteria are the only photolithoautotrophic prokaryotes performing oxygenic photosynthesis. As in plant chloroplasts, the light reactions are situated on an internal membrane system, the thylakoids. Linear electron flow starts at PSII connected to the water-splitting center and transfers electrons via the cytochrome b₆f (Cytb₆f) complex and PSI to NADP⁺. Additionally, cyanobacteria are able to perform cyclic electron flow around PSI, producing only ATP. These light reactions allow cyanobacteria to obtain the necessary energy and reductants at varying levels in the light. In the dark, cyanobacteria also perform a respiratory electron transport to fulfill energy demands at the expense of stored carbohydrates, usually glycogen. As in heterotrophic bacteria, electrons from NAD(P)H+H⁺ are fed into the respiratory chain via the NAD(P)H oxidoreductase or complex I (NDH1). However, the cyanobacterial respiratory and photosynthetic electron transport chains are linked (i.e. both use several electron carriers together, such as the Cytb₆f complex and mobile electron carriers). The lumenal electron carriers cytochrome c (Cytc) and plastocyanin donate electrons not only to PSI but also to the respiratory terminal cytochrome oxidase (Cytox), usually of the aa3 type, where oxygen is reduced back to water. The proton gradient generated via respiratory or photosynthetic electron transport is used by the ATPase to generate ATP (Bryant, 1994).It has been shown that distinct, strain-dependent differences exist depending on which respiratory and photosynthetic electron flow routes are interconnected or more separated. In strains such as our model, Synechocystis sp. PCC 6803 (hereafter Synechocystis 6803), the complete respiratory chain is localized on thylakoids, whereas in cyanobacteria such as Synechococcus elongatus PCC 7942, the respiratory chain is more separated on the cytoplasmic membrane from the thylakoid-localized photosynthetic chain (Peschek et al., 1994). To acclimate toward different environmental conditions, the cyanobacterial electron transfer network shows a relatively high degree of flexibility not only in its activity but also in its composition. For example, the preference for plastocyanin under copper-replete conditions switches to Cytc under copper-deplete conditions, while iron limitation results in a switch from the iron-containing ferredoxin to flavodoxin (Hagemann et al., 1999). The cyclic electron flow around PSI can use different routes, mainly via NDH1 but also directly to Cytb₆f (Yeremenko et al., 2005). Finally, respiratory electron transport also can be connected to three different terminal oxidases depending on strain or growth conditions (Pils and Schmetterer, 2001).Particularly high functional as well as structural diversity was shown for the cyanobacterial NDH1 complex (Zhang et al., 2004). As in other bacteria, it is involved in respiration, transferring electrons from carbohydrate catabolism into the plastoquinone (PQ) pool (Haimovich-Dayan et al., 2011). However, NDH1 also is involved in the cyclic electron flow around PSI (Yeremenko et al., 2005; Bernát et al., 2011). These two NDH1 functions are conserved in the chloroplastidial NDH complex that is phylogenetically derived from the cyanobacterial one (Ifuku et al., 2011). Moreover, it also has been established that NDH1 is essential for the CO₂ conversion into HCO₃⁻ as part of the cyanobacterial inorganic carbon-concentrating mechanism (Ogawa, 1991; Shibata et al., 2001). This functional diversity is reflected in a structural diversity thought to serve these different purposes. For example, many of the smaller NDH1 subunits are encoded by multigene families (e.g. ndhF or ndhD), which are differentially expressed under changing conditions such as high or low CO₂. The expression changes result in the generation of differently sized NDH1 complexes with different subunit composition, which can preferentially function in respiratory electron transport and cyclic electron transfer around PSI (called NDH1L) or in the conversion of CO₂ into HCO₃⁻ (called NDH1MS; Zhang et al., 2004). Despite intensive investigations on the cyanobacterial as well as the chloroplastidial NDH1 complexes, the subunits for NAD(P)H oxidation are still unknown, making the functioning of these complexes enigmatic (for review, see Battchikova et al., 2011a). Recent isolations of functional NDH complexes from Thermosynechococcus elongatus indicated that reduced ferredoxin could possibly directly transfer electrons via ferredoxin-NADP⁺ oxidoreductase to NDH1 (Hu et al., 2013).Accordingly, genome searches or proteomic analyses of isolated NDH1 complexes have often been used to gain more insights into the function of the NDH1 complex. A new NDH subunit was found in chloroplasts, named NDH-dependent flow6 (NDF6; Ishikawa et al., 2008). A protein called NdhP displaying weak similarities to NDF6 was recently copurified with active NDH1 complexes from the cyanobacterium T. elongatus (Nowaczyk et al., 2011). Here, we report on the generation and characterization of the mutant Δsml0013::Km, in which the NDF6 homolog Sml0013 of Synechocystis 6803 was inactivated.     

