CELLULOSE SYNTHASE-LIKE A2, a Glucomannan Synthase,Is Involved in Maintaining Adherent Mucilage Structure in Arabidopsis Seed

Mannans are hemicellulosic polysaccharides that are considered to have both structural and storage functions in the plant cell wall. However, it is not yet known how mannans function in Arabidopsis (Arabidopsis thaliana) seed mucilage. In this study, CELLULOSE SYNTHASE-LIKE A2 (CSLA2; At5g22740) expression was observed in several seed tissues, including the epidermal cells of developing seed coats. Disruption of CSLA2 resulted in thinner adherent mucilage halos, although the total amount of the adherent mucilage did not change compared with the wild type. This suggested that the adherent mucilage in the mutant was more compact compared with that of the wild type. In accordance with the role of CSLA2 in glucomannan synthesis, csla2-1 mucilage contained 30% less mannosyl and glucosyl content than did the wild type. No appreciable changes in the composition, structure, or macromolecular properties were observed for nonmannan polysaccharides in mutant mucilage. Biochemical analysis revealed that cellulose crystallinity was substantially reduced in csla2-1 mucilage; this was supported by the removal of most mucilage cellulose through treatment of csla2-1 seeds with endo-β-glucanase. Mutation in CSLA2 also resulted in altered spatial distribution of cellulose and an absence of birefringent cellulose microfibrils within the adherent mucilage. As with the observed changes in crystalline cellulose, the spatial distribution of pectin was also modified in csla2-1 mucilage. Taken together, our results demonstrate that glucomannans synthesized by CSLA2 are involved in modulating the structure of adherent mucilage, potentially through altering cellulose organization and crystallization.Mannan polysaccharides are a complex set of hemicellulosic cell wall polymers that are considered to have both structural and storage functions. Based on the particular chemical composition of the backbone and the side chains, mannan polysaccharides are classified into four types: pure mannan, glucomannan, galactomannan, and galactoglucomannan (Moreira and Filho, 2008; Wang et al., 2012; Pauly et al., 2013). Each of these polysaccharides is composed of a β-1,4-linked backbone containing Man or a combination of Glc and Man residues. In addition, the mannan backbone can be substituted with side chains of α-1,6-linked Gal residues. Mannan polysaccharides have been proposed to cross link with cellulose and other hemicelluloses via hydrogen bonds (Fry, 1986; Iiyama et al., 1994; Obel et al., 2007; Scheller and Ulvskov, 2010). Furthermore, it has been reported that heteromannans with different levels of substitution can interact with cellulose in diverse ways (Whitney et al., 1998). Together, these observations indicate the complexity of mannan polysaccharides in the context of cell wall architecture.CELLULOSE SYNTHASE-LIKE A (CSLA) enzymes have been shown to have mannan synthase activity in vitro. These enzymes polymerize the β-1,4-linked backbone of mannans or glucomannans, depending on the substrates (GDP-Man and/or GDP-Glc) provided (Richmond and Somerville, 2000; Liepman et al., 2005, 2007; Pauly et al., 2013). In Arabidopsis (Arabidopsis thaliana), nine CSLA genes have been identified; different CSLAs are responsible for the synthesis of different mannan types (Liepman et al., 2005, 2007). CSLA7 has mannan synthase activity in vitro (Liepman et al., 2005) and has been shown to synthesize stem glucomannan in vivo (Goubet et al., 2009). Disrupting the CSLA7 gene results in defective pollen growth and embryo lethality phenotypes in Arabidopsis, indicating structural or signaling functions of mannan polysaccharides during plant embryo development (Goubet et al., 2003). A mutation in CSLA9 results in the inhibition of Agrobacterium tumefaciens-mediated root transformation in the rat4 mutant (Zhu et al., 2003). CSLA2, CSLA3, and CSLA9 are proposed to play nonredundant roles in the biosynthesis of stem glucomannans, although mutations in CSLA2, CSLA3, or CSLA9 have no effect on stem development or strength (Goubet et al., 2009). All of the Arabidopsis CSLA proteins have been shown to be involved in the biosynthesis of mannan polysaccharides in the plant cell wall (Liepman et al., 2005, 2007), although the precise physiological functions of only CSLA7 and CSLA9 have been conclusively demonstrated.In Arabidopsis, when mature dry seeds are hydrated, gel-like mucilage is extruded to envelop the entire seed. Ruthenium red staining of Arabidopsis seeds reveals two different mucilage layers, termed the nonadherent and the adherent mucilage layers (Western et al., 2000; Macquet et al., 2007a). The outer, nonadherent mucilage is loosely attached and can be easily extracted by shaking seeds in water. Compositional and linkage analyses suggest that this layer is almost exclusively composed of unbranched rhamnogalacturonan I (RG-I) (>80% to 90%), with small amounts of branched RG-I, arabinoxylan, and high methylesterified homogalacturonan (HG). By contrast, the inner, adherent mucilage layer is tightly attached to the seed and can only be removed by strong acid or base treatment, or by enzymatic digestion (Macquet et al., 2007a; Huang et al., 2011; Walker et al., 2011). As with the nonadherent layer, adherent mucilage is also mainly composed of unbranched RG-I, but with small numbers of arabinan and galactan ramifications (Penfield et al., 2001; Willats et al., 2001; Dean et al., 2007; Macquet et al., 2007a, 2007b; Arsovski et al., 2009; Haughn and Western, 2012). There are also minor amounts of pectic HG in the adherent mucilage, with high methylesterified HG in the external domain compared with the internal domain of the adherent layer (Willats et al., 2001; Macquet et al., 2007a; Rautengarten et al., 2008; Sullivan et al., 2011; Saez-Aguayo et al., 2013). In addition, the adherent mucilage contains cellulose (Blake et al., 2006; Macquet et al., 2007a), which is entangled with RG-I and is thought to anchor the pectin-rich mucilage onto seeds (Macquet et al., 2007a; Harpaz-Saad et al., 2011, 2012; Mendu et al., 2011; Sullivan et al., 2011). As such, Arabidopsis seed mucilage is considered to be a useful model for investigating the biosynthesis of cell wall polysaccharides and how this process is regulated in vivo (Haughn and Western, 2012).Screening for altered seed coat mucilage has led to the identification of several genes encoding enzymes that are involved in the biosynthesis or modification of mucilage components. RHAMNOSE SYNTHASE2/MUCILAGE-MODIFIED4 (MUM4) is responsible for the synthesis of UDP-l-Rha (Usadel et al., 2004; Western et al., 2004; Oka et al., 2007). The putative GALACTURONSYLTRANSFERASE11 can potentially synthesize mucilage RG-I or HG pectin from UDP-d-GalUA (Caffall et al., 2009). GALACTURONSYLTRANSFERASE-LIKE5 appears to function in the regulation of the final size of the mucilage RG-I (Kong et al., 2011, 2013). Mutant seeds defective in these genes display reduced thickness of the extruded mucilage layer compared with wild-type Arabidopsis seeds.RG-I deposited in the apoplast of seed coat epidermal cells appears to be synthesized in a branched form that is subsequently modified by enzymes in the apoplast. MUM2 encodes a β-galactosidase that removes Gal residues from RG-I side chains (Dean et al., 2007; Macquet et al., 2007b). β-XYLOSIDASE1 encodes an α-l-arabinfuranosidase that removes Ara residues from RG-I side chains (Arsovski et al., 2009). Disruptions of these genes lead to defective hydration properties and affect the extrusion of mucilage. Furthermore, correct methylesterification of mucilage HG is also required for mucilage extrusion. HG is secreted into the wall in a high methylesterified form that can then be enzymatically demethylesterified by pectin methylesterases (PMEs; Bosch and Hepler, 2005). PECTIN METHYLESTERASE INHIBITOR6 (PMEI6) inhibits PME activities (Saez-Aguayo et al., 2013). The subtilisin-like Ser protease (SBT1.7) can activate other PME inhibitors, but not PMEI6 (Rautengarten et al., 2008; Saez-Aguayo et al., 2013). Disruption of either PMEI6 or SBT1.7 results in the delay of mucilage release.Although cellulose is present at low levels in adherent mucilage, it plays an important adhesive role for the attachment of mucilage pectin to the seed coat epidermal cells. The orientation and amount of pectin associated with the cellulose network is largely determined by cellulose conformation properties (Macquet et al., 2007a; Haughn and Western, 2012). Previous studies have demonstrated that CELLULOSE SYNTHASE A5 (CESA5) is required for the production of seed mucilage cellulose and the adherent mucilage in the cesa5 mutant can be easily extracted with water (Harpaz-Saad et al., 2011, 2012; Mendu et al., 2011; Sullivan et al., 2011).Despite all of these discoveries, large gaps remain in the current knowledge of the biosynthesis and functions of mucilage polysaccharides in seed coats. In this study, we show that CSLA2 is involved in the biosynthesis of mucilage glucomannan. Furthermore, we show that CSLA2 functions in the maintenance of the normal structure of the adherent mucilage layer through modifying the mucilage cellulose ultrastructure.     

