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Golgi Localized Barley MTP8 Proteins Facilitate Mn Transport

  • Pai Pedas ,

    pp@plen.ku.dk

    Affiliation Plant and Soil Science Laboratory, Department of Plant and Environmental Sciences, Faculty of Science, University of Copenhagen, Copenhagen, Denmark

  • Michaela Schiller Stokholm,

    Affiliation Plant and Soil Science Laboratory, Department of Plant and Environmental Sciences, Faculty of Science, University of Copenhagen, Copenhagen, Denmark

  • Josefine Nymark Hegelund,

    Affiliation Plant and Soil Science Laboratory, Department of Plant and Environmental Sciences, Faculty of Science, University of Copenhagen, Copenhagen, Denmark

  • Anne Hald Ladegård,

    Affiliation Plant and Soil Science Laboratory, Department of Plant and Environmental Sciences, Faculty of Science, University of Copenhagen, Copenhagen, Denmark

  • Jan Kofod Schjoerring,

    Affiliation Plant and Soil Science Laboratory, Department of Plant and Environmental Sciences, Faculty of Science, University of Copenhagen, Copenhagen, Denmark

  • Søren Husted

    Affiliation Plant and Soil Science Laboratory, Department of Plant and Environmental Sciences, Faculty of Science, University of Copenhagen, Copenhagen, Denmark

Golgi Localized Barley MTP8 Proteins Facilitate Mn Transport

  • Pai Pedas, 
  • Michaela Schiller Stokholm, 
  • Josefine Nymark Hegelund, 
  • Anne Hald Ladegård, 
  • Jan Kofod Schjoerring, 
  • Søren Husted
PLOS
x

Abstract

Many metabolic processes in plants are regulated by manganese (Mn) but limited information is available on the molecular mechanisms controlling cellular Mn homeostasis. In this study, a yeast assay was used to isolate and characterize two genes, MTP8.1 and MTP8.2, which encode membrane-bound proteins belonging to the cation diffusion facilitator (CDF) family in the cereal species barley (Hordeum vulgare). Transient expression in onion epidermal cells showed that MTP8.1 and MTP8.2 proteins fused to the green fluorescent protein (GFP) are localized to Golgi. When heterologously expressed in yeast, MTP8.1 and MTP8.2 were found to be Mn transporters catalysing Mn efflux in a similar manner as the Golgi localized endogenous yeast protein Pmr1p. The level of MTP8.1 transcripts in barley roots increased with external Mn supply ranging from deficiency to toxicity, while MTP8.2 transcripts decreased under the same conditions, indicating non-overlapping functions for the two genes. In barley leaves, the expression of both MTP8 genes declined in response to toxic Mn additions to the roots suggesting a role in ensuring proper delivery of Mn to Golgi. Based on the above we suggest that barley MTP8 proteins are involved in Mn loading to the Golgi apparatus and play a role in Mn homeostasis by delivering Mn to Mn-dependent enzymes and/or by facilitating Mn efflux via secretory vesicles. This study highlights the importance of MTP transporters in Mn homeostasis and is the first report of Golgi localized Mn2+ transport proteins in a monocot plant species.

Introduction

Manganese is next to iron (Fe) the most prevalent transition metal in the earth's crust and can be found in potentially toxic concentrations in many environments. Despite the many important physiological functions of manganese (Mn) in the plant cell, the amount required for optimal growth is relatively low. However, the Mn2+ uptake capacity greatly exceeds this requirement [1], [2] and consequently an effective efflux system must exist to ensure homeostasis of Mn in plant tissue. The Mn2+ concentration in soil solution increases with decreasing soil pH and redox potential [3]. Mn toxicity is therefore a widespread phenomenon in acidic and waterlogged soils, constituting approximately 30% of the Earth's surface [4].

As an essential micronutrient, Mn has many functions in plant metabolism. In the cytosol, Mn activates the enzyme phenylalanine ammonia-lyase (PAL) of the shikimic pathway, leading to biosynthesis of various key metabolites e.g. the cell wall component lignin [5]. In peroxisomes and mitochondria, Mn acts as an inorganic cofactor of Mn superoxide dismutase (Mn-SOD), a protein responsible for scavenging of reactive oxygen species [6], [7]. Also, a number of glycosyl transferases localized in Golgi has been shown to have Mn-dependent activity. Some of these enzymes, such as arabinan arabinosyltransferase, xyloglucan glycosyltransferase, UDP-xylose glucuronyltransferase and arabinoxylan arabinosyltransferase, catalyse synthesis of cell wall polysaccharides [8]-[11]. Finally, Mn is also an unspecific activator of a number of different enzymes such as decarboxylases and dehydrogenases in the tricaboxylic acid cycle [3]. However, the most prominent role of Mn is its involvement in the oxygen evolving complex (OEC) of photosystem II (PSII). PSII is responsible for the photolytic dissociation of water, which releases molecular oxygen and protons while initiating the photosynthetic electron flow [12]. Due to its wide variety of essential functional properties, Mn deficiency leads to multiple visual symptoms in plants. Among these are interveinal chlorosis, necrotic spots, lower root biomass and slack leaves due to a reduction in the content of fructans and structural carbohydrates, resulting in an overall reduction in the yield potential of Mn-deficient plants [13]-[15].

Cellular Mn homeostasis in plants is regulated by processes involved in uptake, translocation, cellular sequestration and storage of Mn [16], [17]. Symplastic Mn transport is facilitated by several transport proteins. In Arabidopsis thaliana, the major player in Mn2+ uptake during conditions of Mn limitation appears to be the natural resistance-associated macrophage protein NRAMP1, which is a high-affinity Mn2+ transporter located in the root plasma membrane [18]. The nramp1 mutant has both reduced biomass production and a threefold reduction in Mn shoot concentrations when compared to wild type plants. As a result, the nramp1 mutant is sensitive towards Mn deficiency [18]. Also, the plasma membrane localized multi-specific ion transporter IRT1 from Arabidopsis has been shown to transport Mn2+ into the cell [19],[20], although the primary role of AtIRT1 is related to Fe2+/Fe3+ uptake, especially during Fe deficiency.

