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Research Article

The ASH1 HOMOLOG 2 (ASHH2) Histone H3 Methyltransferase Is Required for Ovule and Anther Development in Arabidopsis

  • Paul E. Grini equal contributor,

    equal contributor Contributed equally to this work with: Paul E. Grini, Tage Thorstensen, Vibeke Alm

    Affiliation: Department of Molecular Biosciences, University of Oslo, Oslo, Norway

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  • Tage Thorstensen equal contributor,

    equal contributor Contributed equally to this work with: Paul E. Grini, Tage Thorstensen, Vibeke Alm

    Affiliation: Department of Molecular Biosciences, University of Oslo, Oslo, Norway

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  • Vibeke Alm equal contributor,

    equal contributor Contributed equally to this work with: Paul E. Grini, Tage Thorstensen, Vibeke Alm

    Affiliation: Department of Molecular Biosciences, University of Oslo, Oslo, Norway

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  • Gema Vizcay-Barrena,

    Affiliation: School of Biosciences, University of Nottingham, Nottingham, United Kingdom

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  • Susanne S. Windju,

    Affiliation: Department of Molecular Biosciences, University of Oslo, Oslo, Norway

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  • Tommy S. Jørstad,

    Affiliation: Department of Biology, Norwegian University of Sciences and Technology, Trondheim, Norway

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  • Zoe A. Wilson,

    Affiliation: School of Biosciences, University of Nottingham, Nottingham, United Kingdom

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  • Reidunn B. Aalen mail

    reidunn.aalen@imbv.uio.no

    Affiliation: Department of Molecular Biosciences, University of Oslo, Oslo, Norway

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  • Published: November 12, 2009
  • DOI: 10.1371/journal.pone.0007817

Abstract

Background

SET-domain proteins are histone lysine (K) methyltransferases (HMTase) implicated in defining transcriptionally permissive or repressive chromatin. The Arabidopsis ASH1 HOMOLOG 2 (ASHH2) protein (also called SDG8, EFS and CCR1) has been suggested to methylate H3K4 and/or H3K36 and is similar to Drosophila ASH1, a positive maintainer of gene expression, and yeast Set2, a H3K36 HMTase. Mutation of the ASHH2 gene has pleiotropic developmental effects. Here we focus on the role of ASHH2 in plant reproduction.

Methodology/Principal Findings

A slightly reduced transmission of the ashh2 allele in reciprocal crosses implied involvement in gametogenesis or gamete function. However, the main requirement of ASHH2 is sporophytic. On the female side, close to 80% of mature ovules lack embryo sac. On the male side, anthers frequently develop without pollen sacs or with specific defects in the tapetum layer, resulting in reduction in the number of functional pollen per anther by up to ~90%. In consistence with the phenotypic findings, an ASHH2 promoter-reporter gene was expressed at the site of megaspore mother cell formation as well as tapetum layers and pollen. ashh2 mutations also result in homeotic changes in floral organ identity. Transcriptional profiling identified more than 300 up-regulated and 600 down-regulated genes in ashh2 mutant inflorescences, whereof the latter included genes involved in determination of floral organ identity, embryo sac and anther/pollen development. This was confirmed by real-time PCR. In the chromatin of such genes (AP1, AtDMC1 and MYB99) we observed a reduction of H3K36 trimethylation (me3), but not H3K4me3 or H3K36me2.

Conclusions/Significance

The severe distortion of reproductive organ development in ashh2 mutants, argues that ASHH2 is required for the correct expression of genes essential to reproductive development. The reduction in the ashh2 mutant of H3K36me3 on down-regulated genes relevant to the observed defects, implicates ASHH2 in regulation of gene expression via H3K36 trimethylation in chromatin of Arabidopsis inflorescences.

Introduction

Active transcription of eukaryotic genes is dependent on a permissive chromatin structure that allows transcription factors access to promoter and enhancer regions. The accessibility of chromatin depends on the position and packaging of the nucleosomes and relies upon enzymes that modify residues on the protruding histone tails, or recognize such modifications. A number of histone tail modifications have been identified including acetylation, phosphorylation, ubiquitination, and methylation [1]. While acetylation of lysine (K) residues in general is associated with transcriptional activity, methylation of lysines can be associated with maintenance of an active or a repressed state depending on the position of the modified residues. In general, euchromatin contains elevated levels of histone H3 lysine methylation at positions 4, 36 and 79 as well as hyperacetylation of histone H4 [2].