Photosystem II and Pigment Dynamics among Ecotypes of the Green Alga Ostreococcus

We investigated the photophysiological responses of three ecotypes of the picophytoplankter Ostreococcus and a larger prasinophyte Pyramimonas obovata to a sudden increase in light irradiance. The deepwater Ostreococcus sp. RCC809 showed very high susceptibility to primary photoinactivation, likely a consequence of high oxidative stress, which may relate to the recently noted plastid terminal oxidase activity in this strain. The three Ostreococcus ecotypes were all capable of deploying modulation of the photosystem II repair cycle in order to cope with the light increase, but the effective clearance of photoinactivated D1 protein appeared to be slower in the deepwater Ostreococcus sp. RCC809, suggesting that this step is rate limiting in the photosystem II repair cycle in this strain. Moreover, the deepwater Ostreococcus accumulated lutein and showed substantial use of the xanthophyll cycle under light stress, demonstrating its high sensitivity to light fluctuations. The sustained component of the nonphotochemical quenching of fluorescence correlated well with the xanthophyll deepoxidation activity. Comparisons with the larger prasinophyte P. obovata suggest that the photophysiology of Ostreococcus ecotypes requires high photosystem II repair rates to counter a high susceptibility to photoinactivation, consistent with low pigment package effects in their minute-sized cells.The prasinophytes are marine planktonic green algae with a phylogenetic position branching near the base of the green lineage (Baldauf, 2003; Turmel et al., 2009). They are widespread in temperate (Diez et al., 2001; Zhu et al., 2005) and polar (Lovejoy et al., 2007) marine habitats, in which they are often significant contributors to primary production (Not et al., 2004). The prasinophytes include the smallest known eukaryotic photoautotroph, Ostreococcus tauri (Courties et al., 1994; Chrétiennot-Dinet et al., 1995), whose particularly simple structure makes it an attractive model minimal chlorophyte, and indeed, minimal eukaryote (Derelle et al., 2006). Recently, genomic sequences for three Ostreococcus strains, isolated from different ecological niches, have become available (Derelle et al., 2006; Palenik et al., 2007), thus increasing the interest of these models for understanding acclimation processes in this deep-branching group of chlorophytes.Photoacclimation strategies differ in two Ostreococcus strains (Cardol et al., 2008; Six et al., 2008), which, although belonging to different phylogenetic clades, are nonetheless morphologically indistinguishable (Rodríguez et al., 2005). O. tauri, a eutrophilic lagoon species, modulates PSII content to enable acclimation and growth over a wide range of irradiances. In marked contrast, Ostreococcus sp. (O. sp.) RCC809, isolated at 105 m depth in the tropical Atlantic Ocean, modulates the size of its large PSII antenna in a strategy that accommodates a narrower range of light levels but that incurs lower nutrient costs compared with photoacclimation in O. tauri (Six et al., 2008). The evidence for different light acclimation strategies between these two Ostreococcus ecotypes raises the question of the underlying physiological processes for niche adaptation in these closely related organisms. Cardol et al. (2008) recently analyzed the coastal O. tauri and the deepwater O. sp. RCC809 grown under low to moderate light and found exciting evidence for a plastid terminal oxidase electron flow path in O. sp. RCC809 from PSII back to oxygen, short-circuiting the usual Z scheme in a mechanism to generate a transthylakoidal pH gradient without net generation of reductant. Like all oxygenic photoautotrophs, the prasinophytes suffer photoinactivation of PSII (Aro et al., 1993; Tyystjarvi, 2008; Guskov et al., 2009) at a rate approximately proportional to the incident irradiance (Nagy et al., 1995; Hakala et al., 2005). To counter this photoinactivation, a PSII repair cycle proteolytically removes the photoinactivated D1 protein (Silva et al., 2003) and replaces it through de novo synthesis and reassembly with the remaining subunits (Aro et al., 1993). If photoinactivation outruns the rate of repair, the PSII pool suffers net photoinhibition (Aro et al., 2005; Nishiyama et al., 2005, 2006; Murata et al., 2007), leading to a decrease in photosynthetic capacity and potentially to a decrease in growth. To limit photoinhibition, photosynthetic cells use physiological processes that dissipate excess light energy into heat, thereby preempting the generation of toxic reactive oxygen species (Baroli et al., 2004; Holt et al., 2004) that can inhibit metabolism, notably including the PSII repair processes (Nishiyama et al., 2006; Murata et al., 2007). These excitation dissipation mechanisms manifest as a drop in PSII fluorescence yield termed nonphotochemical quenching of fluorescence (NPQ). In land plants and characterized chlorophytes, NPQ is notably associated with changes in light-harvesting complex conformation along with pigmentation changes (Demmig-Adams and Adams, 1992; Baroli et al., 2004; Holt et al., 2004; Li et al., 2004).The specialization of Ostreococcus ecotypes to contrasting environments suggests that they may have evolved distinct capacities to cope with rapid fluctuations in light. Here, we investigate this question by subjecting three different Ostreococcus ecotypes to short-term increases in light irradiance to uncover their capacities for PSII repair and susceptibilities to photoinactivation. We use a target theory approach (Nagy et al., 1995; Sinclair et al., 1996) to parameterize their susceptibility to primary photoinactivation in a form useful for predicting and modeling responses to changes in irradiance. We moreover compare the Ostreococcus strains to a much larger prasinophyte derived from temperate surface waters, Pyramimonas obovata, to explore how cell size can influence photophysiology in the prasinophytes.     