In the tonoplast, AtCAX2 belonging to the cation exchanger (CAX) family has the ability to transport Mn2+ into the vacuole. Expression studies in tobacco (Nicotiana tabacum) and yeast (Saccharomyces cerevisiae) have indicated a role for AtCAX2 in Mn2+ removal from the cytosol during excess Mn2+ conditions [21]-[24]. In seeds, the vacuolar iron transporter VIT1 from Arabidopsis is involved in storage of Mn and Fe, thus ensuring the availability of micronutrients during early growth of seedlings [25]. The third known vacuolar Mn2+ transporter, ShMTP1, has been identified in the Mn-tolerant tropical legume Stylosanthes hamata and is a member of the cation diffusion facilitator (CDF) transporter family. Heterologous expression of ShMTP8 in yeast or Arabidopsis results in increased Mn tolerance and higher cellular contents of Mn [26] (ShMTP1 has been renamed to ShMTP8 following the nomenclature for Mn-MTP proteins; [27]). Recently, the MTP8 homolog from rice has been isolated in a yeast Mn tolerance screen. OsMTP8 was found to be localized to the vacuole and it is suggested that OsMTP8 is important for Mn detoxification by sequestering Mn in the vacuole of rice plants [28]. Remobilization of vacuolar Mn in Arabidopsis is mediated by NRAMP3 and NRAMP4. In mesophyll cells, these proteins are likely to be involved in transport of Mn2+ from the vacuole to chloroplast, thus ensuring optimal OEC activity in PSII. However, neither NRAMP3 nor NRAMP4 seems to be involved in supplying vacuolar stored Mn2+ to the mitochondrial Mn superoxide dismutase [29], [30].

Transport of intracellular Mn2+ can also be mediated by P-type ATPases belonging to the subfamily P2A. The endoplasmic reticulum-type Ca2+-ATPase 1 (ECA1), from Arabidopsis transports Mn into ER [31]. The ECA1 homolog AtECA3 has been localized to Golgi and the growth of eca3 mutants was severely hampered under low Mn conditions indicating a crucial role under Mn limiting conditions [32]. However, an additional study has shown that AtECA3-GFP is associated with prevacuolar compartments and AtECA3 seems to be involved in detoxification of excess Mn2+ since eca3 mutants were sensitive to 50 µM Mn2+ [33]. Two additional genes, ECA2 and ECA4, are identified in the Arabidopsis genome [34], but are still not characterized. MTP11 from Arabidopsis was localized to the Golgi apparatus by Peiter et al [55] and they suggested that AtMTP11 is involved in Mn tolerance by loading Mn into secretory vesicles that allows Mn removal from the cell via exocytosis. A contrasting study localized AtMTP11 to the prevacuolar compartment indicating compartmentalization as the tolerance mechanism [35]. These findings indicate that AtMTP11 could be dynamically localized depending on the actual Mn status and cellular conditions of the plant tissue. Taken together, the studies conducted on Mn homeostasis show that Mn homeostasis is regulated by a highly dynamic series of transporters depending on the Mn status of the plant.

The majority of studies concerning Mn transport proteins have so far been obtained from dicotyledonous plants and solid experimental evidence regarding transport proteins controlling Mn2+ transport in monocotyledonous plants are lacking. In addition to OsMTP8, four plasma membrane localized transporters from monocot plant species have been identified. First, the IRT1 homologue from barley is a multi-substrate protein, which in addition to Mn also has the ability to transport Fe, Zn and Cd. Transcription of IRT1 is induced by Fe and Mn deficiency, where both deficiencies independently lead to an increased Mn uptake capacity of the root [36]. The second Mn transport protein from monocots is the yellow stripe-like protein 2 (YSL2) from rice. OsYSL2 mediates in vitro transport of both Mn(II)- and Fe(III)-nicotianamine. OsYLS2 expression is particularly pronounced in companion cells in roots, phloem cells of the vascular bundles in leaves and in developing seeds [37]. Based on the physiological performance of different rice lines with varying expression levels of OsYSL2, the encoded transporter has been suggested to operate in Fe and Mn translocation, especially to shoots and the endosperm of developing grains [38]. The YSL2 homologue OsYSL6 is involved in Mn translocation between the apoplast and symplast in leaves, a process which could affect the plants tolerance towards Mn toxicity [39]. Finally, in rice OsNRAMP3 is shown to regulate Mn shoot distribution depending on environmental conditions [40], [41]. The OsNRAMP3 protein is constitutively expressed except during Mn excess conditions, where it is internalized in vesicles and rapidly degraded. The vascular-bundle specific localization in nodes ensures that Mn follows the transpiration stream to the youngest leaves during low and moderate Mn conditions, whereas during Mn excess Mn is translocated to old leaves and thereby preventing Mn toxicity in the young shoot tissue.

In the present study we have used yeast as a tool to identify and characterize two novel barley genes, MTP8.1 and MTP8.2, encoding Mn2+ transport proteins. Root transcripts of MTP8.1 and MTP8.2 show contrasting responses towards external concentrations of Mn, suggesting that the two proteins are transcriptionally regulated depending on the Mn nutritional status of the plant. Both MTP8.1 and MTP8.2 proteins fused to the green fluorescent protein (GFP) were localized to Golgi. This is the first report of Golgi localized Mn2+ transport proteins that are involved in intracellular Mn homeostasis of a monocot plant species.

Materials and Methods

Functional complementation in yeast

Wild type (WT) yeast (Saccharomyces cerevisiae) strain (BY4741) and 7 deletion mutants in the same genetic background were used in this study (Table 1). The yeast strains were transformed with either MTP8.1, MTP8.2 expressed from pFL61 [36] or the empty vector. Transformants were grown on synthetic minimal media composed of 2% glucose (SD), 50 mM succinic acid/Tris base, pH 5.5, 0.7% yeast nitrogen base w/o amino acids (Difco), 0.3% of appropriate amino acids (histidine (H), leucine (L), methionine (M)). The presence of URA3 on pFL61 was used as auxotroph marker for uracil synthesis. For solid medium 2% agar was added [42]. Media deprived of Ca2+ were obtained using the chelators ethylene glycol-bis-β-aminoethylether-N,N,N′,N′-tetreacetic acid (EGTA, Sigma) or (2,2-bis(o-aminophenoxy)ethane-N,N,N′,N′-tetra acetic acid) (BAPTA, Sigma). The metal concentrations used as supplements in yeast media are presented in Table 1. Plates were incubated at 30°C for 3-5 days. All growth assays were repeated three times with independent yeast transformants.

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Table 1. List of yeast (Saccharomyces cerevisiae) strains used in this study.

https://doi.org/10.1371/journal.pone.0113759.t001

Identification of Mn transporter proteins

The yeast strain pmr1Δ was transformed by electroporation with a cDNA library from barley roots inserted into the vector pFL61 as previously described [36]. Transformants were selected on minimal media lacking uracil, harvested from the solid media, pooled, and resuspended in glycerol. From this pool, yeast aliquots were re-grown on medium with 2 mM Mn2+ to select for yeast cells complementing the Mn sensitivity of the pmr1Δ mutant. Plasmids were extracted from colonies complementing pmr1Δ [43] and amplified in Escherichia coli by standard procedures. Plasmids complementing pmr1Δ after re-transformation were sequenced and the barley genes were identified from similarity searches using BLAST analysis.

Yeast growth assay

Transformed pmr1Δ cells were cultured in 2 ml minimal media overnight at 30°C. The next day, 120 ml fresh medium was added and cells were re-incubated O/N to obtain a healthy yeast culture. The following day, all strains were inoculated in triplicates at seven different Mn2+ concentrations (0, 0.1, 0.25, 0.5, 1, 2, 5 mM) in 50 ml SD-HLM media at OD600  = 0.02.and grown for 46 hours at 30°C.