SALT-OVERLY SENSITIVE5 Mediates Arabidopsis Seed Coat Mucilage Adherence and Organization through Pectins

Interactions between cell wall polymers are critical for establishing cell wall integrity and cell-cell adhesion. Here, we exploit the Arabidopsis (Arabidopsis thaliana) seed coat mucilage system to examine cell wall polymer interactions. On hydration, seeds release an adherent mucilage layer strongly attached to the seed in addition to a nonadherent layer that can be removed by gentle agitation. Rhamnogalacturonan I (RG I) is the primary component of adherent mucilage, with homogalacturonan, cellulose, and xyloglucan constituting minor components. Adherent mucilage contains rays composed of cellulose and pectin that extend above the center of each epidermal cell. CELLULOSE SYNTHASE5 (CESA5) and the arabinogalactan protein SALT-OVERLY SENSITIVE5 (SOS5) are required for mucilage adherence through unknown mechanisms. SOS5 has been suggested to mediate adherence by influencing cellulose biosynthesis. We, therefore, investigated the relationship between SOS5 and CESA5. cesa5-1 seeds show reduced cellulose, RG I, and ray size in adherent mucilage. In contrast, sos5-2 seeds have wild-type levels of cellulose but completely lack adherent RG I and rays. Thus, relative to each other, cesa5-1 has a greater effect on cellulose, whereas sos5-2 mainly affects pectin. The double mutant cesa5-1 sos5-2 has a much more severe loss of mucilage adherence, suggesting that SOS5 and CESA5 function independently. Double-mutant analyses with mutations in MUCILAGE MODIFIED2 and FLYING SAUCER1 that reduce mucilage release through pectin modification suggest that only SOS5 influences pectin-mediated adherence. Together, these findings suggest that SOS5 mediates adherence through pectins and does so independently of but in concert with cellulose synthesized by CESA5.Cellulosic cell walls are a defining feature of land plants. Primary cell walls are composed of three major classes of polysaccharides: cellulose, hemicelluloses, and pectins. In addition, approximately 10% of the primary cell wall is composed of protein (Burton et al., 2010). Cell walls provide mechanical support for the cell, and cell wall carbohydrates in the middle lamellae mediate cell-cell adhesion (Caffall and Mohnen, 2009). Current models of cell wall structure depict a cellulose-hemicellulose network embedded in an independent pectin gel (for review, see Albersheim et al., 2011). These components are believed to interact through both covalent and noncovalent bonds to provide structure and strength to the cell wall, although the relative importance of pectin and its interactions with the hemicellulose-cellulose network remain unclear (for review, see Cosgrove, 2005).Another gap in our understanding of cell wall structure and assembly is the role of arabinogalactan proteins (AGPs). AGPs are a family of evolutionarily conserved secreted proteins highly glycosylated with type II arabinogalactans, and they can be localized to the plasma membrane by a C-terminal glycophosphatidylinositol (GPI) lipid anchor (for review, see Schultz et al., 2000; Showalter, 2001; Johnson et al., 2003; Seifert and Roberts, 2007; Ellis et al., 2010). AGPs can be extensively modified in the cell wall; many glycosyl hydrolases can affect AGP function by cleaving their glycosyl side chains (Sekimata et al., 1989; Cheung et al., 1995; Wu et al., 1995; Kotake et al., 2005). The GPI anchor can also be cleaved, releasing the AGPs from the membrane into the cell wall (Schultz et al., 2000). Although their exact roles are still unclear, AGPs have been proposed to interact with cell wall polysaccharides, initiate intracellular signaling cascades, and influence a wide variety of biological processes (for review, see Seifert and Roberts, 2007; Ellis et al., 2010; Tan et al., 2013).Many fasciclin-like AGPs (FLAs), which contain at least one fasciclin domain (FAS) associated with protein-protein interactions, have been suggested to influence cellulose biosynthesis or organization (Seifert and Roberts, 2007; Li et al., 2010; MacMillan et al., 2010). FLA3 RNA interference lines have reduced intine cell wall biosynthesis and loss of Calcofluor white (a fluorescent dye specific for glycan molecules) staining in aborted pollen grains (Li et al., 2010). A fla11 fla12 double mutant was shown to have reduced cellulose deposition, altered cellulose microfibril angle, and reduced cell wall integrity (MacMillan et al., 2010). The fla11 fla12 double mutant also had reductions in arabinans, galactans, and rhamnose (MacMillan et al., 2010). FLA4/SALT-OVERLY SENSITIVE5 (SOS5) was identified in a screen for salt sensitivity in roots. The SOS5 gene encodes an FLA protein with a GPI anchor, two AGP-like domains, and two FAS domains (Shi et al., 2003). Plants homozygous for the loss-of-function conditional allele sos5-1 have thinner root cell walls that appear less organized (Shi et al., 2003). The presence of the two FAS domains has led to the suggestion that SOS5 may interact with other proteins, forming a network that strengthens the cell wall (Shi et al., 2003). SOS5 is involved in regulation of cell wall