Plant gas exchange is regulated by guard cells that form stomatal pores. Stomatal adjustments are crucial for plant survival; they regulate uptake of CO2 for photosynthesis, loss of water, and entrance of air pollutants such as ozone. We mapped ozone hypersensitivity, more open stomata, and stomatal CO2-insensitivity phenotypes of the Arabidopsis thaliana accession Cvi-0 to a single amino acid substitution in MITOGEN-ACTIVATED PROTEIN (MAP) KINASE 12 (MPK12). In parallel, we showed that stomatal CO2-insensitivity phenotypes of a mutant cis (CO2-insensitive) were caused by a deletion of MPK12. Lack of MPK12 impaired bicarbonate-induced activation of S-type anion channels. We demonstrated that MPK12 interacted with the protein kinase HIGH LEAF TEMPERATURE 1 (HT1) —a central node in guard cell CO2 signaling—and that MPK12 functions as an inhibitor of HT1. These data provide a new function for plant MPKs as protein kinase inhibitors and suggest a mechanism through which guard cell CO2 signaling controls plant water management.
Human activities have increased the concentrations of CO2 and harmful air pollutants such as ozone in the troposphere. During the last 200 y, the CO2 concentration has increased from 280 to 400 ppm, and it is predicted to double relative to the preindustrial level by 2050 [1]. Elevated CO2 is likely to have complex effects on plant productivity, since CO2 is not only a driver of climate change but also the main substrate for photosynthesis. Altered atmospheric chemistry is not limited to CO2; the concentration of tropospheric ozone has more than doubled within the past 100 y [2]. Ozone is a notorious air pollutant causing severe damage to crops; present day global yield reductions caused by ozone range from 8. 5%–14% for soybean, 3. 9%–15% for wheat, and 2. 2%–5. 5% for maize [3]. Both CO2 and ozone enter the plant through stomata—small pores on the surfaces of plants that are formed by pairs of guard cells. Guard cells also regulate plant water balance since plants with more open stomata allow faster water evaporation. Water availability is the most limiting factor for agricultural production, and insufficient water supply can cause large reductions in crop yields [4]. Thus, plants are constantly facing a dilemma; assimilation of CO2 requires stomatal opening but also opens the gates for entrance of harmful air pollutants and leads to excessive water loss. A consequence of increased atmospheric CO2 concentration can be higher biomass production [5], but at the same time, plants adjust to elevated CO2 by partial closure of stomata [5,6] and expressing an altered developmental program that leads to reduced stomatal number [7]. CO2-induced stomatal closure reduces water loss; hence, it can directly modify plant water use efficiency (WUE) —carbon assimilated through photosynthesis versus water lost through stomata. Natural variation among Arabidopsis thaliana accessions provides a rich genetic resource for addressing plant function and adaptation to diverse environmental conditions. The Arabidopsis accession Cvi-0 from the Cape Verde Islands has impaired CO2 responses, more open stomata than Col-0, and is extremely sensitive to ozone treatment [8,9]. A single amino acid change in Cvi-0 MITOGEN-ACTIVATED PROTEIN KINASE 12 (MPK12) was recently shown to affect water use efficiency as well as stomatal size and to impair abscisic acid (ABA) -induced inhibition of stomatal opening [10]. MPK12 also regulates auxin signaling in roots [11]. However, the involvement of MPK12 in the CO2 signaling pathway in guard cells has not been addressed thus far. Among the important components of A. thaliana guard cell CO2 signaling are carbonic anhydrases (βCA1 and βCA4) that catalyze the conversion of CO2 to bicarbonate and the protein kinase HIGH LEAF TEMPERATURE 1 (HT1) that has been suggested to function as a negative regulator of CO2-induced stomatal movements [12,13]. Ultimately, for stomata to close, a signal from the bicarbonate has to activate protein kinases such as OPEN STOMATA 1 (OST1) that in turn activate plasma membrane anion channels, including SLOW ANION CHANNEL 1 (SLAC1), followed by extrusion of ions and water that causes stomatal closure [14–17]. Isolation of a dominant HT1 allele, ht1-8D, revealed that HT1 may directly inhibit OST1- and GUARD CELL HYDROGEN PEROXIDE-RESISTANT 1 (GHR1) -induced activation of SLAC1 [18]. Bicarbonate-induced activation of SLAC1 has been reconstituted in Xenopus laevis oocytes [19,20]. The pathway was shown to consist of RESISTANT TO HIGH CARBON DIOXIDE 1 (RHC1), HT1, OST1, and SLAC1 [19], while more recently the importance of CARBONIC ANHYDRASE 4 (βCA4), aquaporin PIP2; 1, OST1, and SLAC1 was demonstrated [20]. Although guard cells are perhaps the best characterized single cell signaling system in the plant kingdom, there are still large gaps in our understanding of how CO2 signaling in guard cells is regulated and by which mechanism CO2 might regulate plant water management and WUE [5,21,22]. Here, we present the results of quantitative trait loci (QTL) mapping and sequencing of near-isogenic lines (NILs) of Cvi-0 ozone sensitivity. In a parallel approach, we mapped more open stomata and CO2-insensitivity phenotypes of a mutant cis (CO2 insensitive). A single amino acid change (G53R) in MPK12 and complete deletion of MPK12 are the causes of more open stomata and altered CO2 responses of Cvi-0 and cis, respectively. Based on kinase activity assays, we conclude that MPK12 acts as an inhibitor of the HT1 kinase, which represents a crucial step in the regulation of plant stomatal CO2 responses.