Elemental profile of MTP8 transformed yeast cells

Wild type and pmr1Δ transformed cells were grown overnight in 50 ml synthetic media. The next day cells were washed twice with ultra-pure H2O and re-suspended in 40 ml minimal media in polypropylene bottles at initial OD600 values of 0.06. The assay was performed with three replicates using two Mn2+ concentrations (2.4 and 100 µM). The yeast cells were grown to mid-exponential phase (17 hours at 150 rpm). The cells were again washed twice with ultra-pure H2O and then transferred to acid washed test tubes and freeze dried in a freeze drier (Christ Alpha 1-4, Martin Christ Gmbh).

The dry and weighed yeast samples were digested in 5 ml 70% HNO3 (J.T. Baker 9598) using a microwave oven (Multiwave 3000, software version 1.24, Anton Paar GmbH). Samples were diluted to 7% HNO3 and analyzed using Inductively Coupled Plasma Optical Emission Spectroscopy (ICP-OES, Optima 5300 DV; Perkin-Elmer) with the following wavelengths; 315.881A (Ca), 228.797A (Cd), 228.610A (Co), 324.750R (Cu), 238.199A (Fe), 766.473R (K), 279.072A (Mg), 257.606A (Mn), 214.909R (P), 181.971R (S), and 213.852A (Zn) nm. The accuracy and precision of the ICP-OES measurements were verified by including a certified reference material (Apple leaf, standard reference material 1515, National Institute of Standards and Technology). Data was accepted if the accuracy was above 90% of the standard reference material value for a given element.

Plant material

Seeds of Hordeum vulgare L. cv. ‘Vanessa’ were germinated at 21°C in vermiculite. After 5 d, uniform seedlings were selected and transferred to light-impermeable 4 L black cultivation units, each holding four plants. The units were filled with a chelate-buffered solution prepared in double ionized water with nutrient concentrations, except for Mn, as specified by Pedas et al. (2005). Four treatments were applied with different amounts of Mn (viz. 0 µg Mn (deficiency), 7.33 µg Mn (control), 110 µg Mn (toxicity I - Mntox1), and 586 µg Mn (toxicity II - Mntox2)) added to each cultivation unit three times per week in the form of MnCl2. The pH was kept at 6.0 by using 0.5 mM MES-TRIS pH 6.0. The plants were grown for 39 days in a controlled growth chamber with a 250 to 280 µmol m-2 s-1 photon flux density, 75% to 80% humidity, and a 20°C/15°C (16/8) day/night temperature regime.

Determination of trace element concentrations in plant material

Multi-elemental analyses by ICP-MS of leaf tissue were performed and compared with critical threshold limits found in [44]. Prior to analysis, plant samples were freeze dried (Christ Alpha 2-4; Martin Christ GmbH)) and digested using ultra-pure acids as previously described [1].

Analysis of gene expression in planta

Total RNA was isolated from root and shoot samples using the Fast RNA Pro Green Kit (MP Biomedicals, Solon, OH, USA) followed by TURBO DNase treatment (Applied Biosystems). RNA was converted to cDNA with M-MuLV Reverse Transcriptase (New England BioLabs), oligo-(dT) and random hexamer primers. The cDNA was diluted 5 times and normalized by further dilution to get the same DNA concentration in all samples. For quantification of MTP8.1, MTP8.2 and IRT1 gene expression, ACTIN was used as reference gene for normalization and cDNA was amplified by RT-qPCR using a Mx3000P Real-Time PCR System (Stratagene) in a total volume of 20 µl per reaction including: 1 µl normalized cDNA, 0.3 µM gene specific forward and reverse primers (Table 2), 1× DyNAmo Flash Master Mix and 0.4× ROX Passive Reference dye from DyNAmo Flash SYBER Green qPCR Kit (Finnzymes). The qPCR programme was set as follows: One cycle at 95°C for 7 minutes, followed by 40 cycles of 95°C for 10 seconds and 60°C for 30 seconds. A dissociation curve to check specificity of the amplified products was performed in the end of each programme with one cycle at 95°C for 1 min, 60°C for 30 seconds, ramping up to 95°C, followed by 1 minute at 95°C. Three biological replicates of each treatment were included and each reaction was performed in duplicate. The Pfaffl equation [45] was applied to calculate the relative expression levels. A standard curve was performed for each primer pair prior to RT-qPCR analysis in order to determine the amplification efficiency required for the Pfaffl equation.

Subcellular localization of MTP8-GFP fusion proteins in onion epidermal cells

A PCR-based cloning strategy was used to generate MTP8 gene sequences without stop codon for C-terminal fusions to the GFP gene. The cloning reaction used forward primers specific to the gateway cassette in pFL61 and reverse primers specific to C-termini of MTP8.1 and MTP8.2, respectively (Table 2) The PCR products were amplified using LA Taq (Takara), cloned using the gateway technique (Invitrogen), and sequenced by Eurofins MWG-Biotech, Germany. Correct clones were subsequently sub-cloned via the gateway technique (Invitrogen) to the p2GWF7 vector, consisting of the CaMV35S promoter, a NOS terminator, and the ORF of GFP [46]. p2GWF7-MTP8.1-GFP and p2GWF7-MTP8.2-GFP were used to transiently express MTP8.1- and MTP8.2-GFP fusion proteins in onion (Allium cepa) epidermal cells. Transient expression and localization were done as described by [47] with a few modifications. Briefly, 1×1 cm2 of onion bulb scales were placed on agar (1x Murashige and Skoog medium, 0.7% agar, and 3% Suc, pH 5.8) with the inner epidermis facing up. They were bombarded using the PDS-1000/He biolistic particle delivery system (Bio-Rad). Approximately 6 µg of expression vector was coated onto 1.5 mg of 1.6-µm gold particles and transferred into the cells. After bombardment, petri dishes containing the onion bulb squares were placed in the dark at room temperature for 18 to 24 h. The epidermis was then peeled and transformed cells were visualized using a Leica TCS SP2/MP confocal laser scanning microscope (Leica Microsystems). As a positive control for Golgi visualization, GONST-YFP proteins were co-localized with the MTP8-GFP proteins [48]. Excitation for GFP and YFP was done at 488 nm, and the emission spectra were recorded between 495 and 510 for GFP (green channel) and 530 and 545 nm for YFP (red channel). Sequential scanning between lines was used to follow both fluorescent signals at once. No fluorescence bleed-through was detected under our experimental conditions (data not shown). The co-localization analyses with GONST1-YFP were conducted with minimum three independent transient experiments. A quantitative co-localization analysis was performed using Fiji (ImageJ 1.49g) with a colocalization threshold plug-in (http://imagej.nih.gov/ij/index.html).

