Integrated Analysis of Molybdenum Nutrition and Nitrate Metabolism in Strawberry

The blends of flavor compounds produced by fruits serve as biological perfumes used to attract living creatures, including humans. They include hundreds of metabolites and vary in their characteristic fruit flavor composition. The molecular mechanisms by which fruit flavor and aroma compounds are gained and lost during evolution and domestication are largely unknown. Here, we report on processes that may have been responsible for the evolution of diversity in strawberry (Fragaria spp) fruit flavor components. Whereas the terpenoid profile of cultivated strawberry species is dominated by the monoterpene linalool and the sesquiterpene nerolidol, fruit of wild strawberry species emit mainly olefinic monoterpenes and myrtenyl acetate, which are not found in the cultivated species. We used cDNA microarray analysis to identify the F. ananassa Nerolidol Synthase1 (FaNES1) gene in cultivated strawberry and showed that the recombinant FaNES1 enzyme produced in Escherichia coli cells is capable of generating both linalool and nerolidol when supplied with geranyl diphosphate (GPP) or farnesyl diphosphate (FPP), respectively. Characterization of additional genes that are very similar to FaNES1 from both the wild and cultivated strawberry species (FaNES2 and F. vesca NES1) showed that only FaNES1 is exclusively present and highly expressed in the fruit of cultivated (octaploid) varieties. It encodes a protein truncated at its N terminus. Green fluorescent protein localization experiments suggest that a change in subcellular localization led to the FaNES1 enzyme encountering both GPP and FPP, allowing it to produce linalool and nerolidol. Conversely, an insertional mutation affected the expression of a terpene synthase gene that differs from that in the cultivated species (termed F. ananassa Pinene Synthase). It encodes an enzyme capable of catalyzing the biosynthesis of the typical wild species monoterpenes, such as alpha-pinene and beta-myrcene, and caused the loss of these compounds in the cultivated strawberries. The loss of alpha-pinene also further influenced the fruit flavor profile because it was no longer available as a substrate for the production of the downstream compounds myrtenol and myrtenyl acetate. This phenomenon was demonstrated by cloning and characterizing a cytochrome P450 gene (Pinene Hydroxylase) that encodes the enzyme catalyzing the C10 hydroxylation of alpha-pinene to myrtenol. The findings shed light on the molecular evolutionary mechanisms resulting in different flavor profiles that are eventually selected for in domesticated species.

The importance of molybdenum for plant growth is disproportionate with respect to the absolute amounts required by most plants. Apart from Cu, Mo is the least abundant essential micronutrient found in most plant tissues and is often set as the base from which all other nutrients are compared and measured. Molybdenum is utilized by selected enzymes to carry out redox reactions. Enzymes that require molybdenum for activity include nitrate reductase, xanthine dehydrogenase, aldehyde oxidase and sulfite oxidase. Loss of Mo-dependent enzyme activity (directly or indirectly through low internal molybdenum levels) impacts upon plant development, in particular, those processes involving nitrogen metabolism and the synthesis of the phytohormones abscisic acid and indole-3 butyric acid. Currently, there is little information on how plants access molybdate from the soil solution and redistribute it within the plant. In this review, the role of molybdenum in plants is discussed, focusing on its current constraints in some agricultural situations and where increased molybdenum nutrition may aid in agricultural plant development and yields. Molybdenum deficiencies are considered rare in most agricultural cropping areas; however, the phenotype is often misdiagnosed and attributed to other downstream effects associated with its role in various enzymatic redox reactions. Molybdenum fertilization through foliar sprays can effectively supplement internal molybdenum deficiencies and rescue the activity of molybdoenzymes. The current understanding on how plants access molybdate from the soil solution or later redistribute it once in the plant is still unclear; however, plants have similar physiological molybdenum transport phenotypes to those found in prokaryotic systems. Thus, careful analysis of existing prokaryotic molybdate transport mechanisms, as well as a re-examination of know anion transport mechanisms present in plants, will help to resolve how this important trace element is accumulated.

Introduction Plants have developed complex biochemical and regulatory pathways to acquire mineral nutrients from the soil environment and distribute them to appropriate tissues. Natural populations of Arabidopsis thaliana (Arabidopsis) provide an excellent system to study how plants have adapted their mineral nutrient and trace element uptake pathways to thrive under different environmental conditions. Molybdenum (Mo) is an important micronutrient for plants, being incorporated into molybdopterin, an essential cofactor for enzymes involved in nitrate assimilation, sulfite detoxification, abscisic acid biosynthesis and purine degradation [1]. Molybdenum in either deficiency or excess has been demonstrated to inhibit plant growth and agricultural productivity [2]. The genes comprising the biochemical pathway that synthesizes the molybdopterin cofactor have been identified in plants, animals and microbes, but to date, a Mo transporter in plants has not been found [2]. The first committed step in molybdopterin biosynthesis occurs in the mitochondria [3], confirming the predicted sub-cellular localization of the enzymes [1]. The remaining 3 steps are thought to occur in the cytoplasm [3]. While a substantial amount is known about the biochemistry, enzymology and underlying genetics of molybdopterin biosynthesis, very little is known about the mechanisms for Mo uptake, distribution and accumulation in plants. In this study, natural variation in whole plant Mo accumulation has been coupled with genomics techniques and genetics to identify a mitochondrial Mo transporter (MOT1) that regulates whole plant Mo content in Arabidopsis. Alleles of this gene are demonstrated to be responsible for low Mo accumulation across a diversity collection of 92 Arabidopsis accessions. All soil grown plant ionomic data from this study is freely available at www.purdue.edu/dp/ionomics [4]. Results Shoot tissue from a geographically diverse panel of 98 Arabidopsis accessions (93 from [5] plus Bu-15, Col-4, Kas-1, Ler-0, Ler-2) was screened in an effort to identify accessions which have altered Mo content in shoot tissue (Figure 1A). Based on this survey it was