Our initial QTL mapping of ozone sensitivity in Cvi-0 placed the two major contributing loci on the lower ends of chromosomes 2 and 3 [8]. To identify the causative loci related to the extreme ozone sensitivity and more open stomata of Cvi-0, we created a NIL termed Col-S (for Col-0 ozone sensitive) through eight generations of backcrossing of Cvi-0 with Col-0 (Fig 1A, S1A Fig, and S1 Video). In parallel, ozone tolerance from Col-0 was introgressed to Cvi-0 by six generations of backcrossing, which generated the ozone-tolerant Cvi-T (S1 Video). Using these accessions, NILs, and recombinant inbred lines (RILs), we mapped the causative ozone QTLs to a region of 90 kb on chromosome 2 and 17. 70–18. 18 Mbp on chromosome 3 (S1B Fig). We have previously shown that the QTL on chromosome 2 also controls plant water loss and stomatal function [8]. We isolated both QTLs by backcrossing Col-S with Col-0 and obtained the NILs Col-S2 and Col-S3. Both of these were less sensitive to ozone than Col-S (S1A Fig), indicating that these QTLs act additively to regulate ozone sensitivity. Col-S2 (but not Col-S3) showed much higher daytime stomatal conductance than Col-0 (Fig 1B). The mapping resolution on chromosome 3 was not sufficient to identify the causative gene. Hence, we focused on Col-S2 and its role in stomatal function. Within the 90-kb mapping region on chromosome 2, one gene, At2g46070, encoding a MAP kinase MPK12, shows strong preferential guard cell expression [23]. A single point mutation was found in Cvi-0 MPK12, leading to a glycine to arginine substitution at position 53 of the protein. CAS (calcium-sensing receptor) is a chloroplast-localized protein important for proper stomatal responses to external Ca2+ [24,25]. While testing stomatal phenotypes in cas mutants, we observed phenotypic discrepancy between different alleles of cas. Whereas the cas-2 (GABI-665G12) line had more open stomata and impaired CO2 responses, this was neither observed in cas-1 nor in cas-3 (Fig 1C and S1C Fig). Further experiments showed that the T-DNA insert in the CAS gene was not linked to the CO2-insensitive phenotype of cas-2. In a backcross with Col-0, the T-DNA insert in cas-2 was removed, thereby generating the mutant cis (CO2 insensitive). Both cis and Col-S2 had impaired responses to high CO2 (800 ppm), leading to longer half-response times, but a residual CO2 response could still be observed (Fig 1D and S1E Fig). In order to identify the causative mutation in cis, mapping and whole genome sequencing of cis × C24 population was performed, which revealed a complete deletion of the MPK12 gene and its neighbor BYPASS2 in cis (Fig 1E and S1D Fig). Thus, cis was renamed mpk12-4. A second mutant (gdsl3-1) from the GABI-Kat collection (GABI-492D11) contained an identical deletion of BYPASS2 and MPK12 (S2 Fig). We also identified a line with a T-DNA insert in exon 2 of MPK12 from the SAIL collection (Fig 1E), which was recently named mpk12-3 [26]. No full-length transcript was found in mpk12-3 (S3 Fig). SALK T-DNA insertion lines of MPK12 were previously described as lethal [11,23]; similarly, we were unable to retrieve homozygous plants of the same alleles, possibly indicating the presence of an additional T-DNA in an essential gene. The new mpk12 deletion, SAIL T-DNA insertion, and Col-S2 point mutation alleles allowed a detailed characterization of the role of MPK12 in stomatal regulation. Stomatal conductance was higher throughout the day in all three lines (Col-S2, mpk12-3, and mpk12-4) (Fig 2A), suggesting that the amino acid substitution in Cvi-0 MPK12 leads to loss of function. Furthermore, Col-0 transformed with MPK12 from Cvi-0 showed stomatal conductance similar to Col-0, which excludes the option that the G53R substitution in MPK12 would lead to gain of function (S1F Fig). Moreover, the wild-type (Col-0) stomatal phenotype was observed in heterozygous F1 plants from a cross of Col-S2 and Col-gl1, in which the gl1 mutation that gives a trichome-less phenotype was used as a noninvasive method for selecting successfully crossed plants in the first generation (S1G Fig). Increased stomatal conductance may result from an increased number of stomata, larger stomata, or more open stomata. However, the stomatal index, length, and density did not differ between the lines, indicating that MPK12 regulates a function related to the stomatal aperture (S4 Fig). Because of the higher degree of stomatal opening, the instantaneous WUE was lower in mpk12-3, mpk12-4, and Col-S2 (Fig 2B). Altered WUE was previously also seen in mpk12-1 and a NIL with Cvi-0 MPK12 in Ler [10]. Cvi-0 and Col-S2 were complemented by expression of MPK12 from Col-0 (Fig 2C and 2D). Similarly, mpk12-4 was complemented by expression of Col-0 MPK12 but not by Cvi-0 MPK12 (Fig 2E). We conclude that MPK12 is a crucial regulator of stomatal conductance, and a single amino acid substitution (G53R) in Cvi-0 leads to loss of function of MPK12. Reduction of CO2 levels inside the leaf [27] is a signal that indicates a shortage of substrate for photosynthesis and triggers stomatal opening. The rate of stomatal opening in response to low CO2 was severely impaired in mpk12 and Col-S2 (Fig 3A and S5A Fig). Another signal for stomatal opening is light; this response was intact in plants with impaired or absence of MPK12 (S5B and S5C Fig). The hormone ABA has dual roles in stomatal regulation; it induces stomatal closure but also inhibits light-induced stomatal opening. The latter response was impaired in mpk12 mutants and Col-S2 (Fig 3B and S5C Fig). Stomata close in response to several signals, including darkness, reduced air humidity, ozone pulse, elevated CO2, and ABA. Of these, only the response to elevated CO2 was impaired in mpk12 and Col-S2 (Fig 3C and 3D, S5D–S5H and S6 Figs). CO2 signaling is impaired in the carbonic anhydrase double mutant ca1 ca4 [13], and the product of carbonic anhydrase, bicarbonate, activates S-type anion currents [15]. In Col-S2 and mpk12-4, bicarbonate-induced S-type anion currents were strongly impaired (Fig 3E). Collectively, these data indicated that MPK12 has an important role in the regulation of CO2-induced stomatal movements in Arabidopsis. Only a few regulators of stomatal CO2 signaling in Arabidopsis have been identified. These include the protein kinases HT1 and