Focus Issue on Calcium Signaling: Calcium-Dependent Protein Kinase CPK6 Positively Functions in Induction by Yeast Elicitor of Stomatal Closure and Inhibition by Yeast Elicitor of Light-Induced Stomatal Opening in Arabidopsis

Yeast elicitor (YEL) induces stomatal closure that is mediated by a Ca²⁺-dependent signaling pathway. A Ca²⁺-dependent protein kinase, CPK6, positively regulates activation of ion channels in abscisic acid and methyl jasmonate signaling, leading to stomatal closure in Arabidopsis (Arabidopsis thaliana). YEL also inhibits light-induced stomatal opening. However, it remains unknown whether CPK6 is involved in induction by YEL of stomatal closure or in inhibition by YEL of light-induced stomatal opening. In this study, we investigated the roles of CPK6 in induction by YEL of stomatal closure and inhibition by YEL of light-induced stomatal opening in Arabidopsis. Disruption of CPK6 gene impaired induction by YEL of stomatal closure and inhibition by YEL of light-induced stomatal opening. Activation by YEL of nonselective Ca²⁺-permeable cation channels was impaired in cpk6-2 guard cells, and transient elevations elicited by YEL in cytosolic-free Ca²⁺ concentration were suppressed in cpk6-2 and cpk6-1 guard cells. YEL activated slow anion channels in wild-type guard cells but not in cpk6-2 or cpk6-1 and inhibited inward-rectifying K⁺ channels in wild-type guard cells but not in cpk6-2 or cpk6-1. The cpk6-2 and cpk6-1 mutations inhibited YEL-induced hydrogen peroxide accumulation in guard cells and apoplast of rosette leaves but did not affect YEL-induced hydrogen peroxide production in the apoplast of rosette leaves. These results suggest that CPK6 positively functions in induction by YEL of stomatal closure and inhibition by YEL of light-induced stomatal opening in Arabidopsis and is a convergent point of signaling pathways for stomatal closure in response to abiotic and biotic stress.Stomata, formed by pairs of guard cells, play a critical role in regulation of plant CO₂ uptake and water loss, thus critically influencing plant growth and water stress responsiveness. Guard cells respond to a variety of abiotic and biotic stimuli, such as light, drought, and pathogen attack (Israelsson et al., 2006; Shimazaki et al., 2007; Melotto et al., 2008).Elicitors derived from microbial surface mimic pathogen attack and induce stomatal closure in various plant species such as Solanum lycopersicum (Lee et al., 1999), Commelina communis (Lee et al., 1999), Hordeum vulgare (Koers et al., 2011), and Arabidopsis (Arabidopsis thaliana; Melotto et al., 2006; Khokon et al., 2010). Yeast elicitor (YEL) induces stomatal closure in Arabidopsis (Klüsener et al., 2002; Khokon et al., 2010; Salam et al., 2013). Our recent studies showed that YEL inhibits light-induced stomatal opening and that protein phosphorylation is involved in induction by YEL of stomatal closure and inhibition by YEL of light-induced stomatal opening (Salam et al., 2013).Cytosolic Ca²⁺ has long been recognized as a conserved second messenger in stomatal movement (Shimazaki et al., 2007; Roelfsema and Hedrich 2010; Hubbard et al., 2012). Elevation of cytosolic free Ca²⁺ concentration ([Ca2+]_cyt) is triggered by influx of Ca²⁺ from apoplast and release of Ca²⁺ from intracellular stores in guard cell signaling (Leckie et al., 1998; Hamilton et al., 2000; Pei et al., 2000; Garcia-Mata et al., 2003; Lemtiri-Chlieh et al., 2003). The influx of Ca²⁺ is carried by nonselective Ca²⁺-permeable cation (I_Ca) channels that are activated by plasma membrane hyperpolarization and H₂O₂ (Pei et al., 2000; Murata et al., 2001; Kwak et al., 2003). Elevation of [Ca2+]_cyt activates slow anion (S-type) channels and down-regulates inward-rectifying potassium (K_in) channels in guard cells (Schroeder and Hagiwara, 1989; Grabov and Blatt, 1999). The activation of S-type channels is a hallmark of stomatal closure, and the suppression of K_in channels is favorable to stomatal closure but not to stomatal opening (Pei et al., 1997; Kwak et al., 2001; Xue et al., 2011; Uraji et al., 2012).YEL induces stomatal closure with extracellular H₂O₂ production, intracellular H₂O₂ accumulation, activation of I_Ca channels, and transient [Ca2+]_cyt elevations (Klüsener et al., 2002; Khokon et al., 2010). However, it remains to be clarified whether YEL activates S-type channels and inhibits K_in channels in guard cells.Calcium-dependent protein kinases (CDPKs) are regulators in Ca²⁺-dependent guard cell signaling (Mori et al., 2006; Zhu et al., 2007; Geiger et al., 2010, 2011; Zou et al., 2010; Munemasa et al., 2011; Brandt et al., 2012; Scherzer et al., 2012). In guard cells, CDPKs regulate activation of S-type and I_Ca channels and inhibition of K_in channels (Mori et al., 2006; Zou et al., 2010; Munemasa et al., 2011). A CDPK, CPK6, positively regulates activation of S-type channels and I_Ca channels without affecting H₂O₂ production in abscisic acid (ABA)- and methyl jasmonate (MeJA)-induced stomatal closure (Mori et al., 2006; Munemasa et al., 2011). CPK6 phosphorylates and activates SLOW ANION CHANNEL-ASSOCIATED1 expressed in Xenopus spp. oocyte (Brandt et al., 2012; Scherzer et al., 2012). These findings underline the role of CPK6 in regulation of ion channel activation and stomatal movement, leading us to test whether CPK6 regulates the induction by YEL of stomatal closure and inhibition by YEL of light-induced stomatal opening.In this study, we investigated activation of S-type channels and inhibition of K_in channels by YEL and roles of CPK6 in induction by YEL of stomatal closure and inhibition by YEL of light-induced stomatal opening. For this purpose, we examined the effects of mutation of CPK6 on induction by YEL of stomatal closure and inhibition by YEL of light-induced stomatal opening, activation of I_Ca channels, transient [Ca2+]_cyt elevations, activation of S-type channels, inhibition of K_in channels, H₂O₂ production in leaves, and H₂O₂ accumulation in leaves and guard cells.     