rheology through a pathway involving two Leu-rich repeat receptor-like kinases, FEI1 and FEI2 (Xu et al., 2008). SOS5 and FEI2 are also required for normal seed coat mucilage adherence and hypothesized to do so by influencing cellulose biosynthesis (Harpaz-Saad et al., 2011, 2012).Arabidopsis (Arabidopsis thaliana) seed coat mucilage is a powerful model for studying cell wall biosynthesis and polysaccharide interactions (Arsovski et al., 2010; Haughn and Western, 2012). Seed coat epidermal cells sequentially produce two distinct types of secondary cell walls with unique morphologies and properties (Western et al., 2000; Windsor et al., 2000). Between approximately 5 and 9 d approximate time of fertilization (DPA), seed coat epidermal cells synthesize mucilage and deposit it in the apoplast, creating a donut-shaped mucilage pocket that surrounds a central cytoplasmic column (Western et al., 2000, 2004; Haughn and Chaudhury, 2005). From 9 to 13 DPA, the cytoplasmic column is gradually replaced by a cellulose-rich, volcano-shaped secondary cell wall called the columella (Beeckman et al., 2000; Western et al., 2000; Windsor et al., 2000; Stork et al., 2010; Mendu et al., 2011).Seed mucilage is composed primarily of relatively unbranched rhamnogalacturonan I (RG I) with minor amounts of homogalacturonan (HG), cellulose, and hemicelluloses (for review, see Haughn and Western, 2012). When mucilage is hydrated, it expands rapidly from the apoplastic pocket, forming a halo that surrounds the seed. Mucilage separates into two fractions: a loose nonadherent fraction and an inner adherent fraction that can only be released by vigorous shaking, strong bases, or glycosidases (for review, see North et al., 2014). Galactans and arabinans are also present in mucilage, and their regulation by glycosidases is required for correct mucilage hydration (Dean et al., 2007; Macquet et al., 2007b; Arsovski et al., 2009). For example, β-XYLOSIDASE1 encodes a bifunctional β-d-xylosidase/α-l-arabinofuranosidase required for arabinan modification in mucilage, and β-xylosidase1 mutant seeds have a delayed mucilage release phenotype (Arsovski et al., 2009). MUCILAGE MODIFIED2 (MUM2) encodes a β-d-galactosidase, and mum2 seeds fail to release mucilage when hydrated in water (Dean et al., 2007; Macquet et al., 2007b). MUM2 is believed to modify RG I galactan side chains but may also affect the galactan component of other mucilage components (Dean et al., 2007; Macquet et al., 2007b). Galactans are capable of binding to cellulose in vitro and could affect mucilage hydration through pectin-cellulose interactions (Zykwinska et al., 2005, 2007a, 2007b; Dick-Pérez et al., 2011; Wang et al., 2012), although carbohydrate linkage analysis suggests that the galactan side chains are very short.Several studies indicate that seed mucilage extrusion and expansion are also influenced by methylesterification of HG. For example, both SUBTILISIN-LIKE SER PROTEASE1.7 and PECTIN METHYLESTERASE INHIBITOR6 are required for proper methyl esterification of mucilage (Rautengarten et al., 2008; Saez-Aguayo et al., 2013). Mutations in another gene, FLYING SAUCER1 (FLY1; a transmembrane E3 ubiquitin ligase), reduce the degree of pectin methylesterification in mucilage and cause increased mucilage adherence and defective mucilage extrusion (Voiniciuc et al., 2013). fly1 seeds have disc-like structures at the edge of the mucilage halo, which are outer primary cell wall fragments that detach from the columella during extrusion and are difficult to separate from the adherent mucilage (Voiniciuc et al., 2013).Recently, CELLULOSE SYNTHASE5 (CESA5) and SOS5 were proposed to facilitate cellulose-mediated mucilage adherence (Harpaz-Saad et al., 2011; Mendu et al., 2011; Sullivan et al., 2011). A simple hypothesis for the role of CESA5 in mucilage adherence is that it synthesizes cellulose, which interacts with the mucilage pectin to mediate adherence. Loss of CESA5 function results in a reduction of mucilage cellulose biosynthesis and a less adherent mucilage cell wall matrix (Mendu et al., 2011; Sullivan et al., 2011). The role of SOS5 in mucilage adherence is more difficult to explain. SOS5 null mutations cause a loss-of-adherence phenotype similar to cesa5-1 seeds, suggesting that SOS5 may regulate mucilage adherence by influencing CESA5 function (Harpaz-Saad et al., 2011). However, the mechanism through which SOS5 could influence CESA5 and/or cellulose biosynthesis is not clear.To better understand the role of SOS5 in mucilage adherence and its relationship to CESA5, we thoroughly investigated the seed coat epidermal cell phenotypes of the cesa5-1 and sos5-2 single mutants as well as those of the cesa5-1 sos5-2 double mutant. We also investigated how cellulose, SOS5, and pectin interact to mediate mucilage adherence by constructing double mutants with either cesa5-1 or sos5-2 together with either mum2-1 or fly1. Our results suggest that SOS5 mediates mucilage adherence independently of CESA5. Furthermore, compared with CESA5, SOS5 has a greater influence on mucilage pectin structure, suggesting that SOS5 mediates mucilage adherence through pectins, not cellulose.     