OST1 [12,15,16]. To find the interaction partners of MPK12, we conducted pairwise split-ubiquitin yeast two-hybrid (Y2H) assays against several kinases and phosphatases involved in stomatal signaling (Fig 4A and 4B and S7A and S7B Fig). A strong interaction was observed between MPK12 and HT1 in yeast. The MPK12–HT1 interaction was also confirmed in Nicotiana benthamiana with bimolecular fluorescence complementation (BiFC) (Fig 4C–4E) and split luciferase complementation assays (S7C Fig). Strong interaction between MPK12 and HT1 was observed in the cell periphery (Fig 4C). Recently, HT1 was shown to be a plasma membrane–associated protein [28]. In contrast, Col-0 and Cvi-0 MPK12-YFP were located inside the cell (S8A–S8D Fig). Hence, it is likely that the interaction with HT1 brings MPK12 to the plasma membrane. HT1 interacted with both the Col-0 and Cvi-0 versions of MPK12, but the interaction with Cvi-0 MPK12 (G53R) was weaker both in quantitative BiFC and Y2H assays (Fig 4B and 4D). MPK11, an MPK from the same group as MPK12 [29], did not interact with HT1 (Fig 4C). INDOLE-3-BUTYRIC ACID RESPONSE 5 (IBR5) is a MPK phosphatase that regulates auxin signaling in roots and has been shown to interact with and regulate the activity of MPK12 [11]. We confirmed the interaction between MPK12 and IBR5 (S7A Fig). However, the ibr5-1 mutant exhibited wild-type stomatal phenotypes in response to CO2 changes (Fig 3A and 3C, and S5A and S5E Fig), suggesting that IBR5 is not required in stomatal CO2 signaling. The function of MPK12 in ABA and CO2 signaling was further explored through genetic analysis. A strong loss-of-function allele, ht1-2, that has low stomatal conductance [12] was used to evaluate the relationship between mpk12 and ht1-2. The Col-S2 ht1-2 and mpk12-4 ht1-2 double mutants had a more closed stomata phenotype similar to ht1-2 (Fig 4F), suggesting that HT1 is epistatic to MPK12. The strong impairment of stomatal function in abi1-1 (ABA insensitive1-1) was additive to Col-S2 in the double mutant Col-S2 abi1-1 (Fig 4F). Hence, signaling through MPK12 seems to act—at least to some extent—independently of the core ABA signaling pathway. Taken together, the MPK12-HT1 interaction (Fig 4A–4E) and the epistasis between ht1-2 and mpk12-4 (Fig 4F) suggest that MPK12 functions upstream of HT1 and could regulate the activity of HT1. To test this directly, we performed in vitro kinase assays with casein as the substrate for HT1 (Fig 5A). HT1 displayed strong autophosphorylation and phosphorylated casein efficiently. Addition of the Col-0 version of MPK12 and a hyperactive version (MPK12 Y122C) efficiently inhibited HT1 activity (Fig 5A and quantified in Fig 5B). A point-mutated version (MPK12 K70R) designed to remove the kinase activity of MPK12 also inhibited the autophosphorylation activity of HT1 and phosphorylation of casein by HT1, although it was less efficient than the wild-type (Fig 5B). Importantly, the Cvi-0 version of MPK12 (G53R) displayed strongly suppressed inhibition of HT1 activity (Fig 5A and 5B). MPK12 did not phosphorylate the kinase-dead version of HT1 (K113M) (Fig 5C). The kinase-dead version of HT1 (K113M) was used as a substrate, since the strong autophosphorylation activity of HT1 would otherwise have obscured the result. Wild-type MPK12 and hyperactive MPK12 (Y122C) displayed autophosphorylation, whereas MPK12 (G53R) as well as MPK12 (K70R) had lost their autophosphorylation activity, indicating that the G53R substitution in Cvi-0 MPK12 disrupts the kinase activity of the protein (Fig 5C). The inhibition of HT1 by MPK12 was specific, as MPK11, which belongs to the same group as MPK12, was not able to affect HT1 kinase activity (S9 Fig). We conclude that the stomatal phenotypes of mpk12 mutants and Cvi-0 can be explained by a lack of inhibition of HT1 activity by MPK12, which leads to more open stomata and impaired CO2 responses (Figs 2A, 3 and 5A and 5C). MPK12 belongs to the same group of MPKs as MPK4, a crucial regulator of pathogen and stress responses [29]. In tobacco, the silencing of MPK4 impaired CO2-induced stomatal closure [30]. Since Arabidopsis MPK4 and MPK12 are highly similar [31], it is possible that both MPK4 and MPK12 could regulate stomatal CO2 responses. Indeed, in an Y2H screen to identify HT1 interacting proteins, one prominent interactor was MPK4 [18]. The Arabidopsis mpk4 mutant is severely dwarfed, and measurements of accurate stomatal conductance with these plants are not feasible [32]. However, the impaired stomatal response to CO2 in mpk12-4 (Fig 3) was further enhanced by guard cell–specific silencing of MPK4 [18]; hence, in guard cells MPK4 is acting redundantly with MPK12 in stomatal CO2 signaling. Furthermore, MPK4 could also inhibit HT1 kinase activity [18]. The G53 residue in MPK12 is conserved in all Arabidopsis MPKs [10]. Since the G53R mutation blocked MPK12 function, we tested whether a similar mutation would impair MPK4 function. This experiment showed that MPK4-induced inhibition of HT1 activity was blocked by the introduction of a G55R mutation in MPK4; this mutation corresponds to G53R in Cvi-0 MPK12 (Fig 6A). Since MPK11 did not inhibit HT1 activity (S9 Fig), the function of MPKs as kinase inhibitors in Arabidopsis may be restricted to MPK12 and its closest homologue MPK4. The Arabidopsis MPK6 crystal structure [33] was used to model the structure of MPK4 and MPK12 and to address the role of the G55R and G53R mutations that were shown to be crucial for the function of these proteins (Fig 6B and 6C). The mutation of Gly to Arg in position 53 in MPK12 caused the protrusion of the arginine sidechain on the surface of the protein, which could affect its binding affinity for other proteins in addition to an altered structure of the loop region. Similarly, the Arg in position 55 of MPK4 protruded from the surface as compared to the wild-type. Thus, the MPK12 G53R and MPK4 G55R amino acid substitutions may alter protein binding affinities of these MPKs to other proteins. Collectively, the presented experiments suggest that the CO2 signal leading to stomatal movements is transmitted through MPK12 and MPK4, leading to inhibition of HT1, and this enables SLAC1 activation by its activators, including OST1 and GHR1. Neither MPK12 G53R from Cvi-0 nor MPK4 G55R can fully inhibit HT1 (Fig 7).