determined that the shoot content of Mo in Arabidopsis is under genetic control (broad sense heritability H2 = 0.48), with an approximately 20-fold difference between the highest and lowest Mo levels observed (Figure 1A) across the diverse set of Arabidopsis accession tested. Shoot Mo content was found to be not normally distributed around the population mean (p<0.001), with 12 accessions (Ler-0, Ler-1, Ler-2, Van-0, Zdr-6, Kondara, KZ-9, Shadahara, Sorbo, Ll-0, Ts-5, Ws-0) accumulating less than 0.7 µg g−1 Mo, and 9 accessions (Ull2-5, Bur-0,Cvi-0, Nfa-10, Tamm-2, Tamm-27, Fab-2, Var2-1, Spr1-6) accumulating more than 3.1 µg g−1 Mo (grey bars in Figure 1A). We had previously identified Ler as a low Mo accumulating accession of Arabidopsis [6] and all Ler lines tested (which are likely genetically identical), were low in Mo. Shoot tissue of Ler-0 contains 70–80% less Mo compared to Col-0 (Figure 1B), and this difference from Col-0 is observed for Ler-0 when plants were grown with a broad range of Mo concentrations in the nutrient solution (Figure 1C). We selected this accession for further study due to the extensive genetic resources available for this accession, including the availability of genome sequence data and recombinant inbred lines (RIL), along with high density genotype data [7],[8]. 10.1371/journal.pgen.1000004.g001 Figure 1 Genetic and physiological analysis of mo in arabidopsis. A: Shoot Mo content across 98 accessions. Histogram of shoot Mo content in 98 Arabidopsis accessions which include 94 from Nordborg et al. (2005). Black bars indicate the distribution of lines having the mot1 Ler-0 deletion. Grey lines denote the low and high accessions, as detailed in the text. The black arrow denotes Col-0 Mo content. Shoot Mo concentrations are normalized so that the average of the Col-0 and Cvi-0 means included in each growth tray are equivalent across all trays. Plants were grown in soil for 5 weeks. Data represents median values (average n = 11.6) for each accession. B: Mo accumulation of Col-0, Ler-0, Van-0, mot1-1, st5.1-1 and the mot1-1st5.1-1 double mutant. Data is shown as a five number summary (the minimum, 1st quartile, median, 3rd quartile and maximum) for each line, and is summarized from an average of 10 replicate plants for each line. Lower case letters denote groups that are not significantly different from each other at P<0.01 with the Holm correction. Plants were grown in soil for 5 weeks. C: Shoot Mo accumulation in Arabidopsis in response to increasing levels of Mo in the nutrient solution. Mo accumulation in Col-0 (Black) and Ler-0 (Red) after 5 weeks of growth in soil at varying concentrations of Mo in the watering solution. Data is shown as a five number summary for each line, and is summarized from 6 replicate plants for each treatment. The analysis of Mo in shoot and root tissue of hydroponically grown Ler-0 and Col-0 plants confirmed the low shoot Mo content of Ler-0 (Figure 2A). Furthermore, Ler-0 also has a reduced Mo content in roots when compared to Col-0, suggesting that the low shoot Mo content is not due to enhanced accumulation of Mo in the roots, but rather to reduced Mo uptake by the roots. Grafting experiments were performed to determine if low shoot Mo in Ler-0 is determined by the root or shoot. Shoots and roots from 5-day old seedlings of Ler-0 and Col-0 were reciprocally grafted, and grafted plants grown for 4 weeks in soil with short days. Plants with Ler-0 roots had significantly lower (p<0.01) shoot Mo contents than plants with Col-0 roots, whether the shoots were Ler-0 or Col-0. The genotype of the shoot stock had no significant effect on Mo content of the shoot (Figure 3). From this it was concluded that the low shoot Mo content of Ler-0 is driven solely by the roots. 10.1371/journal.pgen.1000004.g002 Figure 2 Mo content in the roots and shoots of plants grown hydroponically. Mo content in Col-0 and Ler-0 after 4 weeks growth (A), and Col-0, mot1-1 and the mot1-1st5.1-1 double mutant after 3-weeks growth (B). Presented data are the means of at least three biological replicates, and error bars represent±SE. 10.1371/journal.pgen.1000004.g003 Figure 3 Shoot mo accumulation in Ler-0 is driven by the roots. Mo contents in Arabidopsis plants grafted at 5 days after germination and transferred to soil for growth were determined in self grafted plants of Col-0 (n = 32) and Ler-0 (n = 11), Col-0 shoot grafted onto Ler-0 root (n = 22), and Ler-0 shoot grafted onto Col-0 root (n = 15). Data is shown as a five number summary (the minimum, 1st quartile, median, 3rd quartile and maximum) for each line with outliers denoted by small circles. Mapping the Loci Responsible for the Low Mo Content of the Landsberg Erecta Arabidopsis Accession In a Ler-0×Col-0 cross 51 of the 200 F2 progeny analyzed were found to have low shoot Mo contents similar to the Ler-0 parent. This ratio is consistent with the hypothesis that the low Mo phenotype in Ler-0 is controlled by a single locus, or several closely linked loci (p<0.00001 by Shapiro test for normality). Similar segregation patterns were observed in an F2 population derived from a Ler-0 cross to an ionomics mutant (14501) in the Col-0 background. To obtain a rough map position, a bulk segregant analysis (BSA) experiment [9] was performed with microarray detection of genetic markers [10],[11], using (14501[Col-0]×Ler-0) F2 plants. Plants with the lowest shoot Mo contents (n = 40) and plants with Mo shoot contents similar to Col-0 (n = 40) were pooled separately, and genomic DNA from each pool hybridized to the Affymetrix Arabidopsis ATH1 DNA microarray. Using the oligonucleotide probes on the DNA microarray which show differential hybridization between Ler-0 and Col-0 as genetic markers (Single Feature Polymorphisms or SFP), the locus responsible for the low shoot Mo content in Ler-0 was mapped to an area centered at 11 Mb on chromosome 2 (Figure 4A). 