Enzymes that can add methyl groups to lysine residues on histone tails can be grouped in evolutionarily conserved classes named after the Drosopohila proteins SU(VAR)3–9, E(Z), TRITHORAX (TRX) and ASH1, that all have a similar 130 amino acid (aa) long SET domain [3], [4]. Proteins belonging to the ASH1 class have properties similar to TRX in maintenance of transcription during development. These four classes have also been identified in Arabidopsis thaliana [5]. In the Arabidopsis ASH1 class there are four ASH1 HOMOLOGs (ASHH) and three ASH1 RELATED (ASHR) members [5]. ASHH2 (At1g77300, called SET DOMAIN GROUP 8 (SDG8) in the Plant Chromatin Database http://www.chromdb.org) was the first Arabidopsis gene of the ASH1 class to be ascribed a biological function, namely in controlling flowering time. This gene is also named EFS as it was identified as the one affected in the mutant early flowering in short days (efs) in the Landsberg erecta (Ler) ecotype, and mutations also result in earlier flowering in the Colombia (Col) ecotype (Table 1) [6], [7]. The early flowering phenotype correlated to transcriptional repression of the key regulator of flowering time, FLOWERING LOCUS C (FLC) [6][8]. FLC-centered studies have been crucial for the elucidation of the molecular mechanisms of epigenetic gene regulation [9]. However, several genes affecting FLC, including ASHH2, ATX1, ELF7 and ELF8, display additional mutant phenotypes, in plant size, flower morphology and/or fertility [8], [10], [11]. Recently, ASHH2 has also been shown to be involved in regulating shoot branching and carotenoid composition (Table 1) [12], [13].

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Table 1. Alleles of ashh2.

doi:10.1371/journal.pone.0007817.t001

These additional phenotypes are worth investigations as they suggest epigenetic gene regulation in other developmental processes. In the present paper we have therefore examined the ashh2 mutant phenotype with respect to causes of severely reduced fertility, which was already noted by [8]. Serious defects in both male and female reproductive organ development are observed. In a microarray experiment comparing gene expression in ashh2 and wild type (wt) inflorescences, followed by quantitative RT-PCR confirmation, we have identified genes associated with the mutant phenotype with significantly reduced expression levels.

In vitro ASHH2 shows histone H3 methyltransferase (HMTase) activity on oligonucleosomes and core histones [12], [14]; but activity on unmodified recombinant histone tails has not been demonstrated, suggesting that the protein need some premodification or cofactor to function. Thus the exact specificity is not known, but Chromatin Immuno Precipitation (ChIP) at FLC and other loci in ashh2/sdg8/efs/ccr1 mutants compared to wt has suggested that ASHH2 is a H3K4 trimethyltransferase [6], [13] and/or a H3K36 di- and trimethyltransferase [7], [12], [14]. We have used antibodies against these marks in our ChIP experiments on chromatin from inflorescences, and demonstrate significant reduction of H3K36me3 methylation, but not H3K4me3 or H3K36me2 on down-regulated genes associated with the mutant ashh2 phenotypes. This suggests that ASHH2 controls development of Arabidopsis reproductive organs via H3K36 trimethylation.