Coexpressing Escherichia coli Cyclopropane Synthase with Sterculia foetida Lysophosphatidic Acid Acyltransferase Enhances Cyclopropane Fatty Acid Accumulation

Cyclopropane fatty acids (CPAs) are desirable as renewable chemical feedstocks for the production of paints, plastics, and lubricants. Toward our goal of creating a CPA-accumulating crop, we expressed nine higher plant cyclopropane synthase (CPS) enzymes in the seeds of fad2fae1 Arabidopsis (Arabidopsis thaliana) and observed accumulation of less than 1% CPA. Surprisingly, expression of the Escherichia coli CPS gene resulted in the accumulation of up to 9.1% CPA in the seed. Coexpression of a Sterculia foetida lysophosphatidic acid acyltransferase (SfLPAT) increases CPA accumulation up to 35% in individual T1 seeds. However, seeds with more than 9% CPA exhibit wrinkled seed morphology and reduced size and oil accumulation. Seeds with more than 11% CPA exhibit strongly decreased seed germination and establishment, and no seeds with CPA more than 15% germinated. That previous reports suggest that plant CPS prefers the stereospecific numbering (sn)-1 position whereas E. coli CPS acts on sn-2 of phospholipids prompted us to investigate the preferred positions of CPS on phosphatidylcholine (PC) and triacylglycerol. Unexpectedly, in planta, E. coli CPS acts primarily on the sn-1 position of PC; coexpression of SfLPAT results in the incorporation of CPA at the sn-2 position of lysophosphatidic acid. This enables a cycle that enriches CPA at both sn-1 and sn-2 positions of PC and results in increased accumulation of CPA. These data provide proof of principle that CPA can accumulate to high levels in transgenic seeds and sets the stage for the identification of factors that will facilitate the movement of CPA from PC into triacylglycerol to produce viable seeds with additional CPA accumulation.Modified fatty acids (mFAs; sometimes referred to as unusual fatty acids) obtained from plants play important roles in industrial applications as lubricants, protective coatings, plastics, inks, cosmetics, etc. The hundreds of potential industrial uses of mFAs have led to considerable interest in exploring their production in transgenic crop plants. mFAs are produced by a limited number of species, and the transfer of genes encoding mFA-producing enzymes from source plants to heterologous hosts has generally resulted in only modest accumulation, usually less than 20% of the desired mFA in transgenic seed (Napier, 2007) compared with levels found in the natural source. For example, ricinoleic acid accounts for more than 90% of the fatty acid of castor bean (Ricinus communis) seeds, and tung (Aleuites fordii) seeds accumulate more than 80% α-eleostearic acid (Thelen and Ohlrogge, 2002; Drexler et al., 2003). In order to elevate the content of mFAs in the engineered plants to that found in the native plant, it is necessary to (1) optimize the synthesis of mFA (Mekhedov et al., 2001), (2) minimize its degradation (Eccleston and Ohlrogge, 1998), and (3) optimize its incorporation into triacylglycerol (TAG; Bafor et al., 1990; Bates and Browse, 2011; van Erp et al., 2011).Cyclic fatty acids (CFAs) are desirable for numerous industrial applications. The strained bond angles of the carbocyclic ring contribute to their unique chemistry and physical properties, and hydrogenation of CFAs results in ring opening to produce methyl-branched fatty acids. Branched chain fatty acids are ideally suited for the oleochemical industry as feedstocks for the production of lubricants, plastics, paints, dyes, and coatings (Carlsson et al., 2011). Cyclopropane fatty acids (CPAs) have been found in certain gymnosperms, Malvales, Litchi spp., and other Sapindales species. They accumulate to as much as 40% in seeds of Litchi chinensis (Vickery, 1980; Gaydou et al., 1993). Sterculia foetida accumulates the desaturated CFA (i.e. cyclopropene fatty acid) to more than 60% of its seed oil (Bohannon and Kleiman, 1978; Pasha and Ahmad, 1992). The first step in its synthesis is the formation of the CPA by the cyclopropane synthase (CPS) enzyme, which transfers a methyl group to C9 of the oleoyl-phospholipid followed by cyclization to form the cyclopropane ring (Grogan and Cronan, 1997; Bao et al., 2002, 2003). None of the known natural sources of CPA are suitable for its commercial production. Therefore, it would be desirable to create an oilseed crop plant that accumulates high levels of CPA by heterologously expressing CPS in seeds. However, to date, heterologous expression of plant cyclopropane synthase genes has led to only approximately 1.0% CPA in the transgenic seeds (Yu et al., 2011).Two pathways for the biosynthesis of TAG exist in plants (Bates and Browse, 2012; Fig. 1). The de novo biosynthesis from glycerol-3-phosphate and acyl-CoA occurs via the Kennedy pathway and includes three acyltransferases: glycerol-2-phosphate acyltransferase, acyl-CoA:lysophosphatidic acid acyltransferase (LPAT), and acyl-CoA:diacylglycerol acyltransferase (DGAT; Kennedy, 1961). Alternatively, acyl-CoAs can be redirected from phosphatidylcholine (PC) via the action of a phospholipase C, choline phosphotransferase, phosphatidylcholine:diacylglycerol cholinephosphotransferase (PDCT; Hu et al., 2012; Lu et al., 2009), or phospholipid:diacylglycerol acyltransferase (PDAT; Dahlqvist et al., 2000). An acyl group can be released from PC to generate lysophosphatidylcholine (LPC) by the back reaction of acyl-CoA:LPC acyltransferase (Stymne and Stobart, 1984; Wang et al., 2012) or a phospholipase A/acyl-CoA synthase (Chen et al., 2011).Open in a separate windowFigure 1.Schematic representation of the plant TAG biosynthesis network. Acyl editing can provide PC-modified fatty acids for de novo diacylglycerol/TAG synthesis. ACS, acyl-CoA synthase; CPT, CDP-choline:diacylglycerol choline phosphotransferase; G3P, glycerol-3-phosphate; GPAT, acyl-CoA:glycerol-3-phosphate acyltransferase; LPC acyltransferase, acyl-CoA:LPC acyltransferase; mFAS, modified fatty acid synthase (in this work, mFAS is CPS); PAP, phosphatidic acid phosphatase; PLA, phospholipase A; PLC, phospholipase C.LPAT is a pivotal enzyme controlling the metabolic flow of lysophosphatidic acid (LPA) into different phosphatidic acids (PAs) in diverse tissues. Membrane-associated LPAT activities, identified in bacteria, yeast, plant, and animal cells, catalyze the transfer of acyl groups from acyl-CoA to LPA to synthesize PA. In plants and other organisms, LPAT activities have been identified in the endoplasmic reticulum (Kim et al., 2005), plasma membrane (Bursten et al., 1991), and mitochondria (Zborowski and Wojtczak, 1969). In higher plants, endoplasmic reticulum-localized LPAT plays an essential role transferring fatty acid from CoA esters to the sn-2 position of LPA in the synthesis of PA, a key intermediate in the biosynthesis of membrane phospholipids and storage lipids in developing seeds (Maisonneuve et al., 2010). LPAT from developing seeds of flax (Linum usitatissimum), rape (Brassica napus), and castor bean preferentially incorporate oleoyl-CoA, weakly incorporate cyclopropane acyl-CoA, and were unable to incorporate methyl-branched acyl-CoA when presented with an equimolar mix of these potential substrates (Nlandu Mputu et al., 2009). Thus, LPAT activity from agronomic plants constitutes a potential bottleneck for the incorporation of branched chain acyl-CoA into PA. In this work, we investigate the utility of an LPAT from a cyclopropanoid-syntheizing plant, S. foetida, with respect to its ability to enhance CPA accumulation. In our efforts to enhance CPA accumulation in transgenic plants, we screened CPS genes from diverse sources and identified Escherichia coli CPS (EcCPS) as an effective enzyme for the production of CPA in plants. However, EcCPS is reported to prefer the sn-2 position of E. coli phospholipid (Hildebrand and Law, 1964), and the data presented here show that its expression primarily leads to the accumulation of CPA at the stereospecific numbering (sn)-1 position. Moreover, coexpression of S. foetida lysophosphatidic acid acyltransferase (SfLPAT) results in the incorporation of CPA at the sn-2 position of LPA. Thus, coexpression of EcCPS and SfLPAT enables a cycle that enriches the accumulation of CPA at both sn-1 and sn-2 positions of PC and increases the accumulation of CPA. This work underscores the utility of coexpressing an acyltransferase from mFA-accumulating species with mFA-synthesizing enzymes to help mitigate bottlenecks in mFA TAG synthesis.     