10.1371/journal.pgen.1000004.g004 Figure 4 The locus determining low shoot Mo content in Ler-0 Maps to the MOT1 Gene. A: Bulk Segregant analysis of the low shoot Mo content in an F2 population from a Col-0×Ler-0 cross.Data are presented as a scaled pool hybridization difference (SPHD), representing the difference between the hybridization of the two pools at the SFPs, scaled so that a pure Col-0 pool would be at −1 and a pure Ler-0 pool would be at 1. The pools were prepared from F2 plants with a low Mo content (n = 40) and F2 plants with a high Mo content (n = 40). SFPs were scored after hybridization of genomic DNA prepared from these pools to Affymetrix ATH1 DNA microarrays. Dotted lines denote likely location of the causal loci. B: Shoot Mo content and genotype on chromosome II of selected Col-0×Ler-0 RILs. The genotype of each of the 106 markers determined by Singer et al. (2006) for chromosome II are shown; Col-0 alleles are denoted in black, Ler-0 in white. The average shoot Mo content (n = 12) for each line is shown, and, those with Col-0 shoot levels of Mo are underlined. Blue lines indicate the narrowed mapping interval on chromosome II (10.771 to 11.056 Mb). C: Structure of the MOT1 gene. The DNA sequence of MOT1 showing location of the T-DNA insert in mot1-1, and the 50 base pair deletion in the 5′ UTR in the seven accessions with low shoot Mo content aligned with the Col-0 DNA sequence, with the TATA box underlined. To further narrow down the map position of the locus controlling low shoot Mo content in Ler-0, the Col-4×Ler-0 RIL population [12] was used to identify seven recombinants in the mapping region we had previously determined from the BSA. DNA microarray-based genotyping of this Col-4×Ler-0 RIL set was used to further refine the break points between Col-4 and Ler-0 genotypes [7],[8]. The shoot Mo contents of these seven RILs showed a clear segregation with the genetic markers for Col-4 and Ler-0 within our mapping region, allowing us to classify these lines as having either the Col-0 or the Ler-0 allele for the low Mo locus (Figure 4B). The precise breakpoints identified by Singer et al. [8] allowed the mapping interval to be narrowed to 346 kb on chromosome 2 (10.771 to 11.056 Mb), an interval containing 81 genes. Candidate genes from this interval were selected based on annotation and expression differences between Col-0 and Ler-0 (T. Singer & S. Briggs, personal communication). T-DNA insertional alleles for these candidate genes were obtained, and the plants scored for low shoot Mo content compared to wild type Col-0. A null mutant (mot1-1) with an insertion disrupting the coding region of the gene At2g25680 (Salk_118311, Figure 4D), was observed to phenocopy the Ler-0 low shoot Mo content when grown in either soil (Figure 1B), or shoots and roots when grown hydroponically (Figure 2). Differences in the absolute concentrations of Mo between Col-0 in Figure 2A and 2B are related to differences in growth conditions between these two experiments. The At2g25680 gene was originally predicted to be a putative sulfate transporter, and named AtSULT5.2 [13]. We have renamed this gene MOT1 (molybdenum transporter 1) based on its phenotype of low shoot Mo content. Furthermore, we detected no change in the shoot content of S in mot1-1 (Figure 5) or in the content of Li, B, Na, Mg, P, K, Ca, Mn, Fe, Co, Ni, Cu, Zn, As, Se, and Cd, providing additional support for the reannotation of AtSULT5.2 as MOT1. Quantitative real-time RT-PCR of the MOT1 transcript in mot1-1 and Ler-0 revealed that both these low shoot Mo lines had significantly reduced expression levels of MOT1 in both root and shoot tissue, compared to Col-0 (Figure 6). Van-0, a second low shoot Mo accession (Figure 1B) was also confirmed by qRT-PCR to have low expression of MOT1 (Figure 6). Significantly, we observed no differences in shoot S content between Col-0 and either Ler-0 or Van-0 (Figure 5). 10.1371/journal.pgen.1000004.g005 Figure 5 Sulfur accumulation in shoots of Col-0, Ler-0, Van-0, mot1-1, st5.1-1 and the mot1-1st5.1-1 double mutant plants. Data is shown as a five number summary (the minimum, 1st quartile, median, 3rd quartile and maximum) for each line, and is summarized from an average of 10 replicate plants for each line. No significant differences were observed. Plants were grown in soil for 5 weeks. The data is from the same plants as in Figure 1B. 10.1371/journal.pgen.1000004.g006 Figure 6 Expression of MOT1 in Col-0, Ler-0, Van-0 and mot1-1. Steady state MOT1 expression level was compared in shoots (A) and roots (B) of Col-0, Ler-0, Van-0, and mot1-1 using quantitative real time PCR (qRT-PCR). RNA was isolated from shoot and root of plants grown in soil for 5 weeks under short day conditions For normalization across samples expression of the Actin 1 gene was used and the relative expression of MOT1 calculated using the 2(−ΔCT) method. Presented data are the means of at least three biological replicates, (2ˆ(ΔCT)) each analyzed 4 times by qRT-PCR. Error bars represent±SD. To establish if MOT1 is the locus responsible for the low shoot Mo content of Ler-0 and Van-0, we crossed mot1-1 and Col-0 to both Ler-0 and Van-0 to test for complementation (Figure 7). F1 plants from the Ler-0×Col-0 and Van-0×Col-0 crosses contained significantly different levels of shoot Mo from either parent (p<0.005 for all pairwise t-tests), suggesting that the Col-0 allele of the low Mo locus could only partially complement the Ler-0 allele. F1 plants from the Ler-0×mot1-1 and Van-0×mot1-1 crosses were found to have significantly lower shoot Mo contents than similar plants from the Ler-0×Col-0 and Van-0×Col-0 crosses (p<0.0005). Such data establishes that mot1-1 is deficient in complementing the low shoot Mo content of both Ler-0 and Van-0. This is strong evidence confirming that the Ler-0 and Van-0 alleles are allelic with the recessive loss of function allele of MOT1. 10.1371/journal.pgen.1000004.g007 Figure 7 Complementation Studies Indicate MOT1 Natural Variant Is Responsible for Reduced Shoot Mo Content in Ler-0 and Van-0. Shoot Mo content of Col-0, Ler-0, Van-0, mot1-1, and F1 plants from crosses between Col-0×Ler-0, Col-0×Van-0, Ler-0×mot1-1, Van-0×mot1-1and Col-0×mot1-1 in 5-week old soil grown plants are shown. Data is represented as a five number summary (the minimum, 1st quartile, median, 3rd quartile and maximum) for each line, and is summarized from an average of 21 replicate plants for each line. Lower case letters denote groups that are not significantly different from each other at P<0.01 with the Holm correction. To determine the polymorphism in the MOT1 Ler-0 allele causal for low shoot Mo content, we sequenced MOT1, including 1 kb upstream and 200 bp downstream of the coding sequence in both Ler-0 and Van-0. We observed 18 polymorphisms in common between Ler-0 and Van-0, as well as several polymorphisms unique to each accession, when compared to the Col-0 reference sequence. These include 15 single nucleotide polymorphisms (SNPs) in the 1 kb upstream region, two SNPs that change two amino acids (I68T and V30L) in the coding region, and a 53 base pair (bp) deletion 27 nucleotides upstream from the translation start site (Text S1). The deletion includes the TATA box (Figure 4C). The altered expression of MOT1 in both of the low shoot Mo accessions, Ler-0 and Van-0, suggested that this 5′ deletion may be the causal polymorphism driving low shoot Mo content in these accessions. To obtain further evidence that this deletion is the casual polymorphism driving low shoot Mo content, we performed an association analysis by sequencing the MOT1 5′ promoter region containing the 53 bp deletion in Ler-0 and Van-0 across 92 of the accessions originally screened for shoot Mo