Results

Mutation in ASHH2 results in a pleiotropic phenotype

Four ashh2 alleles were analyzed; with T-DNAs inserted in the promoter 643 bp upstream of the translation start (ashh2-6), in the first intron (ashh2-2/sdg8-2), in the sixth exon (ashh2-5) and the sixth intron/seventh exon (ashh2-1/sdg8-1), respectively (Figure 1A, Table 1). In the latter three alleles the ASHH2 expression levels are strongly reduced compared to wt (Figure 1B). These alleles are not expected to produce functional proteins, as the T-DNAs are positioned upstream of or in the region encoding the SET domain, suggesting that they are null alleles. Plants homozygous for ashh2-1, ashh2-2 and ashh2-5 show a characteristic dwarf and bushy phenotype (Figures 1C and 1H, and Figure S1). This phenotype was not found in ashh2-6 plants, the only allele that can be expected to produce a normal transcript and for which the expression level in inflorescences was only reduced to 55% (Figure 1B and Figure S1). We have mainly focused on the phenotypes found to be common to all alleles. All ashh2 organs were smaller than wt organs (Figures 1D and 1E). Stamens were shorter with thinner filaments that often were bent just beneath the anther, while the carpels were shorter and thicker compared to wt (Figure 1F). ashh2 siliques developed poorly (Figure 1G), and flowering and growth continued for at least 100 days (Figure 1H). These plants had highly branched internodes (Figure 1I) and composite or clustered flowers without pedicels (Figure 1J).

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Figure 1. Alleles of ashh2 and the pleiotropic phenotype of ashh2 mutant plants.

(A) Position of the T-DNA insertions of different SALK lines as indicated. The 15 exons of ASHH2 are shown as black boxes and the introns as thin lines. Numbers refer to base pairs (bp) in the Arabidopsis genomic BAC clone T14N5 (acc.no. AC004260) and indicate insertion sites of the T-DNAs, start and stop codons and selected exon-intron borders. The positions of primers used for real-time PCR are show in green above exons 10 and 11. Both the right and the left junction between the ASHH2 gene and the insertions were cloned and sequenced for all alleles except ashh2-5 which is likely to have a complex insertion. Genomic deletions of 33 and 8 bp where found at the insertion sites of ashh2-2 and ashh2-1, respectively. The lower panel shows the ASHH2 protein and the positions of known domains. (B) Relative expression level of ASHH2 in ashh2 mutant plants. Real-time PCR on cDNA from inflorescences of plants homozygous for the indicated alleles as compared to the level in wt inflorescences (set to 1). Standard deviations are shown. (C) Dwarf phenotype of ashh2-1 with several inflorescences (left) compared to wt plant with main inflorescence and a shorter auxiliary shoot (right). (D) Small ashh2-1 cauline leaf (top) and wt cauline leaf (bottom). (E) Small ashh2-1 flower (left) compared to wt flower (right). (F) ashh2-1 flowers with mild (top left) and more severe (bottom left) distorted stamens and carpels compared to wt flowers (right). Some sepals and petals have been removed to display the inner whorl organs. ashh2-1 stamens are often shorter than wt stamens (bottom middle). (G) Siliques of ashh2-1 plant (left) and wt plant (right). (H) ashh2-1 plant 100 days after sowing. (I) Highly branched internode of ashh2-1 plant 100 days after sowing. (J) Composite flower of ashh2-1 plant 100 days after sowing. (K) Scanning electron micrograph (SEM) of ashh2-1 flower with sepals and carpeloid organs with vestigial ovules (ov) and stigmatic papillae (sg). (L) ashh2-1 flower with carpeloid sepals (cs) and stamenoid petals (sp). (M) SEM of stamenoid petal of ashh2-1 flower.

doi:10.1371/journal.pone.0007817.g001

Inflorescences with flowers exhibiting homeotic transformations were consistently observed in all alleles inspected, including the efs1-1 allele in Ler background (Table S1). The transformed flowers mainly displayed sepals and carpeloid organs (Figure 1K) or carpeloid sepals and stamen-like petals (Figures 1L and 1M). Homeotic changes with sepal and petal organs only, were never encountered (n = 83, Table S1).

ashh2 transmission is affected through both male and female gametes

Mutant plants of all alleles had short siliques. In ashh2-1 siliques the ovule number was reduced by 80% compared to wt (Figure 2A), and less than a quarter of the ovules developed into mature seeds (Figures 2B and 2D). Reduced seed setting was also observed after hand self-pollination of the mutant. In situ hybridization demonstrated expression of ASHH2 in the endosperm as well as in the developing embryo (Figure 2C). If the reduced seed set was due to developmental defects in homozygous ashh2 fertilization products, one would have expected 25% aborted seeds when self-fertilizing heterozygous plants. However, ASHH2 appears to be redundant both for embryo and endosperm development as no deviation from wt in number of ovules/seeds or phenotype could be observed during embryogenesis in siliques of selfed heterozygous ASHH2/ashh2-1 plants (Figure 2B).