Natural variation within a species holds great potential to identify regulatory mechanisms that are not easily uncovered through mutant screens. The Cvi-0 accession originates from the southern border of the Arabidopsis distribution area, the Cape Verde Islands. The Ler × Cvi RIL population was one of the first RILs produced, and it has been phenotyped for multiple traits [34]. Despite this, only a few QTLs from Cvi-0 have been identified at the molecular level. Our earlier research identified a locus related to ozone sensitivity and more open stomata phenotype of Cvi-0 in chromosome 2 [8]. Recently, the G53R substitution in MPK12 that affects plant water use efficiency was identified by using the Ler × Cvi populations, but the biochemical function of MPK12 in stomatal regulation was not further investigated [10]. Here, we generated NILs by backcrossing Cvi-0 eight times to Col-0 and show that the same natural mutation in Cvi-0 and lack of MPK12 in cis are the causes of ozone sensitivity, more open stomata, and altered CO2 responses of Arabidopsis plants. Furthermore, we showed that MPK12 regulates the activity of the protein kinase HT1, a major component of the CO2 signaling pathway in guard cells. The regulators of HT1 have remained largely unknown, despite the exceptionally strong CO2-insensitivity phenotype of plants with impaired HT1 function [12,15]. Our findings provide the first evidence for the role of MPK12 in guard cell CO2 signaling and provide a mechanistic insight for the MPK12 function in the regulation of plant water management. The role of MPKs in Arabidopsis guard cell signaling has concentrated on MPK9 and MPK12, which are preferentially expressed in guard cells. Plants with point mutations in MPK9 (mpk9-1, L295F) and MPK12 (mpk12-1, T220I) had wild-type ABA responses, but mpk12-1 has decreased WUE [10]. The mpk9-1, mpk12-1, and mpk12-2 alleles are Tilling (Targeting Induced Local Lesions IN Genomes) lines in the Col-erecta background and the previously characterized MPK12-Cvi NIL is in the Ler background [10,23]. Mutations in ERECTA modify transpiration efficiency and stomatal density, which may have influenced some of the previously described mpk12-1 phenotypes [10,35]. In contrast, the full knockout alleles described here, mpk12-3 and mpk12-4, are in Col-0 and imply a major function for MPK12 in CO2 signaling. Additional roles for MPK12 in stomatal responses have been inferred through the use of the double mutant mpk9-1 mpk12-1 that has impaired stomatal closure responses to ABA and H2O2 treatment and has impaired S-type anion channel activation in response to ABA and Ca2+ [23]. It is also highly susceptible to Pseudomonas syringae infection and impaired in yeast elicitor-, chitosan-, and methyl jasmonate–induced stomatal closure [36]. Since the mpk9 mpk12 double mutant appears to be more severely impaired in abiotic and biotic stomatal responses and S-type anion channel activation than the loss of function MPK12 alleles (Fig 3), it is possible that MPK12 together with MPK9 regulates stomatal aperture in response to various signals. MPK12 also regulates auxin responses in the root [11,26]. However, beyond the observation that plants with impaired MPK12 are hypersensitive to auxin inhibition of root growth, no details about the targets of MPK12 in roots are known. HT1 was the first component shown to be specifically associated with stomatal CO2 signaling, and the ht1-2 mutant has more closed stomata displaying constitutive high CO2 response at ambient CO2 levels (Fig 4D [12]). The opposite phenotypes of mpk12 and ht1-2 allowed us to use genetic analysis to position MPK12 in the guard cell signaling network. The stomata of mpk12 ht1-2 were more closed, thus positioning MPK12 upstream of HT1 and possibly as a direct regulator of HT1 (Fig 4D). CO2 signaling in guard cells is initiated through the production of bicarbonate by carbonic anhydrases, and bicarbonate initiates signaling leading to activation of S-type anion channels [13,15]. In mpk12, the bicarbonate-dependent activation of S-type anion channels was impaired, as was previously found for the plants with impaired OST1 and SLAC1 (Fig 3E) [15]. The combined evidence from mpk12 phenotypes, genetic analysis, and measurements of S-type anion currents all pointed towards MPK12 as a crucial regulator of CO2 signaling acting through HT1. Indeed, HT1 kinase activity was inhibited in the presence of Col-0 MPK12 but not by the Cvi-0 version of MPK12 (Fig 5A). Thus, the inhibitory function of MPK12 was impaired by the G53R amino acid substitution, probably by its weaker interaction with HT1 (Figs 4 and 5A). This explains the similar phenotypes of the NIL Col-S2, mpk12-3, and mpk12-4; they all display lack of inhibition of the negative regulator HT1, leading to higher stomatal conductance. Further support for the regulatory interplay between HT1 and MPK12 is provided by the isolation of a dominant mutation in HT1, ht1-8D, which in contrast to ht1-2 has constitutively more open stomata and is biochemically resistant to inhibition by MPK12 [18]. Cvi-0 has altered phenotypes in many traits, including drought and pathogen resistance [34,37,38]. All of these traits are regulated through stomatal function; thus, the MPK12-HT1 regulatory module identified here may influence many of the previously observed phenotypes of Cvi-0. Recently, two independent studies used X. laevis oocytes as a heterologous expression system to reconstitute bicarbonate-induced activation of the SLAC1 anion channel [19,20]. Tian et al. [19] reported that a multidrug and toxic compound extrusion (MATE) -type transporter RHC1 functions as a bicarbonate-sensing component that inactivates HT1 and promotes SLAC1 activation by OST1. More recently, it was demonstrated that expression of RHC1 alone was sufficient to activate ion currents in oocytes; these currents were independent of bicarbonate, calling into question the role of RHC1 as a bicarbonate sensor [20]. Furthermore, it was shown that SLAC1 activation can be reconstituted by extracellular bicarbonate in the presence of aquaporin PIP2; 1, carbonic anhydrase CA4, and the protein kinases OST1, CPK6, and CPK23 [20]. However, in the guard cell, any proposed CO2 signaling pathway should include HT1, since plants with mutations in HT1 completely lack CO2-induced stomatal responses [12,18,28]. We showed that bicarbonate-induced S-type anion currents were strongly impaired in guard cell protoplasts, which lacked functional MPK12 (Fig 3E). Thus, MPK12, MPK4, and possibly other MPKs that are expressed in guard cells play a role in controlling the activity of HT1, and future research should identify the signaling pathway upstream of MPK12 (Fig 7). Dissection of different domains in SLAC1 revealed that the CO2 signal may involve the transmembrane region of SLAC1, whereas ABA activation of SLAC1 requires an intact N- and C-terminus [39]. Hence, ABA and CO2 regulation of SLAC1 could use different signaling pathways, and this may explain the lack of strong ABA phenotypes in plants with mutations in MPK12. We propose that stomatal movements triggered by changes in CO2 concentration are regulated by MPK12- and MPK4-induced inhibition of HT1 activity (Fig 7). The MPK12 glycine 53 is conserved in all Arabidopsis MPKs [10] and is located on the protein surface in the glycine-rich loop that coordinates the gamma-phosphate of ATP (Fig 6B and 6C). Thus, this glycine may also be important for the function of other Arabidopsis MPKs. Further studies into the mechanisms controlling activation of MPKs in guard cells will help to identify molecular switches that function in plant acclimation to environmental stress and modulate the overall plant water use efficiency. Such information may allow the designing of molecular targets that can be used for breeding crops with improved water management.