content (Text S2). Combining this information with the Nordborg [5] genotypes, we were able to scan for significant genetic associations with low shoot Mo content. The 53 bp deletion identified in Ler-0 and Van-0 was found in seven of the 92 accessions tested, and all accessions with the deletion had low shoot Mo content compared to the overall distribution of shoot Mo contents (Figures 4C and 1A). The distribution of p-values for genome-wide associations with shoot Mo contents were skewed towards significance, suggesting a relationship between Mo content and the underlying population structure (Figure S1), making the evaluation of individual loci difficult. However, when kinship and population structure were taken into account [14], the presence of the 53 bp deletion was found to be highly significantly associated with low shoot Mo content (p<0.0001) and accounted for ∼14% of the total variation in Mo accumulation. Once the MOT1 Ler loci is accounted for, there were several other markers which showed significant associations with Mo accumulation, and these may represent additional loci of interest (Text S3). To establish that MOT1 has the capacity to transport Mo, the Arabidopsis MOT1 cDNA was expressed in yeast. Yeast expressing MOT1 were observed to specifically accumulate five time more Mo than vector only controls (p<1E-14, Figure 8). Furthermore, the accumulation of no other element, including Na, Mg, P, S, K, Ca, Mn, Fe, Co, Ni, Cu, Zn, and Cd, was observed to be altered more than 20% in two independent experiments. This evidence is consistent with MOT1 being a specific molybdate transporter. 10.1371/journal.pgen.1000004.g008 Figure 8 Cell Associated Mo in Yeast Expressing Arabidopsis MOT1. Cell associated Mo in yeast transformed with either p416 vector only or vector containing cDNAs encoding ST5.1 and MOT1 after growth for 24 hours. Data is represented as a five number summary (the minimum, 1st quartile, median, 3rd quartile and maximum) for each line, and is summarized from n = 32 replicate yeast cultures for each genotype. Localization of MOT1 Expression and Sub-Cellular Localization of the MOT1 Protein To determine the tissue localization of MOT1 expression, Col-0 was transformed with a 1.8 kb MOT1 promoter-GUS construct. In all of the promoter-GUS lines examined, GUS staining was observed in the roots, hypocotyls and leaves (Figure 9). In roots, GUS staining was most pronounced just behind the growing root tip in the primary root (Figure 9A, B), and the lateral roots (data not shown). Cross sections show that the strong GUS staining behind the root tip was restricted mainly to the protodermal cells (Figure 9B2). At the beginning of the elongation zone, GUS staining was mainly restricted to the epidermis and cortex (Figure 9C2). Thereafter, GUS staining in the root also occurred in the vascular tissue (Figure 9D). In the hypocotyls the GUS staining was also mainly restricted to the vascular tissue (Figure 9E). In fully expanded leaves GUS staining was found in the vascular tissue. However, the main vein was less intensely stained than the lateral veins (Figure 9F). During flowering GUS activity was also visible in the vasculature of the stem leaves but not in the vasculature of the stem, flowers or developing siliques including seeds (data not shown). 10.1371/journal.pgen.1000004.g009 Figure 9 Tissue Localization of Expression of MOT1 Using GUS Activity Visualized by Histochemical Staining. Pictures represent histochemical analysis of GUS activity in Arabidopsis plants stably transformed with a MOT1-promoter-GUS construct. A: Primary root shown from root tip to the beginning of the lateral root development. Boxes denote close-ups shown in B,C and D; B: Root tip and cross section shown in insert panel B2. C: Root elongation zone with a cross section shown in insert panel C2; D: Root shown from between the elongation zone and the start of the lateral root production zone; E: Hypocotyl; F: Fully expanded leaves. Pd – protoderm; co – cortex; vb vascular bundle; ep – epidermis. The sub-cellular localization of the MOT1 protein was determined by transiently expressing a MOT1 C-terminal GFP translational fusion construct in shoot derived Col-0 protoplasts (Figure 10A–10D), and by stable ectopic expression of a similar construct in Col-0 (Figure 10E–10G). The GFP signal was observed to co-localize with the mitochondrial marker F-ATPase–RFP in shoot derived protoplasts transiently expressing the construct, and with the Mitotracker Red dye in roots of the stably transformed lines. The experimentally determined mitochondrial localization for MOT1 is in good agreement with several sub-cellular prediction programs (summarized at the SUBA database, [15]), which predict a mitochondrial targeting sequence at the N-terminus of MOT1. 10.1371/journal.pgen.1000004.g010 Figure 10 Subcellular localization of MOT1. MOT1::GFP was transiently expressed in Arabidopsis leaf protoplasts co transformed with F1-ATPase::RFP: (A) DIC (B) GFP filter (C) RFP filter and (D) merged image. Roots of Arabidopsis stably transformed with MOT1::GFP and stained with Mitotracker Red: (E) Red Filter (F) GFP Filter (G) Merged. Phylogenetic analysis of the sulfate transporter family in Arabidopsis and rice [13],[16] reveal two Arabidopsis genes, MOT1 and ST5.1, to have diverged significantly from the other sulfate transporter family members, and each Arabidopsis gene has a rice ortholog. Given the sequence similarity between ST5.1 and MOT1, the shoot Mo content of a st5.1-1 T-DNA insertion line (Salk_015044) was analyzed to determine if it also shows the low Mo phenotype observed in mot1-1. We were unable to detect any significant changes in the Mo content of shoot of st5.1-1 when grown in soil and the roots and shoot Mo accumulation of a mot1-1/st5.1-1 double mutant was not significantly different from the mot1-1 mutant alone. (Figures 1B and 2B). The Mo content of yeast heterologously expressing the ST5.1 cDNA was found not to be reproducibly significantly different from vector only controls in two independent experiments (Figure 8). Thus, we can find no evidence that ST5.1 is also a Mo transporter. A search of the PiiMS database [4]; www.purdue.edu/ionomics) found four T-DNA lines with insertions in sulfate transporters, representing the ST1, ST2 and ST3 subfamilies (At3g15990, At4g02700, At1g77990, At4g08620), none of which accumulated significantly different levels of Mo than Col-0. Discussion Molybdenum is one of the 14 essential minerals required by plants. Despite its importance as a cofactor in processes ranging from nitrogen metabolism to hormone biosynthesis, we still know relatively little about the regulation, uptake and transport of this transition metal. Using an ionomics approach to identify genes that affect the elemental composition of plants, we