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Figure 2. Ovule development and seed set in ashh2 mutant plants, and pASHH2:GUS expression during ovule and seed development.

(A) Total number of seeds/ovules per silique in selfed wt (nsiliques = 12), homozygous (nsiliques = 125) and heterozygous ashh2-1 plants (nsiliques = 26). (B) Percentage of developing green seeds and undeveloped ovules per silique in selfed wt (nsiliques = 12), homozygous (nsiliques = 125) and heterozygous ashh2 plants (nsiliques = 26) prior to seed desiccation. (C) In situ hybridization on longitudinal sections of seeds at the heart stage (left) and the walking stick stage (right) of embryo development with ASHH2 antisense probe (AS) and control sense probe (S). Expression was seen in the whole heart stage embryo (em), the chalazal endosperm (cze) as well as the endosperm nodules (en) aligning the embryo sac around the vacuole (v). At the walking stick stage expression was seen both in the cotyledons (cot), hypocotyl (hyp) and root tip (r). (D) Full-length ashh2-1 mutant silique compared to a segment of a wt siliques, with enlarged sections to the right. Arrows point to undeveloped ovules. (E) pASHH2:GUS expression in the nucellus of the developing ovule. The GUS signal is located in the L2 layer where the megaspore (m) forms. Nucellar tissue (n), chalazal tissue (cz), inner integuments (ii), outer integuments (oi). (F) pASHH2:GUS expression in the ovule with mature embryo sac. Strong expression is found in maternal chalazal proliferating tissue (cz). Weaker expression was observed in the nucellus and inner (ii) and outer integuments (oi). (G) pASHH2:GUS expression in maternal tissue strongly in the chalazal tissues (cz) and weaker in the inner integuments (ii) and even weaken in the outer integument (oi) after fertilization. The chalazal region (cz) is indicated by an arrow and pollen tubes (pt) that have grown along the funiculus (f) with thin lines. The septum (s) with its transmitting tract (tt) is indicated.

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If the reduced seed set was due to a defect in ashh2 haploid gametophytes, one would expect reduced transmission of the mutant allele. Therefore we genotyped the progeny resulting from self-fertilization of heterozygous plants. Self-fertilization of ASHH2/ashh2-1 plants resulted in only 8% homozygous ashh2-1/ashh2-1 mutant progeny and 37% wt plants, instead of the expected 25% (n = 62, Table 2). A similar frequency of homozygous plants resulted from selfing of heterozygous ASHH2/ashh2-2, ASHH2/ashh2-5 and ASHH2/ashh2-6 plants (10.7%, n = 140; 8.5%, n = 71; 17%, n = 94, respectively). As no seed abortion could be observed, this suggested that male and/or female transmission was affected. This was tested with reciprocal crosses of ASHH2/ashh2-1 heterozygous plants with wt plants, which revealed that both female and male transmission was reduced from the expected 50% to 39% and 37%, respectively (Table 2). The transmission efficiency (Table 2) for the male and female mutant alleles would result in an expected frequency of ashh2 homozygous progeny of 9%, i.e. close to the observed 8%. The expected number of male and female gametophytes in ASHH2/ashh2 plants defective in transmission of mutant gametes would be about 20% (Table 2) [15]. Since no obvious defects in pollen or embryo sac development could be observed in heterozygous lines, this suggests a role for ASHH2 in gametophyte function, e.g. pollen tube growth or attraction.

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Table 2. Segregation of ASHH2/ashh2 in reciprocal crosses with wt.