Col-0, Col-gl, Cvi-0, gdsl3-1 (GABI-492D11; CS447183), cas-1 (SALK_070416), cas-2 (GABI-665G12), and cas-3 (SAIL_1157_C10) were from the European Arabidopsis Stock Centre (www. arabidopsis. info). Seeds of ht1-2 were a gift from Dr. Koh Iba. Col-0 × Cvi-0 RILs were obtained from INRA Versailles. The abi1-1 allele used was in Col-0 accession. Double mutants and other crosses were made through standard techniques and genotyped with PCR-based markers (S1 Table). For ozone screening, seeds were sown at high density on a 1: 1 v/v mixture of vermiculite and peat (type B2, Kekkilä, Finland), and kept for 2 d at 4°C for stratification. The plants were grown in controlled growth chambers (Bio 1300, Weiss Umwelttechnik, Germany) under a 12 h photoperiod, with a 23°C/19°C day/night temperature and a 70%/90% relative humidity or in growth rooms with equivalent growth conditions. The average photosynthetic photon flux density during the light period was 200 μmol m-2 s-1. When seedlings were 1 wk old, they were transplanted into 8 × 8 cm pots at a density of five plants per pot. Three-week-old plants were exposed to ozone in growth chambers under the same conditions as they were grown until the experiments. Ozone exposure was acute (300–350 ppb for 6 h) and started 2 h after light was switched on. Ozone damage was visualized with trypan blue stain or quantified as electrolyte leakage. NILs were created by crossing Col-0 with Cvi-0 and selecting the most ozone-sensitive plant in F2 and backcrossing to Col-0 for eight generations (generating Col-S) or selecting the most tolerant plant and backcrossing to Cvi-0 for six generations (generating Cvi-T). The genomes of Cvi-0 and Cvi-T were sequenced at BGI Tech Solutions (Hong Kong) with Illumina technology, and the genomes of Col-S and Cvi-T were sequenced at the DNA Sequencing and Genomics lab of the University of Helsinki with SOLiD technology. Genome sequence data is available from the NCBI BioProject database with the accession number PRJNA345097. The 90-bp-long Illumina paired end sequencing library reads were mapped onto the Col-0 reference genome (TAIR10) with using the Bowtie2 aligner (version 2. 0. 0-beta7; [40]) in “end-to-end” alignment mode, yielding an average genomic sequence coverage of 45-fold. Variation calling and haplotype phasing was performed with the help of samtools (tools for alignments in the SAM format, Version: 0. 1. 18; [41]). Based on the aligned sequences, various PCR-based markers (S1 Table) were designed to genotype Cvi-0 versus Col-0 in the NILs and informative RILs from the INRA Versailles Col-0 × Cvi-0 RIL population. The markers were also used to genotype ozone-sensitive individuals from segregating F2 populations. Mapping population was created by crossing cis (Col-0) and C24 as an Arabidopsis accession with low stomatal conductance. High water loss from excised leaves and decreased responses to high CO2 were used as a selective trait. Rough mapping with 22 markers using 59 F2 samples showed linkage to the bottom of chromosome 2, at the marker UPSC_2–18415 at 18. 4 Mbp. Pooled genomic DNA from 66 selected F3 plants was used for sequencing. Whole genome sequencing was conducted with Illumina HiSeq 2000, and the reads were mapped against Col-0 genome (release TAIR10) by BGI Tech Solutions (Hong Kong). Genome sequence data is available from the NCBI BioProject database with the accession number PRJNA345097 and PRJNA343292. For mapping the genomic area of the mutation, the Next Generation Mapping tool was used [42], which positioned the mutation on chromosome 2 between 18,703,644 –19,136,098 bp. The deletion mutation in cis was verified by PCR to be 4,770 bp (at the position 18,945,427–18,950,196 bp). MPK12 and its promoter were amplified from Col-0 or Cvi-0 genomic DNA using Phusion (Thermo Fisher Scientific) and Gateway (Invitrogen) cloned into entry vector pDONR-Zeo. Subsequently, the genes were cloned into pGWB13 and pMCD100. Plants were transformed with floral dipping [43]. Total DNAs from different genotyping plants were extracted by CTAB method, and 12 micrograms of total DNA was digested by HindIII or EcoRI. The DNAs were running on the gel and transformed onto Nylon membrane. Hybridization was performed with digoxigenin-labeled specific genomic DNA amplified by primers F3 and R4 for 12 h. The membrane was washed several times by washing buffer and Maleic acid buffer. The membrane was blocked by blocking solution for 1 h at room temperature and washed and incubated with anti-DIG-AP for 30 min. Detection was performed using substrate DIG CSPD. Seeds were planted on a soil mixture consisting of 2: 1 (v: v) peat: vermiculite and grown through a hole in a glass plate covering the pot as described previously [44]. Plants were grown in growth chambers (MCA1600, Snijders Scientific, Drogenbos, Belgium) at 12 h/12 h day/night cycle, 23°C/20°C temperature, 100 μmol m-2 s-1 light, and 70% relative humidity (RH). For gas exchange experiments, 24- to 30-d-old plants were used. Stomatal conductance of intact plants was measured using a rapid-response gas exchange measurement device consisting of eight through-flow whole-rosette cuvettes [44]. The unit of stomatal conductance mmol m-2 s-1 reflects the amount of H2O moles that exits the plant through stomata per one m2 of leaf area per second. Prior to the experiment, plants were acclimated in the measurement cuvettes in ambient CO2 concentration (~400 ppm), 100 μmol m-2 s-1 light (if not stated otherwise), and ambient humidity (RH 65%–80%) for at least 1 h or until stomatal conductance was stable. Thereafter, the following stimuli were applied: decrease or increase in CO2 concentration, darkness, reduced air humidity, and ozone. CO2 concentration was decreased to 100 ppm by filtering air through a column of granular potassium hydroxide. In CO2 enrichment experiments, CO2 was increased by adding it to the air inlet to achieve a concentration of 800 ppm. Darkness was applied by covering the measurement cuvettes. In blue light experiments, dark-adapted plants were exposed to blue light (50 μmol m-2 s-1) from an LED light source (B42180, Seoul Semiconductor, Ansan, South Korea). The decreased or increased CO2 concentration, darkness, and blue light were applied for 58 min. In the long-term elevated CO2 experiment (Fig 1D and S1E Fig), CO2 concentration was increased from 400 ppm to 800 ppm for 2. 