identified MOT1 as the causal gene driving reduced shoot Mo in various accessions of Arabidopsis. We have combined several lines of evidence to support this conclusion. First, a 54 bp deletion in the promoter of MOT1 was found to be strongly associated (p<0.0001) with low shoot Mo content across 92 Arabidopsis accessions. Given the strong association between the presence of this deletion and low shoot Mo content, and the rate of linkage disequilibrium decay in Arabidopsis [17], if this deletion is not the causal polymorphism, it is within 20 kb of the causal polymorphism. Second, deficiency complementation with a T-DNA allele (SALK_118311) indicates that the MOT1 allele found in Ler-0 and Van-0, accessions with a low content of shoot Mo, is responsible for this reduced Mo content. Third, MOT1 shows reduced expression in both Ler-0 and Van-0 compared to Col-0, and the mot1-1 null allele in the Col-0 background phenocopies the low shoot Mo observed in both Ler-0 and Van-0. Given the fact that MOT1 belongs to the sulfate transporter superfamily, and can transport Mo when expressed in yeast, it is easy to imagine how reduced expression of a Mo transporter could lead to low shoot Mo content, either via reduction in uptake from the soil and/or translocation to the shoot. In Col-0, the functional MOT1 allele is strongly expressed in the root differentiation zone and in mature vasculature tissue of both the roots and the shoots, suggesting a defect in either or both roles could be the possible explanation for the observed phenotype. Our grafting experiments clearly show that the Mo defect is associated with the roots. Surprisingly, the MOT1 protein is not localized to the plasma membrane of roots cells where it could function in uptake into cells, but rather MOT1 is localized to the mitochondria. Based on these observations, and the grafting data, it is hypothesized that MOT1 regulates whole plant Mo accumulation at the level of the mitochondria in the root. Interestingly, the first committed step in molybdopterin biosynthesis has recently been shown to occur in the mitochondria, and this is consistent with the mitochondria acting as a control point in regulating whole plant Mo content [3]. Given that characterized members of the sulfate transporter superfamily are SO4 −2/H+ co-transporters, we speculate that MOT1 is transporting MoO4 −2 from the acidic mitochondrial intermembrane space to either the cytoplasm or the matrix. While we have localized MOT1 to the mitochondria, the question of how Mo enters the root cells remains. Based on its homology, ST5.1-1 is a candidate for this role, however a ST5.1 C-terminal GFP fusion was found to localize to the vacuole (Buchner and Hawkesford, unpublished). Additionally, the st5.1-1 T-DNA insertional mutant does not have altered shoot Mo content, and heterologous expression of ST5.1 cDNA in yeast has no effect on Mo accumulation. ST5.1 also appears not to interact with MOT1 since the double mutant st5.1mot1-1 showed the same reduction in Mo content as mot1-1. Alternatively, the putative plasma membrane molybdate transporter could be from a family unrelated to the SUL gene family, as multiple gene families have been shown to transport Zn2+ and Ca2+, for example [18],[19]. Finally, it remains possible that MoO4 2− is transported across the plasma membrane through a promiscuous transporter(s) with broad ion specificity as shown for E. coli [20]. Both sulfate and phosphate starvation have been shown to increase Mo accumulation, which suggests that Mo may be transported across the plasma membrane by sulfate and phosphate transporters [21],[22]. Sequencing results show that the MOT1 Ler-0 allele has a frequency of approximately 7% (7/92) in the natural diversity collection of Arabidopsis obtained from populations collected from a broad geographical region. This frequency is higher than we would expect if the lowered Mo content strongly reduced fitness. For example, the overall reduction in Mo content might cause a reduction in molybdopterin, negatively impacting the activity of MoCo containing enzymes like nitrate reductase. However, we found no significant reduction in growth, N accumulation or nitrate reductase activity in mot1-1 lines when grown with nitrate as the sole N source (data not shown). This suggests that MoCo levels are not limiting in mot1-1. Alternatively, loss of MOT1 function might increase the fitness of Arabidopsis by some as yet unknown process, and the association of Mo with population structure is consistent with Mo accumulation having a selective effect. However, an analysis of haplotype sharing [23] around this gene gave no indication of recent selection on the MOT1 Ler-0 allele (C. Toomajian, unpublished). Finally, it has been noted that large effect QTLs' might generally be too rare to be detected by association mapping [5],[17],[24]. The MOT1 Ler-0 allele provides a clear counter-example, demonstrating that, given the dense marker maps that are now obtainable, association mapping will at least sometimes be a useful tool for finding such loci. While this paper was in review, Tomatsu et al. [25] also reported that MOT1 is the locus responsible for low Mo in Ler. However, they did not confirm this directly by complementation. Here we conclude that MOT1 is the locus responsible for low Mo in Ler-0 and Van-0 based on genetic complementation, and further show that a deletion in the 5′ UTR of MOT1 is strongly associated with low Mo in 92 different Arabidopsis accessions. The sequence for the MOT1 Ler locus reported by Tomatsu et al. [25], derived from the Cereon resequencing project [7], differs from the results presented here by two additional amino acid altering SNPs. The MOT1 Ler sequence presented here is based on resequencing after PCR amplification, and is consistent with that published by Clark et al. [26]. Furthermore, here we conclude that MOT1 is localized to the mitochondria. This is in contrast to Tomatsu et al. [25], who suggest that MOT1 is localized to the plasma membrane and the secretory and/or endocytic pathways. We attribute these inconsistencies to differences in constructs and localization systems used in the two studies. To determine the localization of MOT1 Tomatsu et al. [25] reported that they prepared a construct in which GFP was fused to the N-terminus of MOT1, blocking the predicted mitochondrial localization signal, and likely mislocalizing the GFP::MOT1 fusion protein in the tobacco BY-2 cells used for transient expression. Results reported here were obtained using a C-terminally fused MOT1::GFP construct that was expressed both transiently and stably in Arabidopsis and that clearly localized to the mitochondria. In summary, natural variation has been used here to identify a mitochondrially localized Mo transporter that controls both root and shoot Mo content in