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The frequency of affected female or male gametophytes alone could not account for the severe reduction in seed set observed in homozygous ashh2 plants (Figures 2A, 2B and 2D). Thus this suggests that the main requirement of ASHH2 is in the sporophyte for proper development or function of ovules and anthers.

ashh2 mutants are defective in ovule and embryo sac development

In wt plants, one megaspore resulting from meiosis of the megaspore mother cell (MMC) develops into the embryo sac comprised of the egg cell, two synergid cells, three antipodal cells, and a dihaploid central cell (Figure 3A). Inner- and outer integuments elongate in the proximal-distal axis and encase the nucellar tissue.

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Figure 3. Ovule and embryo sac development in wt and ashh2-1.

Differential interference contrast (DIC) micrographs of (A) wt and (B–L) ashh2-1 ovules at one day post anthesis (A–C), anthesis (D–F), day before anthesis (G–I) and at the time point of the first syncytial nuclear division (J–L). Scale bar, 25 µm. (A) Wt mature ovule harboring embryo sac with (arrows) egg cell (ec), central cell (cc) and synergid cells (syn, only one synergid cell is in the focal plane). The embryo sac is surrounded by maternal chalazal (cz) tissue and endothelium layer (et), and further surrounded by two more layers of inner integuments (ii) and two layers of outer integuments (oi). Arrowheads mark the border between the embryo sac and the adaxial (adx) endothelium and the abaxial (abx) chalazal tissue. (B) ashh2-1 ovule without embryo sac between endothelium and the adaxial chalazal tissue (arrowheads). Ovule morphology appears fairly normal with two outer integument layers (oi) and three inner integuments (ii and et). The chalazal tissue in the center of the ovule appears to have proliferated more than in wt. (C) ashh2-1 ovule from same silique as (B) with a single mono-nucleate cell (boxed). Inset in the upper right corner shows magnification of boxed area (n, nucleus). The outer integuments engage both inner integuments and nucellus. (D) ashh2-1 syncytial embryo sac with eight nuclei. Inset in the upper right corner shows magnification of boxed area (n, nucleus). Two nuclei are not in the focal plane. (E) Proliferated ashh2-1 syncytial embryo sac. Inset in the upper right corner is a merge of two focal planes and shows magnification of the boxed area (n, nucleus). The basally located nuclei appear to degenerate. Note that the micropylar end of the embryo sac is not covered by integuments in both (E) and (F). (F) ashh2-1 embryo sac. Inset in the upper right corner shows magnification of the boxed area show two nuclear structures reminiscent of egg and central cell nuclei (n, nucleus). (G–H) ashh2-1 ovules with embryo sac-like structure (arrow) budding off the micropylar end of the ovule. The integuments do not encase the structure. (I) ashh2-1 ovule arrested or delayed in development. The inner integuments have developed longer than the outer integuments. (J–L) ashh2-1 ovules with two nucleate syncytial embryo sacs. No vacuole could be observed between the nuclei (n, nucleus).

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One day post anthesis (flower stage 12) when wt ovules harbor a mature embryo sac (Figure 3A), no apparent embryo sac, or in a few cases an embryo sac consisting of a single-nucleated cell, was found in mutant ovules (Figures 3B and 3C; 79%, n = 141). The overall ovule and integument morphology was close to wt in this class, however, an overproliferation of the abaxial chalazal part of the ovule was often observed (Figure 3B). In slightly earlier stages, a small fraction of ovules could be found where up to three rounds of nuclear proliferation had occurred in the embryo sac (Figures 3D to 3F; 9%, n = 141, in corresponding wt stages 95%, n = 111). In most cases, these syncytial embryo sacs were not encased completely by the outer integuments (Figures 3E and 3F). The observed proliferating nuclei were in most cases undifferentiated (Figure 3D) or appeared to start to degenerate (Figure 3E), but nuclear structures reminiscent of egg and central cell nuclei were also observed (Figure 3F). In some cases (10%, n = 141) the embryo sac-like structure was not surrounded by the integuments and protruded out of the micropyle as a “bag” of nuclei (Figures 3G and 3H). The nuclei in some cases appeared degenerated (Figure 3G) or were of different sizes (Figure 3H). In ovules that aborted in early stages both outer and inner integument elongation appeared to be delayed (Figure 3I).