Dynamic Changes in the Distribution of Minerals in Relation to Phytic Acid Accumulation during Rice Seed Development

Phytic acid (inositol hexakisphosphate [InsP₆]) is the storage compound of phosphorus in seeds. As phytic acid binds strongly to metallic cations, it also acts as a storage compound of metals. To understand the mechanisms underlying metal accumulation and localization in relation to phytic acid storage, we applied synchrotron-based x-ray microfluorescence imaging analysis to characterize the simultaneous subcellular distribution of some mineral elements (phosphorus, calcium, potassium, iron, zinc, and copper) in immature and mature rice (Oryza sativa) seeds. This fine-imaging method can reveal whether these elements colocalize. We also determined their accumulation patterns and the changes in phosphate and InsP₆ contents during seed development. While the InsP₆ content in the outer parts of seeds rapidly increased during seed development, the phosphate contents of both the outer and inner parts of seeds remained low. Phosphorus, calcium, potassium, and iron were most abundant in the aleurone layer, and they colocalized throughout seed development. Zinc was broadly distributed from the aleurone layer to the inner endosperm. Copper localized outside the aleurone layer and did not colocalize with phosphorus. From these results, we suggest that phosphorus translocated from source organs was immediately converted to InsP₆ and accumulated in aleurone layer cells and that calcium, potassium, and iron accumulated as phytic acid salt (phytate) in the aleurone layer, whereas zinc bound loosely to InsP₆ and accumulated not only in phytate but also in another storage form. Copper accumulated in the endosperm and may exhibit a storage form other than phytate.The transport of nutrients into developing seeds has received considerable attention. During the grain-filling stage, plants remobilize and transport nutrients distributed throughout the vegetative source organs into seeds. Plant seeds contain large amounts of phosphorus (P) in organic form, which supports growth during the early stages of seedling development. Most of the P in seeds is stored in the form of phytic acid (inositol hexakisphosphate [InsP₆]). Seeds also accumulate mineral nutrients such as potassium (K), magnesium (Mg), calcium (Ca), iron (Fe), zinc (Zn), copper (Cu), and manganese (Mn), which are used in seedling growth. Phytic acid acts as a strong chelator of metal cations and binds them to form phytate, a salt of InsP₆ (Lott et al., 2002; Raboy, 2009). During germination, phytate is decationized and hydrolyzed by phytases, and then inorganic phosphates, inositol, and various minerals are released from the phytate (Loewus and Murthy, 2000). Phytate accumulates within protein bodies, generally of vacuolar origin, in seed storage cells and is usually concentrated in spherical inclusions called globoids. Many studies of the elemental composition of phytate in seeds have been published. Energy-dispersive x-ray microanalyses of many plant species have revealed that, other than P, globoids contain mainly K and Mg as well as low levels of Ca, Mn, Fe, and Zn (Lott, 1984; Lott et al., 1995; Wada and Lott, 1997). This indicates that phytate is a mixed salt of these cations.Whether all storage metal elements can bind equally to InsP₆ is not known, although most elements are thought to exist in seeds in the form of phytate (Raboy, 2009). To form phytate, P and the other elements must be present in the same place. Therefore, determination of the precise locations of P and other elements in seed tissues makes it possible to judge whether an element exists in the form of phytate. Differences in metal distribution with P might suggest a storage form other than phytate. For determining distributions, synchrotron-based x-ray microfluorescence (µ-XRF) imaging utilizing an x-ray microbeam is a powerful tool. The microbeam excites the elements, thereby revealing the details of their spatial distribution. The development of focusing optics for high-energy x-rays using a Kirkpatrick-Baez mirror raises the imaging resolution of elements in µ-XRF analysis. A focal spot size smaller than 1 µm with x-ray energy as high as 100 keV enables detection of the subcellular distribution of elements in plant tissues (Fukuda et al., 2008; Takahashi et al., 2009).Whether there is an order in the affinity of elements for phytic acid in plant cells remains unknown. The stability of InsP₆-metal complexes has been estimated by in vitro titration (Maddaiah et al., 1964; Vohra et al., 1965; Persson et al., 1998). The binding strength of InsP₆ with metal is stronger for Zn and Cu than for Fe, Mn, and Ca. We also do not know if the mineral composition of phytate in seeds is determined by the relative abundance of these elements in the seed or by their biochemical characteristics. As a first step to address these issues, we examined the simultaneous changes in the distribution of P and metal elements during seed development using µ-XRF imaging analysis.Our objective in this study was to observe the dynamic changes in the distribution of some nutritionally important minerals (P, Ca, K, Fe, Zn, and Cu) in relation to the accumulation of phytic acid during rice (Oryza sativa) seed development.     

MAIGO5 Functions in Protein Export from Golgi-Associated Endoplasmic Reticulum Exit Sites in Arabidopsis

Plant cells face unique challenges to efficiently export cargo from the endoplasmic reticulum (ER) to mobile Golgi stacks. Coat protein complex II (COPII) components, which include two heterodimers of Secretory23/24 (Sec23/24) and Sec13/31, facilitate selective cargo export from the ER; however, little is known about the mechanisms that regulate their recruitment to the ER membrane, especially in plants. Here, we report a protein transport mutant of Arabidopsis thaliana, named maigo5 (mag5), which abnormally accumulates precursor forms of storage proteins in seeds. mag5-1 has a deletion in the putative ortholog of the Saccharomyces cerevisiae and Homo sapiens Sec16, which encodes a critical component of ER exit sites (ERESs). mag mutants developed abnormal structures (MAG bodies) within the ER and exhibited compromised ER export. A functional MAG5/SEC16A–green fluorescent protein fusion localized at Golgi-associated cup-shaped ERESs and cycled on and off these sites at a slower rate than the COPII coat. MAG5/SEC16A interacted with SEC13 and SEC31; however, in the absence of MAG5/SEC16A, recruitment of the COPII coat to ERESs was accelerated. Our results identify a key component of ER export in plants by demonstrating that MAG5/SEC16A is required for protein export at ERESs that are associated with mobile Golgi stacks, where it regulates COPII coat turnover.     

Salicylic Acid Regulates Arabidopsis Microbial Pattern Receptor Kinase Levels and Signaling

In Arabidopsis thaliana, responses to pathogen-associated molecular patterns (PAMPs) are mediated by cell surface pattern recognition receptors (PRRs) and include the accumulation of reactive oxygen species, callose deposition in the cell wall, and the generation of the signal molecule salicylic acid (SA). SA acts in a positive feedback loop with ACCELERATED CELL DEATH6 (ACD6), a membrane protein that contributes to immunity. This work shows that PRRs associate with and are part of the ACD6/SA feedback loop. ACD6 positively regulates the abundance of several PRRs and affects the responsiveness of plants to two PAMPs. SA accumulation also causes increased levels of PRRs and potentiates the responsiveness of plants to PAMPs. Finally, SA induces PRR- and ACD6-dependent signaling to induce callose deposition independent of the presence of PAMPs. This PAMP-independent effect of SA causes a transient reduction of PRRs and ACD6-dependent reduced responsiveness to PAMPs. Thus, SA has a dynamic effect on the regulation and function of PRRs. Within a few hours, SA signaling promotes defenses and downregulates PRRs, whereas later (within 24 to 48 h) SA signaling upregulates PRRs, and plants are rendered more responsive to PAMPs. These results implicate multiple modes of signaling for PRRs in response to PAMPs and SA.     