Accession numbers

The GenBank accession numbers for the sequences described in this article are as follows: Arabidopsis thaliana (AtMTP8: NP_191365; AtMTP9: NP_178070; AtMTP10: NP_173081; AtMTP11: NP_181477), Stylosanthes hamata (ShMTP8: AY181256; ShMTP9: AY181257; ShMTP10: AY181258; ShMTP11: AY181259), Oryza sativa (Os02g53490/OsMTP8; Os03g12530; Os01g03910; Os01g03914; Os05g38670; Os01g62070) and Hordeum vulgare (MTP8.1: JX051321; MTP8.2: JX051322; IRT1: EU545802; ACTIN: TC131547).

Results

Isolation of MTP8 genes from a yeast screen for barley Mn tolerance genes

To identify transport proteins involved in intracellular Mn2+ transport, we employed a yeast screen using the pmr1Δ mutant, which is deleted in PMR1 encoding a Ca2+/Mn2+-specific Golgi localized P-type ATPase [49], [50]. The pmr1Δ cells were transformed with a cDNA library prepared from barley root RNA. Complementing yeast transformants were selected on media containing 2 mM Mn, a condition which is toxic to pmr1Δ yeast cells [51]. Of 150 analyzed yeast transformants, 95% of the colonies were transformed with the same barley cDNA clone, 4% contained a second barley clone and 1% were false positives. The sequences of the two barley cDNA clones showed similarity to cation diffusion facilitator (CDF) family genes. The CDF family is a ubiquitous family of heavy metal transporters, found in all three kingdoms of life: Archaea, Eubacteria and Eukaryotes. All known CDF substrates are divalent cations (Me2+) and most of the characterized transporters are Me2+/H+ (K+) antiporters involved in efflux of the metal ion from the cytoplasm to the outside of the cell or into subcellular organelles (Montanini et al., 2007). Using bioinformatics, the barley MTP8 proteins were found to cluster within the MTP-subgroup of Mn specific transporters (data not shown). A phylogenetic analysis of protein data from Mn specific MTP plant proteins originating from Arabidopsis, Stylosanthes hamata, rice and barley revealed that the barley MTP proteins identified here belong to a subgroup, which contains MTP8-like proteins (Fig. 1). The barley proteins were consequently named MTP8.1 and MTP8.2. The closest relatives to the MTP8 proteins were two uncharacterized rice proteins Os03g12530 and Os02g53490, showing 92.4 and 69.3% identity to MTP8.1, and 70 and 80.7% identity to MTP8.2, respectively.

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Figure 1. Phylogenetic analysis of 16 MTP protein sequences from Hordeum vulgare (Hv), Oryza sativa (Os), Arabidopsis thaliana (At) and Stylosanthes hamata (Sh).

Alignment of full-length sequences was done as described for S1 Figure. The phylogenetic tree was drawn with the MEGA version 4.0 (http://www.megasoftware.net) [59]. Numbers represent bootstrap values for 1000 trees.

https://doi.org/10.1371/journal.pone.0113759.g001

The barley MTP8 proteins both include the conserved glycine and aspartate residues as well as the N-terminal CDF signature sequence [27], [52] (S1 Figure). MTP8.1 and MTP8.2 consist of 400 and 410 amino acids, respectively, corresponding to predicted molecular masses of 44.8 kDa and 45.7 kDa. Secondary structure predictions suggest five transmembrane (TM) domains in MTP8.1, whereas MTP8.2 contains four TM domains.

Screen for MTP8 metal selectivity in yeast

MTP8.1 and MTP8.2 complemented the Mn sensitivity of pmr1Δ cells when cultured on media with high Mn concentrations (Fig. 2A). The pmr1Δ mutant was also unable to grown on Ca depleted media because the Pmr1 protein is essential for loading of Ca into the ER and Golgi apparatus [49], [50]. The barley MTP8 proteins were not able to complement this phenotype (data not shown), suggesting that the MTP8 proteins are selective for Mn over Ca. Expression of MTP8 genes could not rescue numerous other yeast mutants defective in metal transport across the tonoplast of Zn and Co (cot1Δ, zrc1cot1Δ); Fe (ccc1Δ) or Cd (ycf1Δ). Also, no beneficial effects of MTP8 expression were found in smf1Δ or ace1Δ mutants defective in controlling Ni and Cu homeostasis, respectively (data not shown). The applied growth conditions for yeast complementation assays are presented in Table 1. These results clearly indicate that MTP8.1 and MTP8.2 has a preference for Mn as the transported ion.

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Figure 2. Effect of MTP8.1 and MTP8.2 expression on Mn2+ tolerance and Mn accumulation in the yeast mutant pmr1Δ.

Serial dilutions (1.0, 0.1 and 0.01 OD600) of pmr1 cells transformed with MTP8.1, MTP8.2 or empty vector (pFL6.1) were spotted on SD selective media with increased Mn content (A). Plates were incubated for 3-5 days at 30°C. The results are from one representative experiment out of three independent yeast transformations. Liquid yeast growth assay with MTP8.1 (circle), MTP8.2 (square) and pFL6.1 (triangle) transformed pmr1Δ cells grown with increasing Mn concentrations over 48 hours, data are the means ± SE of three independent yeast samples (B). Mn accumulation in pmr1Δ cells determined by ICP-OES analysis, cells were cultivated for 17 h with either 2.4 µM (black bars) or 100 µM (grey bars) Mn2+ in medium (C). Data are the means ± SE of three independent yeast samples. Values with the same letter within the same treatment are not significantly different (P>0.05).

https://doi.org/10.1371/journal.pone.0113759.g002

MTP8 proteins confer Mn tolerance to pmr1 via a Mn efflux mechanism

In liquid cultures of yeast pmr1Δ cells, both MTP8.1 and MTP8.2 resulted in high levels of Mn tolerance (Fig. 2B). The growth rates for pmr1Δ expressing either of the MTP8 homologs saturated at Mn concentrations above 1 mM and were unaffected by concentrations up to 5 mM Mn. In contrast, the growth rate of the control cells was severely reduced by Mn concentrations above 0.5 mM and growth almost ceased at 5 mM Mn.

To determine the elemental changes resulting from MTP8 expression, Inductively Coupled Plasma-Mass Spectrometry (ICP-MS) was performed on cells grown in normal media (2.4 µM Mn) or enriched with 100 µM Mn (Fig. 2C). The external Mn concentration of 100 µM did not restrict growth of either wild type or pmr1Δ cells due to Mn toxicity, thereby ensuring a minimum regulation of secondary toxicity affects including yeast endogenous Mn transporters. Elemental analysis showed that deletion of PMR1 by itself caused a 25-fold increase in the cellular Mn contents relative to the wild type. Mn concentrations in pmr1Δ cells expressing MTP8.1 or MTP8.2 were reduced by 20% when compared to pmr1Δ containing the empty vector (Fig. 2C). No other changes in elemental composition occurred between empty vector and MTP8 transformed yeast cells (S2 Figure).