Arabidopsis. This discovery demonstrates that natural accessions of Arabidopsis are a rich source of interesting alleles, useful for the functional characterization of genes of unknown function. Furthermore, the identification of MOT1 as a regulator of total plant Mo accumulation provides molecular insight into plant Mo homoeostasis. Note added in proof: While this paper was in review, Tejada-Jimenez et al. [27] published the identification and characterization of the MOT1 ortholog in Chlamydomonas reinhardtii. Materials and Methods Plant Materials All accessions were obtained from the ABRC or Lehle seeds. The insertion of the T-DNA into the MOT1 coding region in mot1-1 and into the ST5.1 coding region in st5.1-1 were verified by sequencing, and the mutant was confirmed to be null for MOT1 expression by RT-PCR (Figure S2). All T-DNA lines analyzed were homozygous for the T-DNA insertion. General Plant Growth Conditions Plants used for elemental profiling by ICP-MS analysis were grown in a controlled environment, 8 h light:16 h dark (90 µmol·m−2·s−1 light intensity) and 19 to 22°C [6]. Briefly, seeds were sown onto moist soil (Sunshine Mix LB2; Carl Brehob & Son, Indianapolis, Indiana, United States) with various elements added at subtoxic concentrations [As, Cd, Co, Li, Ni, Pb, and Se [6]] and stratified at 4°C for 3 d. Plants were bottom-watered twice per week with 0.25× Hoagland solution in which iron was replaced with 10 µM Fe-HBED [N,N′-di(2-hydroxybenzyl)ethylenediamine-N,N′-diacetic acid monohydrochloride hydrate; Strem Chemicals, Inc., http://www.strem.com). For elemental analysis after 5-weeks, plants were nondestructively sampled by removing one or two leaves. The plant material was rinsed with 18 MΩ water and placed into Pyrex digestion tubes. To alter the concentration of Mo in the watering solution, 0.25× Hoagland solution was made without any MoO4 2− which was then added back in varying concentrations from a solution of dissolved MoO3. Hydroponic Growth of Arabidopsis At Purdue University seeds of Col-0 and Ler-0 were germinated in the dark at 4°C for 2 days on 0.5× Murashige and Skoog media with 0.5× MS Vitamins (Caisson Laboratories, Inc.), 3 mg/L Benomyl [methyl 1-(butylcarbamoyl)-2-benzimidazolecarbamate; Sigma, http://www.sigmaaldrich.com), and 10 µM Fe-HBED solidified with 1.5% agar in 1.5 ml eppendorf microcentrifuge tubes before being transferred into growth conditions described above. For the first 5 days after germinationthe tubes containing the seedlings were kept covered to maintain high humidity. The bottom of each tube was then removed and the tube inserted into foam floats placed in tubs containing ∼4 L of 0.25× Hoaglands solution with 10 µM Fe-HBED. The solution was changed weekly until harvest at 4 weeks from planting. Leaves were harvested as described above. The roots were rinsed twice in distilled water and a third time in double distilled water before being put in Pyrex digestion tubes. At Rothamsted seeds of Col-0, mot1-1 and st5.1mot1-1 were germinated on 0.5% agarose in 0.5 ml tubes (with excised lower portion) in racks placed on boxes (with transparent lids) filled with 700 ml nutrient solution: 1.0 mM KNO3, 0.5 mM Ca(NO3)2, 1.0 mM KH2PO4, 1.0 mM MgSO4, 100 µM FeEDTA, 30 µM H3BO3, 5 µM MnCl2, 1 µM ZnCl, 1 µM CuCl and 0.1 µM Na2MoO4. To synchronize germination, the boxes were incubated at 4°C over night and then transferred to a controlled growth room under light/dark cycle 16/8h at 20°C. The nutrition solution was exchanged 2 times per week. After 3 weeks, shoot and root materials were harvested. Roots were washed twice by dipping in deionised water and dried on paper towels before freezing in liquid nitrogen. Tissue Elemental Analysis At Purdue University tissue samples were dried at 92°C for 20 h in Pyrex tubes (16×100 mm) to yield approximately 2–4 mg of tissue for elemental analysis. After cooling, seven of approximately 100 samples from each sample set were weighed. All samples were digested with 0.7 ml of concentrated nitric acid (OmniTrace; VWR Scientific Products; http://www.vwr.com), and diluted to 6.0 ml with 18 MΩ water. Elemental analysis was performed with an ICP-MS (Elan DRCe; PerkinElmer, http://www.perkinelmer.com) for Li, B, Na, Mg, P, S,K, Ca, Mn, Fe, Co, Ni, Cu, Zn, As, Se, Mo, and Cd. All samples were normalized to calculated weights, as determined with an iterative algorithm using the best-measured elements, the weights of the seven weighed samples, and the solution concentrations, implemented in the PiiMS database [4]. Alternatively, for the data shown in Figure 2B, samples were analyzed at Rothamsted. Frozen plant material was homogenized with a mortar and pestle in liquid nitrogen. After transfer into 2 ml tubes, the plant material was freeze-dried. Samples were acid digested (83% HNO3 & 13% (70%) HClO4) and analyzed by ICP-MS (Agilent ICP-MS 7500ce, Agilent Technologies, Santa Clara, CA, US) [28]. Heritability and Association Analysis Broad sense heritability was calculated using a general ANOVA to account for line and growth tray variation. A linear mixed model adjusting population structure confounding effects as in [14],[29] was used to test the marker-trait associations. A brief summary of the model is given below, where y is the vector of phenotype, α is the vector of fixed allele effects, β is the vector of subpopulation effects, u is the vector of random effects reflecting the genome-wide relatedness, and X, Q, Z are known incidence matrices relating the observations to fixed and random effects, respectively. The variance of phenotype was modeled as Thus, the phenotypic variance can be partitioned into two parts: σ2 g, the genetic variance attributable to genome-wide effects, and σ2 e, the residual variance. The Q and K* matrix was the same as in [14], with Q being the population assignments by Structure [30] and K* being the kinship coefficient matrix, estimated as the proportion of shared haplotypes between individual pairs. DNA Microarray-Based BSA DNA microarray-based BSA was realized as previously described [11],[31]. Briefly, SFPs were identified between Col-0 and Ler-0 by hybridizing labeled genomics DNA from each one of the accessions to Affymetrix ATH1 microarrays and comparing them to Col-0 hybridizations downloaded from http://www.naturalvariation.org/xam. Two genomic DNA pools from an F2 population of a cross between Ler-0 and the 14501 mutant in the Col-0 background were created and hybridized to separate DNA microarrays. Each one of the pools contained plants with either shoot Mo contents similar to Col-0 (“control” pool) or low shoot Mo contents similar to Ler (“Low Mo” pool). At loci unlinked to the low Mo phenotype, the pools should have equivalent amounts of each genotype, and the hybridization signal at each SFP should be intermediate between the