Arabidopsis RTE1 is essential to ethylene receptor ETR1 amino-terminal signaling independent of CTR1

The Arabidopsis (Arabidopsis thaliana) ethylene receptor Ethylene Response1 (ETR1) can mediate the receptor signal output via its carboxyl terminus interacting with the amino (N) terminus of Constitutive Triple Response1 (CTR1) or via its N terminus (etr1^1-349 or the dominant ethylene-insensitive etr1-1^1-349) by an unknown mechanism. Given that CTR1 is essential to ethylene receptor signaling and that overexpression of Reversion To Ethylene Sensitivity1 (RTE1) promotes ETR1 N-terminal signaling, we evaluated the roles of CTR1 and RTE1 in ETR1 N-terminal signaling. The mutant phenotype of ctr1-1 and ctr1-2 was suppressed in part by the transgenes etr1^1-349 and etr1-1^1-349, with etr1-1^1-349 conferring ethylene insensitivity. Coexpression of 35S:RTE1 and etr1^1-349 conferred ethylene insensitivity in ctr1-1, whereas suppression of the ctr1-1 phenotype by etr1^1-349 was prevented by rte1-2. Thus, RTE1 was essential to ETR1 N-terminal signaling independent of the CTR1 pathway. An excess amount of the CTR1 N terminus CTR1^7-560 prevented ethylene receptor signaling, and the CTR1^7-560 overexpressor CTR1-Nox showed a constitutive ethylene response phenotype. Expression of the ETR1 N terminus suppressed the CTR1-Nox phenotype. etr1^1-349 restored the ethylene insensitivity conferred by dominant receptor mutant alleles in the ctr1-1 background. Therefore, ETR1 N-terminal signaling was not mediated by full-length ethylene receptors; rather, full-length ethylene receptors acted cooperatively with the ETR1 N terminus to mediate the receptor signal independent of CTR1. ETR1 N-terminal signaling may involve RTE1, receptor cooperation, and negative regulation by the ETR1 carboxyl terminus.The gaseous plant hormone ethylene is perceived by a small family of ethylene receptors. Arabidopsis (Arabidopsis thaliana) has five ethylene receptors that are structurally similar to prokaryotic two-component histidine kinase (HK) proteins. Mutants defective in multiple ethylene receptor genes show a constitutive ethylene response phenotype, which indicates a negative regulation of ethylene responses by the receptor genes (Hua and Meyerowitz, 1998).The receptor N terminus has three or four transmembrane domains that bind ethylene. The GAF (for cGMP-specific phosphodiesterases, adenylyl cyclases, and FhlA) domain, which follows the transmembrane helices, mediates noncovalent receptor heterodimerization and may have a role in receptor cooperation (Gamble et al., 2002; O’Malley et al., 2005; Xie et al., 2006; Gao et al., 2008). The subfamily I receptors Ethylene Response1 (ETR1) and Ethylene Response Sensor1 (ERS1) have a conserved HK domain following the GAF domain. For subfamily II members ETR2, Ethylene Insensitive4 (EIN4), and ERS2, the HK domain is less conserved, and they lack most signature motifs essential for HK activity (Chang et al., 1993; Gamble et al., 1998; Hua et al., 1998; Qu and Schaller, 2004; Xie et al., 2006). Among the five receptors, ETR1, ETR2, and EIN4 have a receiver domain following the HK domain. The ETR1 HK domain may have a role in mediating the receptor signal to downstream components, and the HK activity facilitates the ethylene signaling (Clark et al., 1998; Huang et al., 2003; Hall et al., 2012). The receiver domain can dimerize and could involve receptor cooperation (Müller-Dieckmann et al., 1999). However, differential receptor cooperation occurs between the receiver domain-lacking ERS1 and the other ethylene receptors, which does not support the hypothesis that the domains involve receptor cooperation (Liu and Wen, 2012).Acting downstream of the ethylene receptors is Constitutive Triple Response1 (CTR1), a MEK kinase (mitogen-activated protein kinase kinase kinase) with Ser/Thr kinase activity, and the kinase domain locates at the C terminus. The CTR1 N terminus does not share sequence similarity to known domains and can physically interact with the ethylene-receptor HK domain (Clark et al., 1998; Huang et al., 2003). ctr1 mutants showing attenuated CTR1 kinase activity or the ETR1-CTR1 association exhibit various degrees of the constitutive ethylene-response phenotype. For example, the ctr1-1 and ctr1^btk mutations result from the D694E and E626K substitutions, respectively, in the CTR1 kinase domain, and ctr1-1 shows a stronger ethylene-response phenotype than ctr1^btk, with ctr1-1 having much weaker kinase activity than ctr1^btk (Kieber et al., 1993; Huang et al., 2003; Ikeda et al., 2009). The ctr1-8 mutation results in the G354E substitution that prevents the ETR1-CTR1 association, and the mutant exhibits a constitutive ethylene-response phenotype. Overexpression of the CTR1 N terminus CTR1^7-560, which is responsible for interaction with ethylene receptors, leads to constitutive ethylene responses, possibly by titrating out available ethylene receptors (Kieber et al., 1993; Huang et al., 2003). These studies suggest that CTR1 kinase activity and the interaction of CTR1 with the receptor HK domain may be important to the ethylene receptor signal output in suppressing constitutive ethylene responses.Although the ETR1-CTR1 interaction via the HK domain is essential to the ethylene receptor signal output, evidence suggests that the ETR1 receptor signal output can also be independent of the HK activity or domain. The etr1 ers1 loss-of-function mutant displays extreme growth defects. The etr1[HGG] mutation inactivates ETR1 HK activity, and expression of the getr1[HGG] transgene rescues the etr1 ers1 growth defects, which indicates a lack of association of ETR1 receptor signaling and its kinase activity (Wang et al., 2003). The dominant etr1-1 mutation results in the C65Y substitution and confers ethylene insensitivity (Chang et al., 1993), and the expression of the HK domain-lacking etr1^1-349 and ethylene-insensitive etr1-1^1-349 isoforms partially suppresses the growth defects of etr1 ers1-2. Loss-of-function mutations of subfamily II members do not affect etr1-1^1-349 functions. Therefore, etr1-1^1-349 predominantly cooperates with subfamily I receptors to mediate the ethylene receptor signal output (Xie et al., 2006). Biochemical and transformation studies showing that ethylene receptors can form heterodimers and that each receptor is a component of high-molecular-mass complexes explain how ethylene receptors may act cooperatively (Gao et al., 2008; Gao and Schaller, 2009; Chen et al., 2010).Reversion To Ethylene Sensitivity1 (RTE1), a Golgi/endoplasmic reticulum protein, was isolated from a suppressor screen of the dominant ethylene-insensitive etr1-2 mutation. The cross-species complementation of the rte1-2 loss-of-function mutation by the rice (Oryza sativa) RTE Homolog1 (OsRTH1) suggests a conserved mechanism that modulates the ethylene receptor signaling across higher plant species (Zhang et al., 2012). RTE1 and OsRTH1 overexpression led to ethylene insensitivity in wild-type Arabidopsis but not the etr1-7 loss-of-function mutant, and expression of etr1^1-349 restored ethylene insensitivity with RTE1 overexpression in etr1-7 (Resnick et al., 2006; Zhou et al., 2007; Zhang et al., 2010). Coimmunoprecipitation of epitope-tagged ETR1 and RTE1 and Trp fluorescence spectroscopy revealed the physical interaction of RTE1 and ETR1 (Zhou et al., 2007; Dong et al., 2008, 2010). Therefore, RTE1 may directly promote ETR1 receptor signal output through the ETR1 N terminus, but whether RTE1 has an essential role in ETR1 N-terminal signaling remains to be addressed.Currently, the biochemical nature of the ethylene receptor signal is unknown, and the underlying mechanisms of mediation of the ethylene receptor signal output remain uninvestigated. Genetic and biochemical studies suggest that activation of CTR1 by ethylene receptors may suppress constitutive ethylene responses; upon ethylene binding, the receptors are converted to an inactive state and fail to activate CTR1, and the suppression of ethylene responses by CTR1 is alleviated (Hua and Meyerowitz, 1998; Klee, 2004; Wang et al., 2006; Hall et al., 2007). However, this model does not address how the ETR1 N terminus, which does not have the CTR1-interacting site, mediates the receptor signal to suppress constitutive ethylene responses. The receptor signal of the truncated etr1 isoforms may be mediated by other full-length ethylene receptors and then activate CTR1; alternatively, the ETR1 N-terminal signal may be mediated by a pathway independent of CTR1 (Gamble et al., 2002; Qu and Schaller, 2004; Xie et al., 2006). Results showing that mutants defective in multiple ethylene receptor genes exhibit a more severe ethylene-response phenotype than ctr1 and that ctr1 mutants are responsive to ethylene support the presence of a CTR1-independent pathway (Hua and Meyerowitz, 1998; Cancel and Larsen, 2002; Huang et al., 2003; Liu et al., 2010).In this study, we investigated whether mediation of ETR1 N-terminal signaling is independent of CTR1 and whether RTE1 is essential to the CTR1-independent ETR1 N-terminal signaling. The ETR1 N-terminal signaling was not mediated via other full-length ethylene receptors, but the signal of full-length ethylene receptors could be mediated by the ETR1 N terminus independent of CTR1. The ETR1 C terminus may inhibit ETR1 N-terminal signaling, whereby deletion of the C terminus facilitates N-terminal signaling. We propose a model for the possible modulation of ETR1 receptor signaling.     

The Rubisco Small Subunit Is Involved in Tobamovirus Movement and Tm-22-Mediated Extreme Resistance

The multifunctional movement protein (MP) of Tomato mosaic tobamovirus (ToMV) is involved in viral cell-to-cell movement, symptom development, and resistance gene recognition. However, it remains to be elucidated how ToMV MP plays such diverse roles in plants. Here, we show that ToMV MP interacts with the Rubisco small subunit (RbCS) of Nicotiana benthamiana in vitro and in vivo. In susceptible N. benthamiana plants, silencing of NbRbCS enabled ToMV to induce necrosis in inoculated leaves, thus enhancing virus local infectivity. However, the development of systemic viral symptoms was delayed. In transgenic N. benthamiana plants harboring Tobacco mosaic virus resistance-2² (Tm-2²), which mediates extreme resistance to ToMV, silencing of NbRbCS compromised Tm-2²-dependent resistance. ToMV was able to establish efficient local infection but was not able to move systemically. These findings suggest that NbRbCS plays a vital role in tobamovirus movement and plant antiviral defenses.Plant viruses use at least one movement protein (MP) to facilitate viral spread between plant cells via plasmodesmata (PD; Lucas and Gilbertson, 1994; Ghoshroy et al., 1997). Among viral MPs, the MP of tobamoviruses, such as Tobacco mosaic virus (TMV) and its close relative Tomato mosaic virus (ToMV), is the best characterized. TMV MP specifically accumulates in PD and modifies the plasmodesmatal size exclusion limit in mature source leaves or tissues (Wolf et al., 1989; Deom et al., 1990; Ding et al., 1992). TMV MP and viral genomic RNA form a mobile ribonucleoprotein complex that is essential for cell-to-cell movement of viral infection (Watanabe et al., 1984; Deom et al., 1987; Citovsky et al., 1990, 1992; Kiselyova et al., 2001; Kawakami et al., 2004; Waigmann et al., 2007). TMV MP also enhances intercellular RNA silencing (Vogler et al., 2008) and affects viral symptom development, host range, and host susceptibility to virus (Dardick et al., 2000; Bazzini et al., 2007). Furthermore, ToMV MP is identified as an avirulence factor that is recognized by tomato (Solanum lycopersicum) resistance proteins Tobacco mosaic virus resistance-2 (Tm-2) and Tm-2² (Meshi et al., 1989; Lanfermeijer et al., 2004). Indeed, tomato Tm-2² confers extreme resistance against TMV and ToMV in tomato plants and even in heterologous tobacco (Nicotiana tabacum) plants (Lanfermeijer et al., 2003, 2004).To date, several host factors that interact with TMV MP have been identified. These TMV MP-binding host factors include cell wall-associated proteins such as pectin methylesterase (Chen et al., 2000), calreticulin (Meshi et al., 1989), ANK1 (Ueki et al., 2010), and the cellular DnaJ-like protein MPIP1 (Shimizu et al., 2009). Many cytoskeletal components such as actin filaments (McLean et al., 1995), microtubules (Heinlein et al., 1995), and the microtubule-associated proteins MPB2C (Kragler et al., 2003) and EB1a (Brandner et al., 2008) also interact with TMV MP. Most of these factors are involved in TMV cell-to-cell movement.Rubisco catalyzes the first step of CO₂ assimilation in photosynthesis and photorespiration. The Rubisco holoenzyme is a heteropolymer consisting of eight large subunits (RbCLs) and eight small subunits (RbCSs). RbCL was reported to interact with the coat protein of Potato virus Y (Feki et al., 2005). Both RbCS and RbCL were reported to interact with the P3 proteins encoded by several potyviruses, including Shallot yellow stripe virus, Onion yellow dwarf virus, Soybean mosaic virus, and Turnip mosaic virus (Lin et al., 2011). Proteomic analysis of the plant-virus interactome revealed that RbCS participates in the formation of virus complexes of Rice yellow mottle virus (Brizard et al., 2006). However, the biological function of Rubisco in viral infection remains unknown.In this study, we show that RbCS plays an essential role in virus movement, host susceptibility, and Tm-2²-mediated extreme resistance in the ToMV-host plant interaction.     