Barley MTP8 proteins are targeted to the Golgi apparatus

To clarify the mechanism of Mn tolerance in yeast induced by MTP8.1 and MTP8.2, C-terminal fusions with green fluorescent protein (GFP) were transiently expressed in onion epidermal cells under control of the CaMV35S promoter. Both MTP8.1- and MTP8.2-GFP fusion proteins resulted in a punctated pattern of GFP-derived fluorescence, a highly characteristic feature of the Golgi apparatus (Fig. 3A and B, left panel). The MTP8-GFP localizations to Golgi were supported by co-expression of the Golgi-localized marker protein GONST1 fused to YFP [48] (Fig. 3A and B, right panel). A co-localization analysis was performed resulting in correlation coefficients of 0.81±0.03 and 0.85±0.05 for HvMTP8.1 and HvMTP8.2, respectively.

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Figure 3. C-terminal MTP8-GFP fusion proteins localizes to the Golgi apparatus.

As a control, GONST1-YFP were transiently co-expressed with MTP8.1-GFP and MTP8.2-GFP in onion epidermal cells (A and B), respectively. The right panels show co-localizations of GONST1-YFP with each MTP8-GFP protein. Scale bars were 75 and 100 µm for A and B, respectively.

https://doi.org/10.1371/journal.pone.0113759.g003

Regulation of MTP8.1 and MTP8.2 in response to plant Mn status

To characterize the in planta expression of MTP8.1 and MTP8.2, barley was cultivated in hydroponics with either insufficient, adequate (control) or excessive Mn supplies. The insufficient treatment reduced leaf Mn concentrations to 10 µg Mn g-1 DW which is 50% lower than in the control (Fig. 4A). Excessive Mn supply (treatments Mntox1 and Mntox2) resulted in foliar Mn concentrations between 170 and 280 µg Mn g-1 DW accompanied by typical Mn toxicity symptoms such as chlorosis and necrotic brown spots (data not shown). The biomass production of root and shoot tissues decreased in response to both insufficient and excessive Mn supplies (Fig. 4B and 4C) and Mn toxicity resulted in 20% increase in leaf dry matter content (Table 3). The altered biomass production was accompanied with marked changes in the elemental profile of the youngest leaves (Fig. 5).

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Figure 4. The effects of insufficient, control or two increasing Mn toxicity levels on Mn accumulation in the youngest fully developed leaves (A), shoot dry weight (B) and root dry weight (C) of barley plants.

Data are means ± SE (n = 3). Values with the same letter between treatments are not significantly different (P>0.05).

https://doi.org/10.1371/journal.pone.0113759.g004

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Figure 5. Elemental analysis of the youngest leaves of barley plants grown with insufficient, control or two increasing Mn toxicity levels.

The concentrations of five macro- (A) and four micronutrients (B) were determined in the youngest leaves. Data are means ± SE (n = 3). Values with the same letter between treatments are not significantly different (P>0.05).

https://doi.org/10.1371/journal.pone.0113759.g005

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Table 3. Leaf % dry weight of barley plants grown with varying Mn supplies. Data are means ± SE (n = 3).

https://doi.org/10.1371/journal.pone.0113759.t003

To determine if MTP8 transcripts fluctuate in response to changes in Mn concentrations of the root environment, quantitative reverse transcription PCR (RT-qPCR) was used on both root and shoot tissues. In roots, MTP8.1 and MTP8.2 transcripts were inversely regulated (Fig. 6A and B). The MTP8.1 transcript level increased with Mn supply ranging from deficiency to toxicity. In contrast, MTP8.2 expression showed a decrease as the external Mn concentration increased. In Mn deficient plants, MTP8.1 transcripts were down-regulated to 40% of the control level, whereas at the Mntox2 supply transcript levels rose to 140% of that obtained in plants grown at the control settings (Fig. 6A). For MTP8.2 transcripts, Mn deficiency increased to levels 40% higher than the control whereas transcript levels declined to 67% of the control at Mntox2 supply (Fig. 6B). MTP8.1 and MTP8.2 transcripts did not respond to Mn deficiency in shoots, whereas toxic supply of Mn resulted in a 3-4 fold down-regulation of both MTP8 genes in this organ (Fig. 6C and D).

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Figure 6. Quantitative expression analysis of MTP8 genes in barley plants grown with insufficient, control or two increasing Mn toxicity levels.

The expression level of MTP8.1 (A and C) and MTP8.2 (B and D) were determined in root (A and B) and shoot tissue (C and D). Data are normalized with respect to the expression of the reference gene ACTIN. Furthermore the relative changes in MTP8 expression levels are indexed to barley plants grown under control conditions. Data represent means (n = 3) ± SE. Values with the same letter between treatments for each MTP gene and plant organ are not significantly different (P>0.05).

https://doi.org/10.1371/journal.pone.0113759.g006

The transcript level of the broad specific metal ion transporter IRT1, which is localized in the plasma membrane of root cells with a potential role in metal uptake, was 60% up-regulated during Mn deficiency (Fig. 7). The IRT1 transcript levels also increased with up to 25% at toxic Mn supplies, indicating that transcriptional down-regulation of IRT1-mediated Mn uptake is not a Mn detoxification mechanism. The increased IRT1 expression level may also be related to declining Fe status since the Fe concentration decreased roughly 20% with increasing Mn supply (Fig. 5B). Foliar Zn and Cu concentrations were lowest in control plants and increased almost 2-fold in response to both insufficient and excessive Mn supplies.

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Figure 7. Quantitative expression analysis of IRT1 in root tissue of barley plants grown with insufficient, control or two increasing Mn toxicity levels.

Data are normalized with respect to the expression of the reference gene ACTIN. Furthermore the relative change in IRT1 expression is indexed to barley plants grown under control conditions. Data represent means ± SE (n = 3). Values with the same letter between treatments are not significantly different (P>0.05).

https://doi.org/10.1371/journal.pone.0113759.g007

Discussion

number of transport proteins with a putative role in cellular detoxification of excess Mn have previously been characterised in dicot plant species [26], [53]. However, similar information is currently not available for monocot species and consequently we conducted a barley cDNA library screen [36] expressed in the Mn sensitive yeast strain pmr1Δ. This resulted in identification of two genes encoding proteins involved in Mn tolerance when expressed in yeast. The encoded proteins were both homologous to the previously characterized MTP proteins OsMTP8 from rice [28], ShMTP8 from Stylosanthes [26] and AtMTP11 from Arabidopsis [53] (Fig. 1). The barley MTP8 proteins alleviated the growth defect of pmr1Δ caused by Mn toxicity (Fig. 2A), but not growth defects in a number of other yeast mutant strains related to defective Fe, Co, Zn, Ni, Cd, Ca or Cu transport (data not shown, Table 1). In addition, yeast strains expressing MTP8 genes were found to be specifically altered in Mn content, while all other divalent metals were unchanged (Fig. 2C and S2 Figure), thus showing a preference for Mn by the MTP8.1 and MTP8.2 proteins.