Unidirectional Movement of Cellulose Synthase Complexes in Arabidopsis Seed Coat Epidermal Cells Deposit Cellulose Involved in Mucilage Extrusion,Adherence, and Ray Formation

CELLULOSE SYNTHASE5 (CESA5) synthesizes cellulose necessary for seed mucilage adherence to seed coat epidermal cells of Arabidopsis (Arabidopsis thaliana). The involvement of additional CESA proteins in this process and details concerning the manner in which cellulose is deposited in the mucilage pocket are unknown. Here, we show that both CESA3 and CESA10 are highly expressed in this cell type at the time of mucilage synthesis and localize to the plasma membrane adjacent to the mucilage pocket. The isoxaben resistant1-1 and isoxaben resistant1-2 mutants affecting CESA3 show defects consistent with altered mucilage cellulose biosynthesis. CESA3 can interact with CESA5 in vitro, and green fluorescent protein-tagged CESA5, CESA3, and CESA10 proteins move in a linear, unidirectional fashion around the cytoplasmic column of the cell, parallel with the surface of the seed, in a pattern similar to that of cortical microtubules. Consistent with this movement, cytological evidence suggests that the mucilage is coiled around the columella and unwinds during mucilage extrusion to form a linear ray. Mutations in CESA5 and CESA3 affect the speed of mucilage extrusion and mucilage adherence. These findings imply that cellulose fibrils are synthesized in an ordered helical array around the columella, providing a distinct structure to the mucilage that is important for both mucilage extrusion and adherence.The epidermal cells of Arabidopsis (Arabidopsis thaliana) seed coats produce two distinct secondary cell walls: pectin-rich mucilage and cellulose-rich columellae (Western et al., 2000). When seeds are hydrated, mucilage expands rapidly, rupturing the outer tangential cell wall and forming a mucilage capsule that surrounds the seed. Seed coat mucilage is composed primarily of rhamnogalacturonan I (RG I) and also contains homogalacturonan (HG), hemicelluloses (such as xylans and glucomannans), and cellulose (for review, see Haughn and Western, 2012). Extruded mucilage consists of an outer, nonadherent fraction and an inner, adherent fraction (Western et al., 2000, 2001; Macquet et al., 2007a). The adherent and nonadherent mucilage layers differ in the amount of methylesterified HG (Rautengarten et al., 2008; Saez-Aguayo et al., 2013; Voiniciuc et al., 2013), galactans (Dean et al., 2007; Macquet et al., 2007b), arabinans (Arsovski et al., 2009), mannans (Yu et al., 2014), and cellulose (Harpaz-Saad et al., 2011; Mendu et al., 2011; Sullivan et al., 2011), all of which influence the physical properties of the layers.Adherent mucilage has a distinct structure, which can be examined using cell wall dyes and antibodies. When treated with cellulose-specific dyes, densely stained rays extend from the top of each columella to the outer edge of the adherent layer, many cell lengths above the seed surface (Mendu et al., 2011; Sullivan et al., 2011). Cytological evidence indicates that cellulose, pectins, and mannans are components of the ray (Haughn and Western, 2012; Griffiths et al., 2014; North et al., 2014; Yu et al., 2014), although the exact manner in which they are assembled is unknown.Cellulose is abundant in mucilage rays and mediates adherence. Loss-of-function mutations in CELLULOSE SYNTHASE5 (CESA5) result in reduced cellulose levels and increased detachment of mucilage from the seed (Harpaz-Saad et al., 2011; Mendu et al., 2011; Sullivan et al., 2011; Griffiths et al., 2014). How a reduction in cellulose results in a loss of adherence is still unknown, but it likely involves interaction with other mucilage components such as pectin and arabinogalactan proteins (Griffiths et al., 2014). Since cesa5 mutants still have some cellulose in the rays of the adherent mucilage halo (Mendu et al., 2011; Sullivan et al., 2011), additional cellulose synthases must be involved in mucilage cellulose biosynthesis.The Arabidopsis genome encodes 10 different CESAs (Delmer, 1999; Richmond and Somerville, 2000). Multiple lines of evidence suggest that three different CESAs are required to form one active cellulose synthase complex (CSC; for review, see Somerville, 2006). CSCs are membrane-bound protein complexes that synthesize cellulose microfibrils in the apoplast (for review, see Somerville, 2006; Endler and Persson, 2011; Lei et al., 2012). CESA1, CESA3, and CESA6 are considered the core components of the primary wall CSC (Desprez et al., 2007; Persson et al., 2007). CESA2, CESA5, and CESA9 are partially redundant to CESA6 in primary wall biosynthesis, and genetic evidence suggests that each of these CESA polypeptides can form a functional CSC with CESA3 and CESA1 (Desprez et al., 2007; Persson et al., 2007). CESA10 is expressed in young plants, stems, floral tissue, and the base of rosette leaves (Beeckman et al., 2002; Doblin et al., 2002), but its function in cellulose biosynthesis is unclear. Other cesa mutant lines have been examined for altered mucilage phenotypes (cesa1, radially swollen1 [Burn et al., 2002; Sullivan et al., 2011], cesa2, cesa6, and cesa9 [Mendu et al., 2011]; CESA3, je5 [Sullivan et al., 2011] and cesa10-1 [Sullivan et al., 2011]); to date, only CESA5 has been shown to be required for cellulose biosynthesis during mucilage deposition.Two mutant alleles of CESA3, isoxaben resistant1-1 (ixr1-1) and ixr1-2, were isolated in a screen for resistance to the herbicide isoxaben (Scheible et al., 2001). Isoxaben inhibits the incorporation of Glc into the emerging cellulose polymer and is considered a potent and specific inhibitor of cellulose biosynthesis (Heim et al., 1990). Homozygous ixr1-1 and ixr1-2 lines show increased resistance to the herbicide, and the mutations causing this resistance were mapped to the genomic locus of CESA3 (Heim et al., 1990; Scheible et al., 2001). The ixr1-1 and ixr1-2 mutations cause amino acid substitutions near the C terminus of the CESA3 protein. ixr1-1 causes a Gly-to-Asn substitution (G998A) located in a transmembrane domain, while ixr1-2 contains a Thr-to-Ile substitution (T942I) in an apoplastic region of the protein between two transmembrane domains (Scheible et al., 2001). Recently, the ixr1-2 allele was shown to affect the velocity of CSCs in the plasma membrane, which consequently modifies cellulose crystallinity in the cell wall (Harris et al., 2012). It is not exactly clear how the ixr1-1 mutation affects cellulose biosynthesis. The effects of either of these mutations on seed coat mucilage have not been investigated.Since mucilage is composed primarily of pectins with smaller amounts of cellulose, seed coat epidermal cells represent an excellent system to study cellulose biosynthesis and interactions between cellulose and other wall components in muro. In this study, we investigated how cellulose is synthesized and deposited in seed coat epidermal cells. We show that at least three different CESA proteins are highly expressed in the seed coat epidermis during mucilage biosynthesis. These CESAs are oriented and move in a linear fashion around the cytoplasmic column of each cell in an identical pattern to cortical microtubules. In addition, we provide evidence that the adherent mucilage has a helical structure that expands and unwinds during extrusion to form the mucilage ray. We propose that during seed coat epidermal cell development, the biosynthesis of cellulose predetermines the structure of rays in the adherent mucilage layer.     