Medicago truncatula Natural Resistance-Associated Macrophage Protein1 Is Required for Iron Uptake by Rhizobia-Infected Nodule Cells

Iron is critical for symbiotic nitrogen fixation (SNF) as a key component of multiple ferroproteins involved in this biological process. In the model legume Medicago truncatula, iron is delivered by the vasculature to the infection/maturation zone (zone II) of the nodule, where it is released to the apoplast. From there, plasma membrane iron transporters move it into rhizobia-containing cells, where iron is used as the cofactor of multiple plant and rhizobial proteins (e.g. plant leghemoglobin and bacterial nitrogenase). MtNramp1 (Medtr3g088460) is the M. truncatula Natural Resistance-Associated Macrophage Protein family member, with the highest expression levels in roots and nodules. Immunolocalization studies indicate that MtNramp1 is mainly targeted to the plasma membrane. A loss-of-function nramp1 mutant exhibited reduced growth compared with the wild type under symbiotic conditions, but not when fertilized with mineral nitrogen. Nitrogenase activity was low in the mutant, whereas exogenous iron and expression of wild-type MtNramp1 in mutant nodules increased nitrogen fixation to normal levels. These data are consistent with a model in which MtNramp1 is the main transporter responsible for apoplastic iron uptake by rhizobia-infected cells in zone II.SNF is carried out by the endosymbiosis between legumes and diazotrophic bacteria called rhizobia (van Rhijn and Vanderleyden, 1995). Detection of rhizobial nodulation (Nod) factors by the legume plant results in curling of a root hair around the rhizobia and development of an infection thread that will deliver the rhizobia to the developing root nodule primordium, which is also triggered by Nod factors (Kondorosi et al., 1984; Brewin, 1991; Oldroyd, 2013). Rhizobia are eventually released into the cytoplasm of host plant cells via endocytosis, resulting in an organelle-like structure known as the symbiosome, which consists of bacteria surrounded by a plant membrane called the symbiosome membrane (SM; Roth and Stacey, 1989; Vasse et al., 1990). Rhizobia within symbiosomes eventually differentiate into nitrogen-fixing bacteroids that produce and export ammonium to the plant for assimilation (Vasse et al., 1990).Two main developmental programs for nodulation have been described (Sprent, 2007). In the determinate type, e.g. in soybean (Glycine max), the nodule meristem is active only transiently, which gives rise to a spherical nodule. In the indeterminate nodules, e.g. in alfalfa (Medicago sativa) and pea (Pisum sativum), the meristem(s) remain active for much longer, resulting in cylindrical and/or branched nodules of indeterminate morphology. Indeterminate nodules can be divided in spatiotemporal zones that facilitate the study of the nodulation process. At least four zones are observed in a mature indeterminate nodule (Vasse et al., 1990). Zone I is the meristematic region that drives nodule growth. In zone II, rhizobia are released from the infection thread and differentiate into bacteroids. Zone III is the site of nitrogen fixation. Finally, Zone IV is the senescence zone, where bacteroids are degraded and nutrients are recycled. Some authors describe two more zones: the interzone, a transition zone between zones II and III (Vasse et al., 1990; Roux et al., 2014), and zone V, where saprophytic rhizobia live on the nutrients released by senescent cells (Timmers et al., 2000).Nodulation and nitrogen fixation are tightly regulated processes (for review, see Oldroyd, 2013; Udvardi and Poole, 2013; Downie, 2014) and require a relatively large supply of nutrients from the host: photosynthates, macronutrients such as phosphate and sulfate, amino acids, at least prior to nitrogen fixation, and metal micronutrients (Udvardi and Poole, 2013). Among the latter, iron is one of the most critical (Brear et al., 2013; González-Guerrero et al., 2014). The activity of some of the most abundant and important enzymes in SNF directly depends on iron as cofactor. Nitrogenase, the enzyme directly responsible for nitrogen fixation, needs iron-sulfur clusters and an iron-molybdenum cofactor to reduce N₂ (Miller et al., 1993). The hemoprotein leghemoglobin, which controls O₂ levels in the nodule (Ott et al., 2005), represents around 20% of total nodule protein (Appleby, 1984). Similarly, different types of superoxide dismutase, including an Fe-superoxide