5 h. To calculate stomatal half-response time, the whole 2. 5-h stomatal response to elevated CO2 was scaled to a range from 0% to 100%, and the time when 50% of stomatal closure had occurred was calculated. Humidity was decreased by a thermostat system to 30%–40% RH, and stomatal conductance was monitored for another 56 min. In ozone experiments, the plants were exposed to 350–450 ppb of ozone for 3 min and stomatal conductance was measured for 60 min after the start of the exposure. In ABA-induced stomatal closure experiments, 5 μM ABA solution was applied by spraying as described in [45]. At time point 0, plants were removed from cuvettes and sprayed with either 5 μM ABA solution (5 μM ABA, 0. 012% Silwet L-77 [PhytoTechnology Laboratories], and 0. 05% ethanol) or control solution (0. 012% Silwet L-77 and 0. 05% ethanol). Thereafter, plants were returned to the cuvettes and stomatal conductance was monitored for 56 min. In ABA-induced inhibition of stomatal opening experiments, plants were acclimated in measurement cuvettes in darkness. At time point 0, plants were removed from cuvettes and sprayed with 2. 5 μM ABA solution (2. 5 μM ABA, 0. 012% Silwet L-77 [PhytoTechnology Laboratories], and 0. 05% ethanol) or control solution (0. 012% Silwet L-77 and 0. 05% ethanol). Thereafter, plants were returned to the cuvettes, dark covers were removed, and stomatal conductance was monitored in light for 56 min. Prior to the measurement of the diurnal pattern of stomatal conductance, plants were preincubated in the measurement cuvette for at least 12 h in respective light and humidity conditions. Plants were measured in 16-min intervals. WUE was calculated based on the data of diurnal experiments as an average of daytime light period (from 9: 00 to 17: 00). CO2-induced stomatal conductance in S2 Fig was measured as following. Five-week-old healthy plants growing in a growth chamber with 70% humidity and a 16 h light/8 h dark condition were used for stomatal conductance analyses at different CO2 concentrations by a LiCOR-6400XT, as previously described [13]. Relative stomatal conductance values were normalized relative to the last data point preceding the [CO2] transitions (400 to 800 or 1,000 ppm). The MPK12 deletion mutant mpk12-4 and wild-type plants were grown in a growth chamber at 70% humidity, 75 μmolm-2 s-1 light intensity, 21°C, and 16 h light/8 h dark regime. Leaf epidermal layers from 2-wk-old plants of both genotypes were preincubated in an opening buffer (10 mM MES, 10 mM KCl, and 50 mM CaCl2 at pH 6. 15) for 2 h, and stomata were individually imaged and tracked for measurement before treatment. After that, the leaf epidermal layers were incubated with buffers containing 10 μM ABA for 30 min and the individually tracked stomata were imaged. Stomatal apertures were measured by ImageJ software and genotype-blind analyses were used. The data presented are means and SEM n = 3 experiments, with 30 stomata per experiment and condition. Plants at the age of 28–30 d were used for stomatal index and density measurements. Rosette leaves of equal size were excised, and the abaxial side was covered with the dental resin (Xantopren M mucosa, Heraeus Kulzer, Germany). Transparent nail varnish was applied onto the dried impressions after the removal of the leaves. The hardened nail varnish imprints were attached onto a microscope glass slide with a transparent tape and imaged under a Zeiss SteREO Discovery. V20 stereomicroscope. For quantification, an image with the coverage of 0. 12 mm2 was taken from the middle of the leaf, next to the middle vein. In total, 81–84 plants per line from two independent biological repeats were analyzed—one leaf from each plant, one image from each leaf. Stomatal index was calculated with the following formula: SI = Stomatal density / (Density of other epidermal cells + Stomatal density). For the stomatal complex length measurements, plants at the age of 28–35 d were used. Whole leaves were preincubated for 4 h abaxial side down in the buffer (10 mM MES, 5 mM KCl, 50 μM CaCl2, pH 6. 15 [with TRIS]) in the light. Four to six plants per genotype and one leaf per plant were analyzed, and altogether 84–126 stomatal complexes per genotype were measured. Interactions between MPK12 and selected protein kinases and phosphatases were tested in pairwise split-ubiquitin Y2H assays using the DUALhunter and DUALmembrane 3 kits (Dualsystems Biotech). For bait construction, the coding sequences of MPK12 were PCR-amplified from total cDNAs from Col-0 and Cvi-0. Other MPK12 variants with point mutations (K70R, Y122C, and D196G+E200A) were created by two-step overlap PCR using the Col-0 MPK12 as a template. HT1 was also PCR-amplified from Col-0 cDNA. All MPK12s and HT1 were digested with SfiI and cloned to the corresponding site in pDHB1, which contained the Cub-LexA-VP16 fusion. For prey constructs, coding sequences of each selected gene were amplified from total Col-0 cDNAs, digested with SfiI, and cloned into either pPR3-N (HT1, OST1, BLUS1, IBR5, MKP2, MPK12, MPK12G53R, MPK11) or pPR3-STE (SnRK2. 