Production of a Brassica napus Low-Molecular Mass Acyl-Coenzyme A-Binding Protein in Arabidopsis Alters the Acyl-Coenzyme A Pool and Acyl Composition of Oil in Seeds

Low-molecular mass (10 kD) cytosolic acyl-coenzyme A-binding protein (ACBP) has a substantial influence over fatty acid (FA) composition in oilseeds, possibly via an effect on the partitioning of acyl groups between elongation and desaturation pathways. Previously, we demonstrated that the expression of a Brassica napus ACBP (BnACBP) complementary DNA in the developing seeds of Arabidopsis (Arabidopsis thaliana) resulted in increased levels of polyunsaturated FAs at the expense of eicosenoic acid (20:1^cisΔ11) and saturated FAs in seed oil. In this study, we investigated whether alterations in the FA composition of seed oil at maturity were correlated with changes in the acyl-coenzyme A (CoA) pool in developing seeds of transgenic Arabidopsis expressing BnACBP. Our results indicated that both the acyl-CoA pool and seed oil of transgenic Arabidopsis lines expressing cytosolic BnACBP exhibited relative increases in linoleic acid (18:2^cisΔ9,12; 17.9%–44.4% and 7%–13.2%, respectively) and decreases in 20:1^cisΔ11 (38.7%–60.7% and 13.8%–16.3%, respectively). However, alterations in the FA composition of the acyl-CoA pool did not always correlate with those seen in the seed oil. In addition, we found that targeting of BnACBP to the endoplasmic reticulum resulted in FA compositional changes that were similar to those seen in lines expressing cytosolic BnACBP, with the most prominent exception being a relative reduction in α-linolenic acid (18:3^cisΔ9,12,15) in both the acyl-CoA pool and seed oil of the former (48.4%–48.9% and 5.3%–10.4%, respectively). Overall, these data support the role of ACBP in acyl trafficking in developing seeds and validate its use as a biotechnological tool for modifying the FA composition of seed oil.Cytosolic low-molecular mass (approximately 10 kD) acyl-coenzyme A-binding protein (ACBP) consists of a four-α-helix domain capable of binding acyl-CoAs with high affinity in a wide range of eukaryotic organisms (Faergeman et al., 2007). It is believed to serve a housekeeping function of maintaining free acyl-CoA concentrations at low nanomolar levels and, thus, prevents micelle formation and the partitioning of acyl-CoA into membranes (Knudsen et al., 1999). This protein is also considered to contribute to another facet of acyl-CoA pool maintenance via its role in the intracellular transport of acyl-CoAs in the aqueous environment of the cytosol (Rasmussen et al., 1994). Moreover, it has also been shown to exhibit more specialized functions in metabolic processes in which acyl-CoA is actively involved, depending on the tissue and physiological state (Guerrero et al., 2006; Xiao and Chye 2011; Yurchenko and Weselake, 2011).In the developing seeds of oleaginous plants, fatty acids (FAs) are synthesized de novo in plastids and are activated to acyl-CoAs upon their transfer to the cytosol, after which time they can undergo additional modifications (e.g. elongation and desaturation) on the membranes of the endoplasmic reticulum (ER; for review, see Rawsthorne, 2002). While FA elongation is performed on the acyl-CoA substrate, the introduction of the second and third double bonds requires the acyl group to be esterified to phosphatidylcholine (PC; Jaworski, 1987). The composition of the acyl-CoA pool, therefore, is highly dynamic and represents a net result of both de novo synthesis and acyl-editing processes (Bates et al., 2009).The acyl-CoA pool provides substrate for acyltransferases involved in the biosynthesis of triacylglycerol (TAG), which is a major component of seed oil (Weselake et al., 2009). More specifically, TAG synthesis typically occurs via a series of acyl-CoA-dependent acylations of a glycerol backbone derived from sn-glycerol-3-phosphate in a pathway known as the sn-glycerol-3-phosphate or Kennedy pathway (for review, see Snyder et al., 2009; Weselake et al., 2009), although acyl-CoA-independent reactions can also be involved in the production of TAG (Stobart et al., 1997; Banaś et al., 2000; Dahlqvist et al., 2000) and thus contribute to its final composition. Low-molecular mass ACBPs have been demonstrated to modulate the activities of Kennedy pathway acyltransferases in a manner dependent upon the ratio of ACBP to acyl-CoA, stimulating TAG biosynthesis under conditions of acyl-CoA excess and inhibiting acyltransferase activities when relative amounts of acyl-CoA are low compared with ACBP, thus regulating the size of the acyl-CoA pool (for review, see Yurchenko and Weselake, 2011).The acyl-CoA pool in seeds is also influenced through a distinct route involving lysophosphatidylcholine acyltransferase (LPCAT), which catalyzes the acyl-CoA-dependent acylation of lysophosphatidylcholine at the sn-2 position to form PC (Ichihara et al., 1995). Acyl groups esterified to PC become substrates for FA desaturation and other modifications (Miquel and Browse, 1992; Broun et al., 1998) and can then be returned back to the acyl-CoA pool or channeled into TAG through acyl-CoA-independent mechanisms (Stymne and Stobart, 1984; Weselake, 2005; Lager et al., 2013). The efficiency of this acyl group channeling to and from PC is an important determinant of the overall composition of FAs in the acyl-CoA pool and, subsequently, in seed oil.Previously, we demonstrated that the expression of the Brassica napus low-molecular mass ACBP (hereafter referred to as BnACBP) in the presence of Arabidopsis (Arabidopsis thaliana) LPCAT isoforms in an in vitro system enhanced the incorporation of oleic acid (18:1^cisΔ9; hereafter referred to as 18:1) into PC and the release of linoleic acid (18:2^cisΔ9,12; hereafter referred to as 18:2) from PC into acyl-CoA (Yurchenko et al., 2009). In line with these results, the expression of BnACBP complementary DNA (cDNA) in Arabidopsis developing seeds was also shown to result in elevated levels of the polyunsaturated fatty acids (PUFAs) 18:2 and α-linolenic acid (18:3^cisΔ9,12,15; hereafter referred to as 18:3) in seed oil, mainly at the expense of eicosenoic acid (20:1^cisΔ11; hereafter referred to as 20:1) and saturated fatty acids (SFAs; Yurchenko et al., 2009). Based on these findings, BnACBP was proposed to be involved in acyl exchange between acyl-CoA and PC pools, which may affect the rate of FA modifications and, ultimately, the FA composition of seed oil (Yurchenko et al., 2009).In this study, we endeavored to provide further evidence that low-molecular mass ACBP functions in acyl trafficking by investigating whether changes in the FA composition of TAG in Arabidopsis seeds expressing BnACBP were correlated with modifications in the composition of the acyl-CoA pool. In addition, since FA modifications such as elongation and desaturation as well as TAG synthesis occur on ER membranes, we also examined the effect of changing the subcellular localization of BnACBP (from the cytosol to the ER) on the acyl composition of TAG and the acyl-CoA pool in transgenic Arabidopsis. Consequently, we generated localized pools of acyl-CoAs that could be readily accessed by acyltransferases involved in seed oil biosynthesis. Taken together, our findings provide insight into the role of low-molecular mass ACBP in seed oil metabolism and suggest that ACBP (either in its native cytosolic form or as an ER-targeted fusion protein) may serve as a useful tool in biotechnological modifications of FA composition in oil crops.     