two parent accessions, for an average difference between the two DNA microarrays of zero. At linked loci, the difference between the two DNA pools should be approximately two-thirds the difference between the parent accessions. By smoothing the signal across multiple SFPs, noise is reduced and the peak of the differences in hybridization signal will correspond to the chromosomal region of the loci controlling the low Mo trait. Raw hybridization data (.CEL files) for each probe on the ATH1 DNA microarrays used in these experiments have been submitted to the Gene Expression Omnibus (http://www.ncbi.nlm.nih.gov/geo) for public distribution (Reference #GSE10039). Grafting of Arabidopsis Seedlings to be grafted as previously described by [10]. Plants were harvested for analysis of shoot Mo content 4 weeks after transfer to soil. Postharvest analysis of graft unions was performed under the stereoscope to identify any adventitious root formation from grafted individuals. Individuals with adventitious roots emerging at or above the graft union or without a clear graft union were eliminated from subsequent analyses. Quantitative Real-Time PCR Plants were first analyzed by ICP-MS and further used to determine MOT1 transcript levels as described previously by Rus et al., [10]. For MOT1 (At2g25680) transcript quantification the following primers were used: forward primer 5′-GGT GGG TGT GTG GCA CTG T-3′ and reverse primer 5′-AGC ACA CCA ACC GGA AAC TT-3′. Four reactions were done per biological sample and three independent replicate samples per genotype were used. to evaluate the transcript abundance of MOT1. Data was analyzed using the SDS software (Applied Biosystems version 1.0), following the method of [32]. Ct values were determined based on efficiency of amplification. The mean Ct values were normalized against the corresponding ACTIN 1 gene (At2g37620) and Ct values calculated as (Ct AtMOT1 - Ct Actin1 ). The expression of MOT1 was calculated as the 2−ΔCt method. The final standard error was estimated by evaluating the 2−ΔCt term using 2−ΔCt plus standard deviation and 2−ΔCt minus the standard deviation [32]. Cloning and Sequencing of MOT1 Genomic DNA Genomic DNA was isolated from 10-day-old Arabidopsis Col-0 seedlings using a DNeasy plant mini kit (Qiagen, Valencia, CA). MOT1 clones containing approximately 1 kb upstream to the ORF, and approximately 0.250 kb downstream to the ORF were sequenced. The following primers were used to amplify different PCR products spanning the selected genomic region . Forward primers were: FP1 5′-CGA GCA AAC TAG AAA AGA GAT CG-3′, FP2 5′-CAG GTG TTA GCT GTT TAA CTG-3′, FP3-5′-GCG ATT TCG TCT ACC GC-3′ and FP4 5′-GGT TTG GAG CAA TGC C-3′. The corresponding reverse primers were: RP1 5′-CAA AAA CCA AAG CGT TGA CA-3′, RP2 5′-GGA CAC CGT AAA CTG C-3′ and RP3 5′-GGG AAG ATG TAG GTG G-3′. Conditions used in all PCR reactions were: initial denaturation 94°C followed by 30 cycles of 94° C 30 sec, 50° C 40 sec, 72° C 1 min 30 sec and final extension at 72° C for 10 min. All PCR products were cloned using TOPO XL PCR cloning kit (Invitrogen Corporation, Carlsbad, CA), and sequenced using Big dye terminator v 3.0 method (Applied Biosystems Foster city, CA) with T7 and universal M13 primers. Cloning of MOT1 cDNA The MOT1 cDNA was isolated by RT-PCR. Oligonucleotide primers MOT1-5′ (5′-ATG GAG TCT CAG TCT CAG AGA GGT CAA-3′) and MOT1-3′ (5′-TCA AGC ATG TTC ACC GGA TTG CGG GGG-3′) were designed to amplify the coding sequence. Total RNA was extracted from roots of 4-week-old Arabidopsis plants grown on solidified one-half Murashige and Skoog + B5 vitamin medium using RNeasy Plant Mini Kit (Qiagen, Hilden, Germany). Reverse transcription was carried out at 50°C in 20 ul solution containing 1 ug total RNA, 0.5 ug oligo (dT) primer, 10 nmol dNTPs and 200 units Superscript II reverse transcriptase (Gibco BRL, Rockville, MD, USA). PCR was carried out on the first-strand cDNA using Ex Taq DNA polymerase (Takara) following the manufacturer's protocols. After a standard PCR of 30 cycles, aliquots were run on an agarose gel. The fragment of putative size was cloned into a pGEM-T Easy vector (Promega) and identified by DNA sequencing. For yeast expression studies, the MOT1 cDNA insert from pGEM-T Easy vector (Promega) was amplified using PCR with the primers (5′-CGG ACT AGT CCA TGG AGT CTC AGT CTC AGA GAG GT-3′) and (5′-TCC GGA TCC TCA AGC GTA ATC AGG AAC ATC GTA AGG GTA AGC ATG TTC ACC GGA TTG CGG GGG-3′), with an HA tag encoded by the reverse promoter. The fragments were cloned into p416 GPD (-uracil (ura)) (ATCC nos. 87360). Two separate MOT1::GFP fusion protein constructs were cloned, one at Purdue (v1) and one at Rothamsted (v2). To construct the MOT1::GFP(v1) fusion protein, MOT1 was amplified from cDNA using PCR with 5′-TGC TCT AGA GCA TGG AGT CTC AGT CTC AGA GAG GT-3′ (MOT1, 5′ primer) and 5′-TCC GGA TCC TTC CTC CTC CAG CAT GTT CAC CGG ATT GCG GGG G-3′ (MOT1, 5′ primer) primers. The PCR product was confirmed by sequencing and cloned into the XbaI and BamHI sites of the 326-SGFP plasmid (kindly provide by Inhwan Hwang, POSTECH, Korea) to created chimeric GFP fusion constructs under the control of the 35S promoter. MOT1-Promoter-GUS and 35S-Promoter- MOT1::GFP (v2) Fusion Constructs The use of the two specific oligonucleotide primers 5′-GGA TCC GCA GTC GAG CTT ACC AAT TCT C-3′ and 5′-GGA TCC GAA ACA GAG CAA TAA GCG TAT CTC-3′ allowed isolation of a 1778 bp MOT1-promoter DNA fragment (−1801 to −21 from the translation start site) from Arabidopsis Col-0 genomic DNA by PCR. After subcloning in pGEM-Teasy (Promega) and sequencing, the BamHI restriction sites in the primer sequences were used for further cloning of the promoter DNA fragment into the BamHI site of the pBI101 vector (Clontech, Mountain View, USA) harboring the promoterless β-glucuronidase gene. For preparation of the MOT1::GFP(v2) construct the full ORF without the stop codon (TGA) was amplified from total cDNA by using the two specific oligonucleotide primers 5′-GGA TCC AAT GGA GTC TCA GTC TCA GAG AG-3′ and 5′-GGA TCC AGC ATG TTC ACC GGA TTG CGG GG-3′. The Bam HI restriction site replacing the stop codon allowed the cloning of the coding DNA in frame to the GFP gene in the binary vector pBIN19 [33], which contained the cauliflower mosaic virus 35S-promoter-MCS-GFP cassette. The binary plasmids were transformed into Agrobacterium tumefaciens GV3101 (pM P90) [34] by the freeze/thaw method. Arabidopsis Col-0 plants were transformed using the floral dip method (Clough and Bent, 1998). Transgenic plants were selected on solidified ½ MS media [35] containing 50 mg/l kanamycin sulphate. Kanamycin-resistant homozygous T3 progenies derived from 5 independent transgenic lines were used for analysis. Cloning ST5.1 cDNA Total RNA and first strand cDNA was isolated from Col-0 seedlings