2, SnRK3. 11, ABI1, ABI2, HAB1, HAB2), which contained a mutated NubG. All primers used are listed in Table S1. The pAI-Alg5 with a native NubI was used as a positive prey control, whereas the pDL2-Alg5 containing NubG served as a negative control. For pairwise Y2H assays, the yeast strain NMY51 was cotransformed with bait and prey plasmids and grown on SD-Leu-Trp plates to select for presence of both plasmids. At least ten colonies from each transformation were pooled and resuspended in water to an OD600 of 0. 5, from which 100,1, 000, and 10,000x serial dilutions were prepared and spotted on SD-Leu-Trp and SD-Leu-Trp-His-Ade plates. SD-Leu-Trp plates were incubated at 30°C for 2 d, photographed, and used for β-galatosidase overlay assays. SD-Leu-Trp-His-Ade plates were incubated for 2–4 d and photographed. The quantitative β-galactosidase assay was performed with three pools of ten independent colonies from each pairwise combination using the Yeast β-galactosidase assay kit (Thermo Fisher Scientific) by the nonstop quantitative method. Binary constructs containing split YFPs were designed and generated for cloning genes of interest by the ligation independent cloning (LIC) method as described in [18]. Each gene of interest was amplified by two consecutive PCR reactions: first with gene-specific primers and later with a pair of universal primers designed specifically for the LIC method. All primers used are listed in S1 Table. To prepare vectors for LIC, plasmids of 35S: YFPn and 35S: YFPc were linearized by PmlI digestion, followed by T4 DNA polymerase treatment with dGTP to create 15–16 nucleotide 5ʹ-overhangs. For insert preparation, the final PCR products of target genes were incubated with T4 DNA polymerase in the presence of dCTP to create the complementary overhangs with the vectors. Both vector and insert were mixed at room temperature and proceeded with Escherichia coli transformation after 5 min. The final constructs were sequence verified and transformed to Agrobacterium tumefaciens GV3101 for agro-infiltration experiments. For the ratiometric BiFC assays, four different agrobacterial clones—each harboring a YFPn fusion, a YFPc fusion, the SLAC1-CFP internal control, or the gene silencing suppressor P19—were co-infiltrated to the leaves of N. benthamiana at an OD600 of 0. 02 for each clone in the infiltration buffer (10mM MES, 10mM MgCl2,200 μM acetosyringone). Images were acquired at 3 dpi with a Zeiss LSM710 confocal microscope using a 63x objective (for high magnification images) or a 20x objective (for fluorescence quantification). The YFP signals were excited by a 514 nm laser, and emission between 518–564 nm was collected. The CFP signals were excited by a 405 nm laser, and emission at 460–530 was collected. Z-stack images of approximately 15 μm thickness were collected, and all images were acquired at the 16-bit depth for a higher dynamic range. The fluorescence intensity was measured by the ImageJ software. The leaf samples used for imaging were collected and used for protein extraction followed by western blot analysis. The leaf samples (30–40 mg) were ground under liquid nitrogen and boiled for 10 min in 100 μL of 6X Laemmli buffer. 12 μL of each sample were separated on 10% SDS polyacrylamide gel. After SDS-PAGE, proteins were transferred onto nitrocellulose membrane. Immunodetection of HA-tagged proteins was performed with a monoclonal anti-HA antibody. The MPK12 cDNA was cloned into a vector containing the N-terminal half of luciferase (nLUC) and HT1 was cloned into the cLUC. The constructs in the A. tumefaciens strain GV3101 were co-infiltrated into N. benthamiana leaves with P19 at an OD600 of 0. 8. The infiltrated leaves after 3 d of infiltration were harvested for bioluminescence detection. Images were captured with a CCD camera. Arabidopsis guard cell protoplasts were isolated as described previously [46]. Guard cell protoplasts were washed twice with a washing solution containing 1 mM MgCl2,1 mM CaCl2,5 mM MES, and 500 mM D-sorbitol (pH 5. 6 with Tris). During patch clamp recordings of S-type anion currents, the membrane voltage started at +35 to –145 mV for 7 s with –30 mV decrements, and the holding potential was +30 mV. The bath solutions contained 30 mM CsCl, 2 mM MgCl2,10 mM MES (Tris, pH 5. 6), and 1 mM CaCl2, with an osmolality of 485 mmol/kg. The pipette solutions contained 5. 86 mM CaCl2,6. 7 mM EGTA, 2 mM MgCl2,10 mM Hepes-Tris (pH 7. 1), and 150 mM CsCl, with an osmolality of 500 mmol/kg. The free calcium concentration was 2 μM. The final osmolalities in both bath and pipette solutions were adjusted with D-sorbitol. Mg-ATP (5 mM) was added to the pipette solution before use. 13. 5 mM CsHCO3 (11. 5 mM free [HCO3-] and 2 mM free [CO2]) was freshly dissolved in the pipette solution before patch clamp experiments. The concentrations of free bicarbonate and free CO2 were calculated using the Henderson–Hasselbalch equation (pH = pK1 + log [HCO3-] / [CO2]). pK1 = 6. 352 was used for the calculation. [HCO3-] represents the free bicarbonate concentration and [CO2] represents the free CO2 concentration. For in vitro kinase assays, the respective sequences of HT1, HT1 K113M, MPK11, MPK12, MPK12 G53R, MPK12 K70R, and MPK12 Y122C were cloned into a pET28a vector (Novagen, Merck Millipore) using primers listed in S1 Table. Point mutations corresponding to K113M in HT1, K70R in MPK12, and Y122C in MPK12 were created with two-step PCR using primers listed in S1 Table. MPK4 was cloned as previously described [18]. 