Cellular tolerance to excess Mn concentrations could either involve compartmentalization or export out of the cell. Analysis of the Mn accumulation in pmr1Δ yeast cells expressing barley MTP8 proteins showed that these proteins are involved in Mn efflux, as MTP8 pmr1Δ cells had a 20% reduction in their Mn contents when compared to the control (Fig. 2C). This reduction is relatively small compared to the 25 fold reduction in Mn content caused by the presence of Pmr1p in wild type yeast compared to pmr1Δ mutant. However, the Mn cellular homeostasis in yeast is tightly controlled [54]. In this heterologous expression system it is therefore unlikely that a plant Mn transport protein would be able to interact with the endogenous homeostatic partners in the same manner as the native Mn transporter. Nevertheless, expression of the MTP8 proteins enabled the yeast mutant to maintain optimal growth even at 5 mM Mn in the growth medium. The elemental profile of yeast cells grown at these two non-toxic Mn concentrations, with a minimum regulation of endogenous Mn homeostasis, strongly suggests that the tolerance mechanism is Mn efflux. The reduction in Mn content may be due to the MTP8 proteins being localized in the plasma membrane and/or Golgi apparatus. Previously, the Zn transporter TgMTP1 has been suggested to have a role in Zn tolerance due to its localization to the plasma membrane [55]. Furthermore, the Mn specific AtMTP11 protein has been suggested to have a role in Mn efflux due to its localization in the Golgi apparatus, where it delivers Mn into secretory vesicles directed to exocytosis [53]. The cellular localization of the MTP8 proteins in planta were clarified using transiently expressed GFP fusion proteins in onion epidermal cells. Transient expression of both MTP8-GFP fusion proteins in onion cells resulted in MTP8-GFP proteins co-localizing with the Golgi marker GONST1, thus supporting localization in the Golgi apparatus (Fig. 3A and 3B). This suggests a physiological role for MTP8 proteins in planta, where they may load Mn into Golgi in order to either provide Mn for Mn dependent enzymes within the Golgi or to efflux Mn via exocytosis of secretory vesicles. This is in contrast to the rice MTP8 homolog shown to be localized in the vacuole with a suggested role in Mn detoxification based on vacuolar Mn sequestration [28].

To determine if MTP8 proteins have a role in Mn toxicity tolerance in barley, similar to the heterologous yeast system, expression analysis by RT-qPCR was performed. The gene expression data showed that plants exposed to excessive Mn supply resulted in down-regulation of both MTP8 transcripts in leaf tissues (Fig. 6), as well as MTP8.2 transcripts in roots (Fig. 6). This indicates that the primary physiological roles of MTP8 proteins are not directly related to detoxification of excess Mn in planta. Instead they may be involved in the delivery of Mn to metabolic processes of the Golgi.

In contrast, the expression pattern of MTP8.1 in roots was positively correlated with the Mn concentration outside the root. Therefore, MTP8.1 may serve dual roles in planta both balancing excess Mn in roots and maintaining Mn homeostasis in Golgi in leaves. The MTP8.1 isoform was highly represented among the yeast clones complementing the pmr1 yeast strain in the original screen of the barley cDNA library, probably due to the generally higher transcript levels of MTP8.1 when compared to MTP8.2 in control plants (data not shown).

Hemicelluloses and pectins are synthesized in Golgi and require several different types of transport proteins to deliver sugars, acetyl-CoA, co-factors and ions to the working glycosyltransferases in the Golgi lumen [56]. Some glycosyltransferases require Mn for their activity [8]-[11] and due to their position in the Golgi lumen they are dependent on Mn-transporters placed in the Golgi membrane to facilitate metal delivery. The importance of the Golgi Mn pool may be directly visualized during Mn deficiency in plants, where slack leaves are a prominent and well described symptom. This is likely to be a result of Mn-deficiency induced defects in the delivery of intact cell wall components to growing cells.

Recent studies in mammalian cells indicate that the maintenance of Mn homeostasis is more complex than simply a matter of compartmentalization of Mn. A human Mn sensing glycoprotein (GPP130) has been found to induce vesicle trafficking from Golgi to multivesicular vesicles in response to elevated Golgi Mn concentrations as a way to regulate Mn extrusion from cells [57], [58]. A similar mechanism remains yet to be identified in plants.

Conclusions

Several enzymes activated or stimulated by Mn have been isolated from the Golgi apparatus, but it has until now not been clear how Mn is transported into Golgi in monocot species. We have here isolated and characterised two MTP8 proteins, MTP8.1 and MTP8.2, and have shown that they localize to the Golgi apparatus when expressed in onion epidermal cells and function as Mn transporters when expressed in yeast. In barley roots, the expression of MTP8.1 and MTP8.2 responds differently to increasing Mn status, suggesting that the two genes undertake contrasting physiological functions with respect to control of Mn homeostasis. Further studies including barley lines with altered expression levels of the two genes are required for further clarification of the exact roles of the MTP8.1 and MTP8.2 proteins in planta.

Supporting Information

S1 Figure.

Alignment of the putative amino acid sequences of barley MTP's to other plant MTP proteins. CLUSTAL W alignment of MTP proteins from Arabidopsis thaliana, Oryza sativa, Stylosanthes hamate and Hordeum vulgare was carried out using T-COFFEE (http://www.ch.embnet.org/software/TCoffee.html). The highly conserved N-terminal CDF signature sequence is marked with a box as well as the conserved aspartate and glycine residues are indicated with # and *, respectively.

https://doi.org/10.1371/journal.pone.0113759.s001

(TIF)

S2 Figure.

Effect of MTP8.1 and MTP8.2 expression on Mn, Fe, Zn and Cu accumulation in the yeast mutant pmr1Δ. Mn, Fe, Zn and Cu accumulation in pmr1Δ yeast determined by ICP-OES analysis, cells were cultivated for 17 h with either 2.4 µM (black bars) or 100 µM (grey bars) Mn2+ in medium. Data are the means ± SE of three independent yeast samples. Values with the same letter within the same treatment are not significantly different (P>0.05).

https://doi.org/10.1371/journal.pone.0113759.s002

(TIF)

Acknowledgments

Imaging data were collected at the Center for Advanced Bioimaging (CAB) Denmark, University of Copenhagen. We thank Paul Dupree for generously providing the AtGONST1-YFP construct. The technical assistance of Bente Broeng and Mette Sylvan is gratefully acknowledged.

Author Contributions

Conceived and designed the experiments: PP JNH JKS SH. Performed the experiments: PP MSS AHL. Analyzed the data: PP MSS JNH AHL JKS SH. Wrote the paper: PP SH.