dismutase, control the free radicals produced during SNF (Rubio et al., 2007). Other ferroproteins are involved in energy transduction and recycling related to the nitrogen fixation process (Ruiz-Argüeso et al., 1979; Preisig et al., 1996).Despite its importance, iron is a growth-limiting nutrient for plants in most soils (Grotz and Guerinot, 2006), especially in alkaline soils. As a result, iron deficiency is prevalent in plants and hampers crop production and human health (Grotz and Guerinot, 2006; Mayer et al., 2008). This is even more so when legumes are nodulated (Terry et al., 1991; Tang et al., 1992). The relatively high iron demand of nodules can trigger the iron deficiency response, i.e. increase in iron reductase activities in the root epidermis and acidification of the surrounding soil (Terry et al., 1991; Andaluz et al., 2009). Consequently, knowing how iron homeostasis is maintained in nodulated legumes, including how this micronutrient is delivered to the nodule, is important for understanding and improving SNF.Taking advantage of state-of-the-art metal visualization methods, the pathway for iron delivery to the nodule has been elucidated (Rodríguez-Haas et al., 2013). Synchrotron-based x-ray fluorescence studies on Medicago truncatula indeterminate nodules indicate that most of the iron is delivered by the vasculature to the apoplast of zone II. In zone III, iron is mostly localized within bacteroids. Therefore, a number of transporters must exist that move iron through the plasma membrane of plant cells and the SM of infected cells. Several transporters have been hypothesized to mediate iron transport through the SM. Soybean Divalent Metal Transporter1 (GmDMT1) is a nodule-induced Natural Resistance-Associated Macrophage Protein (Nramp) that was found in the soybean SM using specific antibodies (Kaiser et al., 2003). However, biochemical studies on Nramp transporters suggest that they transport substrates into the cytosol (Nevo and Nelson, 2006), rather than outwards or into symbiosomes. More recently, the study of stationary endosymbiont nodule1 (sen1) mutants in Lotus japonicus indicated that SEN1, a yeast (Saccharomyces cerevisiae) Cross Complements CSG1/Arabidopsis (Arabidopsis thaliana) Vacuolar Iron Transporter1 homolog, could play a role in delivering iron across the SM (Hakoyama et al., 2012), albeit this is merely based on the mutant plant phenotype and the role of members of this family in other organisms.Very little is known about the molecular identity of transporters that mediate iron uptake from the nodule apoplast. Based on known plant metal transporters and their biochemistry, the most likely candidates are members of the Nramp and Zinc-Regulated Transporter1, Iron-Regulated Transporter1-Like Protein (ZIP) families, because these can transport divalent metals into the cytosol (Vert et al., 2002; Nevo and Nelson, 2006). Moreover, given that the expression of at least one Nramp transporter (GmDMT1) is activated by nodulation (Kaiser et al., 2003), it is possible that members of this family might mediate iron uptake into rhizobia-containing cells. Nramp transporters are ubiquitous divalent transition metal importers (Nevo and Nelson, 2006). Phenotypical and electrophysiological studies indicate that they have a wide range of possible biological (Fe²⁺, Mn²⁺, Zn²⁺, Cu²⁺, Co²⁺, and Ni²⁺) and nonbiological (Pb²⁺ and Cd²⁺) substrates (Belouchi et al., 1997; Curie et al., 2000; Thomine et al., 2000; Mizuno et al., 2005; Rosakis and Köster, 2005; Cailliatte et al., 2009). In plants, Nramp transporters have been associated with a number of biological roles, such as Fe²⁺ and Mn²⁺ uptake from soil (Curie et al., 2000; Cailliatte et al., 2010), Mn²⁺ long-distance trafficking (Yamaji et al., 2013), metal remobilization during germination (Lanquar et al., 2005), Cd²⁺ and Ni²⁺ tolerance (Mizuno et al., 2005; Cailliatte et al., 2009), and the immune response (Segond et al., 2009), in addition to participating in SNF (Kaiser et al., 2003).In this study, M. truncatula MtNramp1 (Medtr3g088460) was identified as the Nramp transporter gene expressed at the highest levels in nodules. MtNramp1 protein was localized in the plasma membrane of nodule cells in zone II, where the expression reached its maximum. Its role in iron uptake and its importance for SNF were established using a loss-of-function mutant, nramp1-1. This work adds to our understanding of how apoplastic metals are imported into nodule cells.     