as described for qRT-PCR. The first strand cDNA was used as a template to synthesize ST 5.1 cDNA using the following primers: SpeI-FP 5′-CGA CTA GTA TGG CGG TCG CAA TAT CTG GGA GT-3′ BamHI-HA-3′RP 5′-CGG GAT CCT TAA GCG TAA TCC GGA ACA TCA TAC GGG TAG TTT GCG AGT ATC GGG TT3′. The reverse primer contained the HA tag. PCR conditions are as follows: initial denaturation 94°C followed by 30 cycles of 94° C 30 sec, 50° C 40 sec, 72° C 1 min 20 sec and final extension at 72° C for 10 min. PCR products were cloned and sequenced as before. Plasmid DNA containing ST5.1 HA were digested with SpeI and BamHI and the cDNA fragment cloned into p416 GPD (Glycerol 3-phosphate dehydrogenase promoter) using the same restriction enzymes. The ligated products were chemically transformed into E. coli DH5α and the positive clones were identified using a vector primer (FP-5′-AAT GGA GTG ATG CAA CCT-3′) and the reverse primer BamHI-HA-3′RP HA. Histochemical Staining of MOT1 Promoter-GUS Plants Transgenic Arabidopsis Col-0 plants were germinated and grown vertically on 0.5× MS agar plates containing 1% sucrose. Plants were transferred to 5 cm Petri dishes containing 2–4 ml staining solution, containing 0.05% 5-bromo 4 chloro 3 indolyl β-D glucuronic acid in 0.1 M sodium phosphate, 10 mM EDTA, 0.5 mM potassium ferricyanide, 0.5 mM potassium ferrocyanide, 0.3% triton X-100 and 10% methanol (pH 7.5). Vacuum infiltration for 1 min was performed twice and the staining reaction allowed to proceed in the dark at 37°C until the blue indigo color appeared. After straining plant samples were rinsed twice in 70% ethanol for 30 min then in 100% ethanol until chlorophyll was removed. After staining and destaining samples were analysed by optical microscopy. Subcellular Localization of MOT1 in Arabidopsis The MOT1::GFP(v1) construct and a mitochondria marker, F1-ATPase-γ-RFP [36], were co-transformed into purified Arabidopsis leaf protoplasts using polyethyleneglycol method [37]. The protoplasts were incubated for 20 hours at 22°C, and examined under an epi-fluorescence microscope, Nikon Eclipse 80i (Nikon USA, Melville, NY). Images of the mitochondria marker and the green fluorescence of MOT1::GFP were sequentially taken within 1 second in the same cell, because plant mitochondria actively moves along F-actins [38]. The filter sets used were 31303 for RFP and 31001 for GFP from Chroma Technol Corp (Rockingham, VT). The plants containing stably transformed 35S-Promoter-MOT1::GFP (v2) fusion constructs described above were grown vertically on B5 plates under continuous light for two weeks. The seedlings were harvested, and incubated with 0.2 µM MitoTracker Red CM-H2X ROS (Invitrogen, Carlsbad, CA) for 10 min at room temperature, and examined using a confocal microscope, Nikon Eclipse 80i (Nikon USA, Melville, NY) using green HeNe laser line (543 nm) for the GFP and red HeNe laser line (633 nm) for MitoTracker. Functional Characterization of MOT1 in Yeast The MOT1-HA and ST5.1-HA containing plasmids were transferred into the Saccharomyces cerevisiae yeast wild-type strain BY4742 (MATα his3 leu2 lys2 ura3) by the lithium acetate method [39]. The transformants were selected on SD minimal media containing 20 g l−1 glucose or glactose and required amino acids. Yeast transformants were first pre-grown at 30°C and 320 rpm in four different culture tubes per construct for one day in SD URA- minimal media. Each independent culture was used to inoculate 8 wells of a 2 mL square deep well 96-well plate (600 µL per well defined minimal growth medium inoculated with 20 µL of yeast culture). The plate was covered with a breathable seal and incubated at 30°C with shaking at 400 rpm for 24 hr. An AcroPrep® 96 PVDF (Polyvinylidene fluoride) filter membrane (0.45 µm, 350 µL) micro well plate (Pall Life Sciences) was wetted by partially filling with methanol and filtered using a vacuum block. Wells were then filled with deionized water and similarly filtered. Yeast culture samples, grown in the 2 ml deep well 96-well plates, were transferred to the 96-well filter plates (200 µL/well) and the yeast growth media removed by filtration. The same amount of culture samples was concurrently transferred into Clear View® micro plate (Whatman) for optical density measurement with a Dynex Opsys MR plate reader. Yeast cells on the membrane were washed four times, respectively, with 1 µM EDTA, pH 8, and deionized water. 96-well filter plates were dried at 88°C for 2 h. Concentrated nitric acid (100 µL/well) was added, the plate covered with polypropylene lid, and placed in a preheated heating block set at 88°C for 35 min to digest the yeast cells. The digested samples were diluted with a gallium internal standard (5 ppb final concentration) and filtered into a 2-mL square deep well 96-well plate containing Triton X-100 (0.025%, 300 µL). The final dilution volume was 1.6 mL, giving an acid and Triton X-100 concentration of about 6.5% and 0.005%, respectively. The filtered culture medium, as well as the original medium, was diluted 50 times but otherwise the matrix prepared in the same manner as the samples. The samples and the media were analyzed on a Perkin Elmer Elan DRC-e ICP-MS coupled with Elemental Scientific SC-2 autosampler and Apex Q nebulizer sample introduction system, and the following analytes quantified: Na, Mg, P, S, K, Ca, Mn, Fe, Co, Ni, Cu, Zn, Mo and Cd. Solution concentrations for all yeast sampleswere normalized to the measured optical densities of the corresponding yeast culture. The amount of yeast was converted from OD to number of cells using the conversion factor of 1ml of 1 OD culture containing 3×107 cells. Accession Numbers The Arabidopsis Biological resource Center (ABRC) accessions used in this paper were CS22660, CS20, CS1965, CS1968, CS1971, CS1986,CS1925, CS1939,CS1975. Supporting Information Figure S1 The Cumulative Distribution of p-Values in Genome-Wide Scans for Shoot Mo Accumulation. The cumulative distribution function of (cdf) of p-values for Mo accumulation across the genome with (mixed model) and without (naïve) correcting for population structure. (0.07 MB TIF) Click here for additional data file. Figure S2 RT-PCR Amplification of the Full Length MOT1 cDNA in mot1-1 and Full Length ST5.1 cDNA in st5.1-1. Forward and reverse 20 bp primer were used that contained the ATG start codon and the TGA-stop codon. (0.04 MB TIF) Click here for additional data file. Text S1 Alignment of MOT1 from Col-0, Ler-0 and Van-0, including sequence 1kb upstream and 250bp downstream of the open reading frame. (0.05 MB DOC) Click here for additional data file. Text S2 Arabidopsis accessions used in the association mapping study. (0.03 MB DOC) Click here for additional data file. Text S3 Significant genotype vs shoot Mo associations. (0.02 MB DOC) Click here for additional data file.