References

  1. 1. Pedas P, Hebbern CA, Schjoerring JK, Holm PE, Husted S (2005) Differential Capacity for High-Affinity Manganese Uptake Contributes to Differences between Barley Genotypes in Tolerance to Low Manganese Availability. Plant Physiol 139:1411–1420.
  2. 2. Rengel Z (2000) Manganese uptake and transport in plants. Metal ions in Biological Systems 37:57–87.
  3. 3. Marschner H (1995) Mineral Nutrition of Higher Plants. ACADEMIC PRESS, San Diego, Californa, USA: 325-329.
  4. 4. Uexküll HRv, Mutert E (1995) Global extent, development and economic impact of acid soils. Plant and Soil 171:1–15.
  5. 5. Burnell JN (1988) The biochemistry of manganese in plants. In: Graham RD, Hannam, RJ, Uren, NCeditor. Manganese in Soils and Plants. Dordrecht, Boston, London: Kluwer academic publishers. pp.125-137.
  6. 6. Bowler C, Slooten L, Vandenbranden S, Rycke RD, Botterman J, et al. (1991) Manganese superoxide dismutase can reduce cellular damage mediated by oxygen radicals in transgenic plants. EMBO Journal 10:1723–1732.
  7. 7. Alscher RG, Erturk N, Heath LS (2002) Role of superoxide dismutases (SODs) in controlling oxidative stress in plants. J Exp Bot 53:1331–1341.
  8. 8. White AR, Xin Y, Pezeshk V (1993) Xyloglucan Glucosyltransferase in Golgi Membranes from Pisum-Sativum (Pea). Biochemical Journal 294:231–238.
  9. 9. Nunan KJ, Scheller HV (2003) Solubilization of an arabinan arabinosyltransferase activity from Mung ban hypocotyls. Plant Physiol 132:331–342.
  10. 10. Zeng W, Chatterjee M, Faik A (2008) UDP-xylose-stimulated glucuronyltransferase activity in wheat microsomal membranes: Characterization and role in glucurono(arabino) xylan biosynthesis. Plant Physiology 147:78–91.
  11. 11. Porchia AC, Sorensen SO, Scheller HV (2002) Arabinoxylan biosynthesis in wheat. Characterization of arabinosyltransferase activity in Golgi membranes. Plant Physiol 130:432–441.
  12. 12. Ono T, Noguchi T, Inoue Y, Kusunoki M, Matsushita T, et al. (1992) X-Ray-Detection of the Period-4 Cycling of the Manganese Cluster in Photosynthetic Water Oxidizing Enzyme. Science 258:1335–1337.
  13. 13. Hebbern CA, Laursen KH, Ladegaard AH, Schmidt SB, Pedas P, et al. (2009) Latent manganese deficiency increases transpiration in barley (Hordeum vulgare). Physiologia Plantarum 135:307–316.
  14. 14. Hebbern CA, Pedas P, Schjoerring JK, Knudsen L, Husted S (2005) Genotypic differences in manganese efficiency: a field trial with winter barley (Hordeum vulgare L.). Plant and Soil 272:233–244.
  15. 15. Pearson JN, Rengel Z (1997) Genotypic Differences in the Production and Partitioning of Carbohydrates Between Roots and Shoots of Wheat Grown under Zinc or Manganese Deficiency. Ann Bot 80:803–808.
  16. 16. Hall JL (2002) Cellular mechanisms for heavy metal detoxification and tolerance. J Exp Bot 53:1–11.
  17. 17. Pittman JK (2005) Managing the manganese: molecular mechanisms of manganese transport and homeostasis. New Phytologist 167:733–742.
  18. 18. Cailliatte R, Schikora A, Briat JF, Mari S, Curie C (2010) High-Affinity Manganese Uptake by the Metal Transporter NRAMP1 Is Essential for Arabidopsis Growth in Low Manganese Conditions. Plant Cell 22:904–917.
  19. 19. Vert G, Grotz N, Dedaldechamp F, Gaymard F, Guerinot ML, et al. (2002) IRT1, an Arabidopsis Transporter Essential for Iron Uptake from the Soil and for Plant Growth. Plant Cell 14:1223–1233.
  20. 20. Korshunova YO, Eide D, Clark WG, Guerinot ML, Pakrasi HB (1999) The IRT1 protein from arabidopsis thaliana is a metal transporter with a broad substrate range. Plant Molecular Biology 40:37–44.
  21. 21. Hirschi KD, Korenkov VD, Wilganowski NL, Wagner GJ (2000) Expression of Arabidopsis CAX2 in Tobacco. Altered Metal Accumulation and Increased Manganese Tolerance. Plant Physiol 124:125–134.
  22. 22. Shigaki T, Pittman JK, Hischi KD (2003) Manganese specificity determinants in the Arabidopsis metal/H+ antiporter CAX2. The Journal of Biological Chemistry 278:6610–6617.
  23. 23. Schaaf G, Catoni E, Fitz M, Schwacke R, Schneider A, et al. (2002) A putative role for the vacuolar calcium/manganese proton antiporter AtCAX2 in heavy metal detoxification. Plant Biology 4:612–618.
  24. 24. Pittman JK, Shigaki T, Marshall JL, Morris JL, Cheng N-H, et al. (2004) Functional and regulatory analysis of the arabidopsis thaliana CAX2 cation transporter. Plant Molecular Biology 56:959–971.
  25. 25. Kim SA, Punshon T, Lanzirotti A, Li L, Alonso JM, et al. (2006) Localization of Iron in Arabidopsis Seed Requires the Vacuolar Membrane Transporter VIT1. Science 314:1295–1298.
  26. 26. Delhaize E, Kataoka T, Hebb DM, White RG, Ryan PR (2003) Genes encoding proteins of the cation diffusion facilitator family that confer manganese tolerance. The Plant Cell 15:1131–1142.
  27. 27. Montanini B, Blaudez D, Jeandroz S, Sanders D, Chalot M (2007) Phylogenetic and functional analysis of the Cation Diffusion Facilitator (CDF) family: improved signature and prediction of substrate specificity. Bmc Genomics 8.
  28. 28. Chen ZH, Fujii Y, Yamaji N, Masuda S, Takemoto Y, et al. (2013) Mn tolerance in rice is mediated by MTP8.1, a member of the cation diffusion facilitator family. Journal of Experimental Botany 64:4375–4387.
  29. 29. Lanquar V, Leliévre F, Bolte S, Hamés C, Alcon C, et al. (2005) Mobilization of vacuolar iron by AtNRAMP3 and AtNRAMP4 is essential for seed germination on low iron. The EMBO Journal 24:4041–4051.
  30. 30. Lanquar V, Ramos MS, Lelievre F, Barbier-Brygoo H, Krieger-Liszkay A, et al. (2010) Export of Vacuolar Manganese by AtNRAMP3 and AtNRAMP4 Is Required for Optimal Photosynthesis and Growth under Manganese Deficiency. Plant Physiology 152:1986–1999.