6xHis-HT1WT, 6xHis-HT1 K113M, 6xHis-MPK12,6xHis-MPK12 G53R, 6xHis-MPK12 K70R, 6xHis-MPK12 Y122C, 6xHis-MPK11,6xHis-MPK4 WT, and 6xHis-MPK4 G55R were expressed in E. coli BL21 (DE3) cells. A 2 mL aliquot of an overnight culture was transferred to a fresh 1 L 2xYT medium and grown at 37°C to an absorbance of ~0. 6 at OD600. The cultures were chilled to 16°C and recombinant protein expression was induced by 0. 3 mM isopropyl b-D-thiogalactopyranoside for 16 h. The cells were harvested by centrifugation (5,000 rpm, 10 min, 4°C) and stored at –80°C until use. All purification procedures were carried out at 4°C. The cells were resuspended in 30 mL of lysis buffer (50 mM Tris-HCl [pH 7. 4], 300 mM NaCl, 5% [v/v] glycerol, 1% [v/v] Triton X-100,1 mM PMSF, 1 μg/ml aprotinin, 1 μg/ml pepstatin A, 1 μg/ml leupeptin) and lysed using an Emulsiflex C3 Homogenizer. Cell debris was removed by centrifugation at 20,000 rpm for 30 min. The protein-containing supernatant was mixed for 1 h at 4°C with 0. 20 mL of Chelating Sepharose Fast Flow resin (GE Healthcare), charged with 200 mM NiSO4 and pre-equilibrated in the lysis buffer. The protein–resin complex was packed into a column, and the beads were washed with 5x10 column volumes (CV) of a wash buffer I (50 mM Tris-HCl [pH 7. 4], 600 mM NaCl, 5% [v/v] glycerol, 1% [v/v] Triton X-100), 5x10 CV of a wash buffer II (50 mM Tris-HCl [pH 7. 4], 300 mM NaCl, 5% [v/v] glycerol, 0. 1% [v/v] NP-40), and 2x10 CV of a wash buffer III (50 mM Tris-HCl [pH 7. 4], 150 mM NaCl, 5% [v/v] glycerol, 0. 1% [v/v] NP-40). The protein was eluted by incubating the beads for 5 min at room temperature with an imidazole-containing elution buffer (50 mM Tris-HCl, 150 mM NaCl, 5% [v/v] glycerol, 0. 1% [v/v] NP-40,300 mM imidazole). MPK12 proteins were concentrated and imidazole was removed by Millipore Amicon Ultra-0. 5 Centrifugal Filter Concentrators (NMWL 3000). Glycerol was added to a final concentration of 20% (v/v), and 20 μL aliquots of the eluted protein were snap-frozen in liquid nitrogen and stored at –80°C. Protein concentrations were estimated on 10% SDS-polyacrylamide gel using BSA as a standard. HT1 kinase activity assay was performed by incubating a constant amount of purified recombinant HT1 and 0–30 μM MPK12,0–20 μM MPK4, or 0–10 μM MPK11 in a reaction buffer (50 mM Tris-HCl [pH 7. 4], 150 mM NaCl, 20 mM MgCl2,60 mM imidazole, 1 mM DTT, 0. 2 mg/ml insulin) at room temperature for 10 min. Then, casein (1 mg/ml), 500 μM ATP, and 100 μCi/ml 32P-γ-ATP were added and reaction aliquots were taken at the 30 min time point. Reactions were stopped by the addition of SDS loading buffer. Proteins were separated on a 10% SDS-polyacrylamide gel and visualized by Coomassie brilliant blue R-250 (Sigma) staining. HT1 activity was determined by autoradiography and quantified by ImageQuant TL Software. Sequence searches and alignments were conducted with SWISS-MODEL [47]. The crystal structure with the best sequence identity and resolution was selected for building homology models. Arabidopsis MPK12 and MPK4 have sequence identity to the 3 Ångstrom resolution Arabidopsis MPK6 structure (5CI6; [33]) of 64. 61% and 70. 67%, respectively. This structure was then used to construct models for the wild-type and mutant structures. The RMSD from aligning the structures for MPK12 and MPK12 G53R was 0. 324 Ångstroms (i. e. , a close structural similarity). Structures were checked for clashes and with quality controls and were then superposed. Statistical analyses were performed with Statistica, version 7. 1 (StatSoft Inc. , Tulsa, Oklahoma, United States). All effects were considered significant at p < 0. 05.
Human activities have increased the concentrations of CO2 and harmful air pollutants such as ozone in the troposphere. These changes can have detrimental consequences for agricultural productivity. Guard cells, which form stomatal pores on leaves, regulate plant gas exchange. To maintain photosynthesis, stomata open to allow CO2 uptake, but at the same time, open stomata lead to loss of water and allow the entrance of ozone. Elevated atmospheric CO2 levels reduce stomatal apertures, which can improve plant water balance but also increases leaf temperature. Using genetic approaches—in which we exploit natural variation and mutant analysis of thale cress (Arabidopsis thaliana) —we find that MITOGEN-ACTIVATED PROTEIN KINASE 12 (MPK12) and its inhibitory interaction with another kinase, HIGH LEAF TEMPERATURE 1 (HT1) (involved in guard cell CO2 signaling), play a key role in this regulatory process. We have therefore identified a mechanism in which guard cell CO2 signaling regulates how efficiently plants use water and cope with the air pollutant ozone.
plant anatomy
stem anatomy
ecology and environmental sciences
guard cells
chemical compounds
atmospheric science
plant cell biology
brassica
ions
anions
computational biology
stomata
plant science
model organisms
genome analysis
plants
arabidopsis thaliana
research and analysis methods
physical chemistry
genomics
biological databases
chemistry
atmospheric chemistry
leaves
environmental chemistry
plant cells
plant and algal models
cell biology
earth sciences
ozone
database and informatics methods
carbon dioxide
biology and life sciences
cellular types
physical sciences
greenhouse gases
genetics
genomic databases
organisms
Natural Variation in Arabidopsis Cvi-0 Accession Reveals an Important Role of MPK12 in Guard Cell CO2 Signaling