Bypassing Iron Storage in Endodermal Vacuoles Rescues the Iron Mobilization Defect in the natural resistance associated-macrophage protein3natural resistance associated-macrophage protein4 Double Mutant

To improve seed iron (Fe) content and bioavailability, it is crucial to decipher the mechanisms that control Fe storage during seed development. In Arabidopsis (Arabidopsis thaliana) seeds, most Fe is concentrated in insoluble precipitates, with phytate in the vacuoles of cells surrounding the vasculature of the embryo. NATURAL RESISTANCE ASSOCIATED-MACROPHAGE PROTEIN3 (AtNRAMP3) and AtNRAMP4 function redundantly in Fe retrieval from vacuoles during germination. When germinated under Fe-deficient conditions, development of the nramp3nramp4 double mutant is arrested as a consequence of impaired Fe mobilization. To identify novel genes involved in seed Fe homeostasis, we screened an ethyl methanesulfonate-mutagenized population of nramp3nramp4 seedlings for mutations suppressing their phenotypes on low Fe. Here, we report that, among the suppressors, two independent mutations in the VACUOLAR IRON TRANSPORTER1 (AtVIT1) gene caused the suppressor phenotype. The AtVIT1 transporter is involved in Fe influx into vacuoles of endodermal and bundle sheath cells. This result establishes a functional link between Fe loading in vacuoles by AtVIT1 and its remobilization by AtNRAMP3 and AtNRAMP4. Moreover, analysis of subcellular Fe localization indicates that simultaneous disruption of AtVIT1, AtNRAMP3, and AtNRAMP4 limits Fe accumulation in vacuolar globoids.Iron (Fe) is an essential micronutrient. In cells, this metal may change between two oxidation states: ferrous (Fe²⁺) and ferric (Fe³⁺). This property makes Fe an important metal cofactor for electron transfer in many biochemical reactions. However, for the same reason, free Fe generates harmful reactive oxygen species via the Fenton reaction (Haber and Weiss, 1932; Halliwell, 1978). Cells thus need to tightly control Fe homeostasis through chelation and compartmentalization. For example, in yeast (Saccharomyces cerevisiae), the membrane transporter yeast Calcium-sensitive Cross-Complementer1 (ScCCC1) is required to move excess Fe into the vacuole (Li et al., 2001). The Δccc1 mutant is sensitive to extracellular Fe. In mammalian cells, excess cytosolic Fe is complexed by ferritins; the assembly of 24 ferritin monomers forms a hollow complex able to safely store up to 4,500 Fe(III) atoms (Finazzi and Arosio, 2014).Fe deficiency is an important public health issue: 2 billion people, corresponding to over 25% of the world population, are anemic (World Health Organization, 2015). To fight Fe deficiency, it has been proposed to develop crops with more available Fe according to a strategy called biofortification (Bouis, 2003). In most crops, seeds are used as food or feed. Fe stores in seeds are also important for the germination of seedlings. In seeds, Fe may be associated with ferritin in plastids, with phytate in vacuoles, or with nicotianamine. Although Fe complexed with ferritin or nicotianamine is considered highly bioavailable, Fe phytate is insoluble and poorly bioavailable (Clemens, 2014).In Arabidopsis (Arabidopsis thaliana) seeds, no more than 5% of the total seed Fe is associated with ferritin (Ravet et al., 2009). About 50% of seed Fe is concentrated in the vacuoles of endodermal and bundle sheath cells surrounding the vasculature in the radicle and cotyledons of the embryo, respectively (Lanquar et al., 2005; Kim et al., 2006; Roschzttardtz et al., 2009; Schnell Ramos et al., 2013). As endodermal and bundle sheath cells belong to the same lineage, they will be collectively referred to as endodermal cells in this report. VACUOLAR IRON TRANSPORTER1 (AtVIT1) is responsible for the loading of Fe in endodermal vacuoles during seed development (Kim et al., 2006). VIT1 is homologous to CCC1, which mediates Fe sequestration in the vacuole in yeast (Li et al., 2001). In addition to VIT1, which is mostly expressed during seed development, the Arabidopsis genome encodes five VIT1-like proteins (VTLs). VTL gene expression is down-regulated under Fe deficiency (Gollhofer et al., 2011). At least one of the VTLs also functions in Fe sequestration in the vacuole (Gollhofer et al., 2014). VIT1 homologs have been identified in most plant species for which genome sequencing data are available. In rice (Oryza sativa), OsVIT1 and OsVIT2 sequester Fe and zinc in the vacuole of the flag leaf (Zhang et al., 2012). Loss of AtVIT1 function perturbs the cell type-specific localization of Fe in mature embryos. Accordingly, in the vit1-1 knockout mutant, Fe is no longer concentrated in cells surrounding the vasculature of the hypocotyl, radicle, and cotyledons but instead is accumulated in cortical cells in the hypocotyl and radicle and in the subepidermal cells of the abaxial side of cotyledons (Kim et al., 2006). Loss of AtVIT1 function also has an impact on germination on alkaline (pH 7.9) soil: vit1-1 mutant seedlings grow poorly compared with the wild type (Kim et al., 2006).NATURAL RESISTANCE ASSOCIATED-MACROPHAGE PROTEIN3 (AtNRAMP3) and AtNRAMP4 function redundantly in the mobilization of seed Fe from vacuoles during germination (Lanquar et al., 2005). They belong to a ubiquitous family of divalent cation transporters represented in all kingdoms of life. NRAMP proteins have well-documented roles in manganese (Mn) uptake in bacteria, yeast, and Arabidopsis (Nevo and Nelson, 2006; Cailliatte et al., 2010). In mammals, NRAMP2/Divalent Cation Transporter1/Divalent Metal Transporter1 is the major uptake system involved in dietary Fe absorption (Andrews, 2004). Recently, some members of this family have been shown to transport other substrates (Xia et al., 2010; Ishikawa et al., 2012; Shin et al., 2014). The Arabidopsis genome encodes six NRAMP homologs. AtNRAMP3 and AtNRAMP4 are targeted to the vacuole and play a role in essential metal remobilization from this organelle, not only during seed germination but also in adult plants (Lanquar et al., 2005, 2010). Even though Fe content and localization are unaffected in mature seeds of the nramp3nramp4 (nr3nr4) double knockout mutant (Schnell Ramos et al., 2013), seedlings of this mutant display strong defects when grown on an Fe-deficient medium: they are chlorotic and their development is arrested (Lanquar et al., 2005).When associated with phytate in vacuolar globoids, Fe is insoluble and notoriously poorly available for animal nutrition (Clemens, 2014). To identify mutations that limit Fe storage in this compartment, we generated an ethyl methanesulfonate (EMS)-mutagenized population of the nr3nr4 mutant and looked for mutations that restore growth on Fe-deficient medium. We called these mutants isv (for bypass iron storage in vacuoles).Here, we report the characterization of two isv mutants displaying Fe distribution patterns similar to the vit1-1 mutant. These mutants carry mutations in the AtVIT1 gene. By genetic analysis, we demonstrate that the mutations in AtVIT1 are loss-of-function alleles that are responsible for the suppression phenotype. The vit1-2 allele in isv1 carries an amino acid change in the AtVIT1 protein leading to a nonfunctional protein, and the vit1-3 allele in isv2 modifies the first intron-splicing consensus sequence leading to nonfunctional RNAs or proteins. Whereas NRAMP3 and NRAMP4 are necessary for retrieving Fe from vacuoles in the wild-type background, they are not necessary for using Fe in a VIT1 loss-of-function background. Actually, combining nramp3, nramp4, and vit1 mutations modifies Fe localization at the tissue and subcellular levels. These changes likely account for the ability of vit1 mutations to rescue Fe mobilization and growth in the nr3nr4 background.