In order to investigate whether embryo sacs develop and thereafter are expelled from the ovule, thus resulting in an apparent lack of the female gametophyte, or if most embryo sacs abort and degenerate at early stages of development, we analyzed young stages of embryo sac development. We found that the majority of the embryo sacs inspected (66%, n = 62) were degenerated and no clear nuclear morphology could be seen. In 18% of the embryo sacs a prominent single nuclei could be found (similar to Figure 3C, n = 62). However, 16% of the embryo sacs had completed the first nuclear division and harbored two syncytial nuclei (Figure 3J–L, n = 62). Our findings thus favor a scenario where most ashh2 embryo sacs arrest and degenerate slightly after or before the first syncytial division. The number of embryo sacs that have made the first nuclear division is in good accordance with the number of protruding embryo sacs found at later stages, suggesting that if the first division is made further divisions can follow, but that most of these syncytial embryo sacs will be expelled, resulting in an apparent lack of the female gametophyte.

Taken together the observed defect in ashh2 ovules appears to be a failure to progress into female gametophyte or embryo sac development after meiosis. Based on the genetics of the mutant lines, a sporophytic requirement of ASHH2 is suggested and thus the primary defect may relay on a failure in meiosis or MMC initiation. In support of this hypothesis, a construct with the ASHH2 promoter coupled to the GUS reporter gene, was expressed in the subepidermal L2 cell layer of the nucellus at the position of MMC initiation (Figure 2E) [16]. The observed phenotype could alternatively be effected by missing support from the maternal ovule integuments. However, during later stages of the mature embryo sac, pASHH2:GUS expression was most prominent in maternal chalazal proliferating tissue and only weakly expressed in the integuments (Figures 2F to 2G).

ashh2 plants have reduced numbers of pollen

Due to the low expected frequency of affected pollen grains in heterozygous plants (Table 2) male semi-sterility was studied in homozygous mutants. All mutant alleles had reduced amounts of pollen (Figure 4A); anthers displayed a large variation in the number of pollen in each pollen sac (locule) with frequent empty or undeveloped locules (Figure 4B, Figure S2), e.g. ~1.6 locules were seen per ashh2-1 anther (total 49 locules in 31 anthers). This suggests that the early stages of archesporial division have been affected, resulting in an absence of the parental cell layers generating the sporocytes.

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Figure 4. Pollen development in ashh2 and pASHH2:GUS expression in anther development.

(A) Average number of pollen per anther (nwt = 4, nashh2>8) in wt and ashh2 mutant lines. Standard deviations are shown. (B) Light- and fluorescent micrographs of ashh2-1 anthers and germinating pollen tubes. (i) Four long stamina from ashh2-1 from a flower just before abscission. All anthers are delayed in dehiscence. Note different numbers of pollen (p) in each locule and absence of normal locule development (arrows). (ii) Mature ashh2-1 anther with released pollen in the trinucleate stage (boxed area). Inset is a magnification of the boxed area, (s) sperm cell, (v) vegetative cell. (iii) Pollen tube germination on the papillae in ashh2-1. (p) pollen, (pt) pollen tube. (C) Stage 7 flower of pASHH2:GUS plant. No GUS expression was seen in the developing floral organs but only in the pedicel. s – sepal; g – gynoecium; pp – petal primordium; sp – stamen primordium. (D) Stage 9 to 11 flowers showing increasing GUS expression post meiosis. The boxed insert shows that no GUS expression was detected in tetrads. s – sepal; g – gynoecium; a – anther. (E) Stage 12 flower with mature anthers with GUS expression in anthers (a), as well as the gynoecium (g) and mid veins of petals (p) and sepals (s). (F) Anther of stage 12 flower showing GUS expression both in the tapetal cell layer (t) and the mature microspores (ms), but not in the anther filaments (f). (G) Detail of GUS expression in floral stage 12 anther demonstrate specific expression in tapetum (t) and microspores (ms), but not in the surrounding endothecium (en) and epidermis (e) cell layers. (H) Scanning electron micrographs of wt pollen (i) with a sexine layer (ii) with regular ridges (muri – m) and spaces (lumina – l). (I) Scanning electron micrographs of ashh2-1 pollen grains (i, ii) and exine layers with filled muris (iii), and in severe cases visible nexine layer (n) and bacula (b) due to absent tectum layer (iv).