Voltage-Sensor Transitions of the Inward-Rectifying K+ Channel KAT1 Indicate a Latching Mechanism Biased by Hydration within the Voltage Sensor

The Kv-like (potassium voltage-dependent) K⁺ channels at the plasma membrane, including the inward-rectifying KAT1 K⁺ channel of Arabidopsis (Arabidopsis thaliana), are important targets for manipulating K⁺ homeostasis in plants. Gating modification, especially, has been identified as a promising means by which to engineer plants with improved characteristics in mineral and water use. Understanding plant K⁺ channel gating poses several challenges, despite many similarities to that of mammalian Kv and Shaker channel models. We have used site-directed mutagenesis to explore residues that are thought to form two electrostatic countercharge centers on either side of a conserved phenylalanine (Phe) residue within the S2 and S3 α-helices of the voltage sensor domain (VSD) of Kv channels. Consistent with molecular dynamic simulations of KAT1, we show that the voltage dependence of the channel gate is highly sensitive to manipulations affecting these residues. Mutations of the central Phe residue favored the closed KAT1 channel, whereas mutations affecting the countercharge centers favored the open channel. Modeling of the macroscopic current kinetics also highlighted a substantial difference between the two sets of mutations. We interpret these findings in the context of the effects on hydration of amino acid residues within the VSD and with an inherent bias of the VSD, when hydrated around a central Phe residue, to the closed state of the channel.Plant cells utilize the potassium ion (K⁺) to maintain hydrostatic (turgor) pressure, to drive irreversible cell expansion for growth, and to facilitate reversible changes in cell volume during stomatal movements. Potassium uptake and its circulation throughout the plant relies both on high-affinity, H⁺-coupled K⁺ transport (Quintero and Blatt, 1997; Rubio et al., 2008) and on K⁺ channels to facilitate K⁺ ion transfer across cell membranes. Uptake via K⁺ channels is thought to be responsible for roughly 50% of the total K⁺ content of the plant under most field conditions (Spalding et al., 1999; Rubio et al., 2008; Amtmann and Blatt, 2009). K⁺ channels confer on the membranes of virtually every tissue distinct K⁺ conductances and regulatory characteristics (Véry and Sentenac, 2003; Dreyer and Blatt, 2009). Their characteristics are thus of interest for engineering directed to manipulating K⁺ flux in many aspects of plant growth and cellular homeostasis. The control of K⁺ channel gating has been identified as the most promising target for the genetic engineering of stomatal responsiveness (Lawson and Blatt, 2014; Wang et al., 2014a), based on the recent development of quantitative systems models of guard cell transport and metabolism (Chen et al., 2012b; Hills et al., 2012; Wang et al., 2012). By contrast, modifying the expression and, most likely, the population of native K⁺ channels at the membrane was found to have no substantial effect on stomatal physiology (Wang et al., 2014b).The Kv-like K⁺ channels of the plant plasma membrane (Pilot et al., 2003; Dreyer and Blatt, 2009) share a number of structural features with the Kv superfamily of K⁺ channels characterized in animals and Drosophila melanogaster (Papazian et al., 1987; Pongs et al., 1988). The functional channels assemble from four homologous subunits and surround a central transmembrane pore that forms the permeation pathway (Daram et al., 1997). Each subunit comprises six transmembrane α-helices, designated S1 to S6, and both N and C termini are situated on the cytosolic side of the membrane (Uozumi et al., 1998). The pore or P loop between the S5 and S6 α-helices incorporates a short α-helical stretch and the highly conserved amino acid sequence TxGYGD, which forms a selectivity filter for K⁺ (Uozumi et al., 1995; Becker et al., 1996; Nakamura et al., 1997). The carbonyl oxygen atoms of these residues in all four K⁺ channel subunits face inward to form coordination sites for K⁺ ions between them (Doyle et al., 1998; Jiang et al., 2003; Kuo et al., 2003; Long et al., 2005) and a multiple-ion pore (Thiel and Blatt, 1991) such that K⁺ ions pass through the selectivity filter as if in free solution. The plant channels are also sensitive to a class of neurotoxins that exhibit high specificity in binding around the mouth of the channel pore (Obermeyer et al., 1994).These K⁺ channels also share a common gating mechanism. Within each subunit, the first four α-helices form a quasiindependent unit, the voltage sensor domain (VSD), with the S4 α-helix incorporating positively charged (Arg or Lys) residues regularly positioned across the lipid bilayer and transmembrane electric field. Voltage displaces the S4 α-helix within the membrane and couples rotation of the S5 and S6 α-helices lining the pore, thereby opening or closing the channel (Sigworth, 2003; Dreyer and Blatt, 2009). For outward-rectifying channels, such as the mammalian Kv1.2 and the D. melanogaster Shaker K⁺ channels, an inside-positive electric field drives the positively charged, S4 α-helix outward (the up position), which draws on the S4-S5 linker to open the pore. This simple expedient of a lever and string secures current flow in one direction by favoring opening at positive, but not negative, voltages. This same model applies to the Arabidopsis (Arabidopsis thaliana) Kv-like K⁺ channels, including outward rectifiers that exhibit sensitivity to external K⁺ concentration (Blatt, 1988; Blatt and Gradmann, 1997; Johansson et al., 2006), and it serves equally in the gating of inward-rectifying K⁺ channels such as KAT1, which gates open at negative voltages (Dreyer and Blatt, 2009).Studies of KAT1 gating (Latorre et al., 2003; Lai et al., 2005) have indicated that the S4 α-helix of the channel most likely undergoes very similar conformational changes with voltage as those of the mammalian and Shaker K⁺ channels. These findings conform with the present understanding of the evolution of VSD structure (Palovcak et al., 2014) and the view of a common functional dynamic to its molecular design. It is likely, therefore, that a similar electrostatic network occurs in KAT1 to stabilize the VSD. Crucially, however, experimental evidence in support of such a network has yet to surface. Electrostatic countercharges and the hydration of amino acid side chains between the α-helices within the VSDs of mammalian and Shaker K⁺ channel models are important for the latch-like stabilization of the so-called down and up states of these channels (Tao et al., 2010; Pless et al., 2011). Nonetheless, some studies (Gajdanowicz et al., 2009; Riedelsberger et al., 2010) have pointed to subtle differences in the structure of KAT1 that relate to the VSD.We have explored the electrostatic network of the KAT1 VSD through site-directed mutagenesis to manipulate the voltage dependence of KAT1, combining these studies with molecular dynamic simulations previously shown to accommodate the plant VSDs and their hydration during gating transitions (Gajdanowicz et al., 2009; Garcia-Mata et al., 2010). We report here that gating of KAT1 is sensitive to manipulations affecting a set of electrostatic charge transfer centers. These findings conform in large measure to the mammalian and Shaker models. However, virtually all manipulations affecting a highly conserved, central Phe favor the up state of the VSD and the closed KAT1 channel, whereas mutations affecting the electrostatic networks on either side of this Phe favor the down state of the VSD and the open channel. These and additional observations suggest that hydration within the VSD is a major determinant of KAT1 gating.