  31. 31. Wu Z, Liang F, Hong B, Young JC, Sussman MR, et al. (2002) An Endoplasmic Reticulum-Bound Ca2+/Mn2+ Pump, ECA1, Supports Plant Growth and Confers Tolerance to Mn2+ Stress. Plant Physiol 130:128–137.
  32. 32. Mills RF, Doherty ML, Lopez-Marques RL, Weimar T, Dupree P, et al. (2008) ECA3, a Golgi-Localized P2A-Type ATPase, Plays a Crucial Role in Manganese Nutrition in Arabidopsis. Plant Physiol 146:116–128.
  33. 33. Li XY, Chanroj S, Wu ZY, Romanowsky SM, Harper JF, et al. (2008) A distinct endosomal Ca2+/Mn2+ pump affects root growth through the secretory process. Plant Physiology 147:1675–1689.
  34. 34. Axelsen KB, Palmgren MG (2001) Inventory of the superfamily of P-type ion pumps in Arabidopsis. Plant Physiology 126:696–706.
  35. 35. Delhaize E, Gruber BD, Pittman JK, White RG, Leung H, et al. (2007) A role for the AtMTP11 gene of Arabidopsis in manganese transport and tolerance. Plant Journal 51:198–210.
  36. 36. Pedas P, Ytting CK, Fuglsang AT, Jahn TP, Schjoerring JK, et al. (2008) Manganese efficiency in barley; identification and characterization of the metal transporter HvIRT1. Plant Physiology 148:455–466.
  37. 37. Koike S, Inoue H, Mizuno D, Takahashi M, Nakanishi H, et al. (2004) OsYSL2 is a rice metal-nicotianamine transporter that is regulated by iron and expressed in the phloem. The Plant Journal 39:415–424.
  38. 38. Ishimaru Y, Masuda H, Bashir K, Inoue H, Tsukamoto T, et al. (2010) Rice metal-nicotianamine transporter, OsYSL2, is required for the long-distance transport of iron and manganese. Plant Journal 62:379–390.
  39. 39. Sasaki A, Yamaji N, Xia JX, Ma JF (2011) OsYSL6 Is Involved in the Detoxification of Excess Manganese in Rice. Plant Physiology 157:1832–1840.
  40. 40. Yang M, Zhang W, Dong H, Zhang Y, Lv K, et al. (2013) OsNRAMP3 is a vascular bundles-specific manganese transporter that is responsible for manganese distribution in rice. PLoS One 8:e83990.
  41. 41. Yamaji N, Sasaki A, Xia JX, Yokosho K, Ma JF (2013) A node-based switch for preferential distribution of manganese in rice. Nature Communications. 4.
  42. 42. Sherman F (1991) Getting started with yeast. Methods Enzym 194:3–21.
  43. 43. Hoffman CS, Winston F (1987) A ten-minute DNA preparation from yeast efficiently releases autonomous plasmids for transformation of Escherichia coli. Gene 57:267–272.
  44. 44. Reuter DJ, Edwards DG, Wilhelm NS (1997) Temperate and Tropical Crops. In: Reuter DJ, Robinson JBeditors. Plant Analysis: An Interpretation Manual.Second Edition ed. Victoria: CSIRO Publishing. pp.81-279.
  45. 45. Pfaffl MW (2001) A new mathematical model for relative quantification in real-time RT-PCR. Nucleic Acids Research. 29.
  46. 46. Karimi M, Inze D, Depicker A (2002) GATEWAY((TM)) vectors for Agrobacterium-mediated plant transformation. Trends in Plant Science 7:193–195.
  47. 47. Jensen MK, Rung JH, Gregersen PL, Gjetting T, Fuglsang AT, et al. (2007) The HvNAC6 transcription factor: a positive regulator of penetration resistance in barley and Arabidopsis. Plant Molecular Biology 65:137–150.
  48. 48. Baldwin TC, Handford MG, Yuseff MI, Orellana A, Dupree P (2001) Identification and characterization of GONST1, a Golgi-localized GDP-mannose transporter in Arabidopsis. Plant Cell 13:2283–2295.
  49. 49. Rudolph HK, Antebi A, Fink GR, Buckley CM, Dorman TE, et al. (1989) The Yeast Secretory Pathway Is Perturbed by Mutations in Pmr1, a Member of a Ca-2+ Atpase Family. Cell 58:133–145.
  50. 50. Antebi A, Fink GR (1992) The Yeast Ca-2+-Atpase Homolog, Pmr1, Is Required for Normal Golgi Function and Localizes in a Novel Golgi-Like Distribution. Molecular Biology of the Cell 3:633–654.
  51. 51. Lapinskas PJ, Cunningham KW, Liu XF, Fink GR, Culotta C (1995) Mutations in Pmr1 Suppress Oxidative Damage in Yeast-Cells Lacking Superoxide-Dismutase. Molecular and Cellular Biology 15:1382–1388.
  52. 52. Paulsen IT, Saier MH (1997) A novel family of ubiquitous heavy metal ion transport proteins. Journal of Membrane Biology 156:99–103.
  53. 53. Peiter E, Montanini B, Gobert A, Pedas P, Husted Sr, et al. (2007) A secretory pathway-localized cation diffusion facilitator confers plant manganese tolerance. PNAS 104:8532–8537.
  54. 54. Reddi AR, Jensen LT, Culotta VC (2009) Manganese Homeostasis in Saccharomyces cerevisiae. Chemical Reviews 109:4722–4732.
  55. 55. Kim D, Gustin JL, Lahner B, Persans MW, Baek D, et al. (2004) The plant CDF family member TgMTP1 from the Ni/Zn hyperaccumulator Thlaspi goesingense acts to enhance efflux of Zn at the plasma membrane when expressed in Saccharomyces cerevisiae. The Plant Journal 39:237–251.
  56. 56. Reyes F, Orellana A (2008) Golgi transporters: opening the gate to cell wall polysaccharide biosynthesis. Current Opinion in Plant Biology 11:244–251.
  57. 57. Mukhopadhyay S, Bachert C, Smith DR, Linstedt AD (2010) Manganese-induced Trafficking and Turnover of the cis-Golgi Glycoprotein GPP130. Molecular Biology of the Cell 21:1282–1292.
  58. 58. Mukhopadhyay S, Linstedt AD (2011) Identification of a gain-of-function mutation in a Golgi P-type ATPase that enhances Mn(2+) efflux and protects against toxicity. Proceedings of the National Academy of Sciences of the United States of America 108:858–863.
  59. 59. Tamura K, Dudley J, Nei M, Kumar S (2007) MEGA4: Molecular evolutionary genetics analysis (MEGA) software version 4.0. Molecular Biology and Evolution 24:1596–1599.
  60. 60. Winzeler EA, Shoemaker DD, Astromoff A, Liang H, Anderson K, et al. (1999) Functional characterization of the S-cerevisiae genome by gene deletion and parallel analysis. Science 285:901–906.