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As the reduced number of pollen grains in ashh2 could also be due to defects in male meiosis, we inspected meiosis in ashh2-1, ashh2-2 and ashh2-5 lines using a whole-mount DAPI/Aniline Blue staining procedure. Tetrad number from each anther was very variable and generally lower in the mutant, however, examination of stages from the initial division of the pollen mother cells (PMC) up to early progamic development post meiosis did not reveal any apparent deviation from wt (Figure S3A). DAPI stained one-nucleated microspores were released from the tetrads (Figures S3A and S3B), but a variable number did not stain or hydrate in DAPI solution, indicating degeneration. After the first mitosis, some DAPI-stained microspores deviated slightly from wt in that generative nuclei appeared less compact and occasionally with two instead of one nucleolus (Figure S3C). At the trinucleate stage typically 25% of the pollen were DAPI stained (n = 65) compared to >99% in wt (n = 1290) (Figure S3D; viability was confirmed by Alexander staining.)

Especially in older flowers, dehiscence appeared to be delayed (Figure 4Bi). However, a low frequency of dehiscence occurred (Figure 4Bii and Figure S2A), releasing trinucleate pollen that could produce a pollen tube and appeared to be fully functional (Figure 4Biii).

pASHH2:GUS is expressed in the tapetum layer and in post-meiotic pollen

pASHH2:GUS plants were used to correlate the defects in anther and pollen development to ASHH2 expression patterns. No GUS expression was detected in the developing floral organ primordia or in pollen tetrads (Figure 4C and Figure 4D, insert). During early post-meiosis (floral stage 9) a weak signal could be detected in floral organs that persisted and increased in intensity at later stages (Figure 4D and 4E). Expression was found in anthers, as well as the gyneocium and mid veins of petals and sepals (Figure 4E). At stage 12, however, pASHH2:GUS was strongly expressed specifically in the maternal sporophytic tapetum layer accompanied by a less intense expression in the microspores (Figures 4F and 4G).

Exine deposition is affected in ashh2 pollen

As the tapetum layer contributes to pollen-wall synthesis and sporopollenin deposition, ashh2 pollen grains were inspected for changes in the exine layer using scanning electron microscopy (SEM) (Figures 4H and 4I). Wt pollen grains have an oval shape with two parallel furrows (Figure 4Hi) and an outer ordered exine lattice mainly composed of polymerized sporopollenin (Figure 4Hii). All four ashh2 alleles had abnormal pollen grains with overall irregular shape and an exine pattern deviating from the even reticulation of the wt (Figures 4I, Figure S4 and Table S3). The ridges (muri) were often flattened and more irregular with smaller spaces (lumina) that in some cases seem to be filled with material (Figures 4Iiii), and the reticulate tectum was in many cases incomplete or even totally absent giving the exine layer a spotted appearance (Figure 4Iiv and Figure S4).

Tapetal development is distorted in ashh2 mutant plants

Mutant anther development was studied in more detail using transmission electron microscopy (TEM), as many ashh2 anthers showed locules with a number of aberrations (Figure S2). During Early Ring Stage in the wt (Figure 5A) the microspores are free and the tapetum is actively synthesizing wall materials. In locules of ashh2-1 and ashh2-2 anthers, abnormal tapetal enlargement could be found at the corresponding stage (Figures 5D, 5G and 5J). During Pollen Mitosis I (PMI) to PMII (Figure 5B) active secretion of wall material occurs by the wt tapetum to form the exine layer, and the tapetal membrane degenerates. In the corresponding stage in ashh2-1 (Figure 5E), globular material accumulated in membrane-bound vesicles (arrow in 5E) that fused to form the major components of the tapetum (Figure 5F). In the ashh2-2 allele abnormal accumulation and deposition of pollen wall material were evident (Figures 5G and 5J and arrow in Figures 5H and 5K) leading to agglutination of the immature pollen grains. Immediately prior to dehiscence in the wt, the tapetum has fully degraded and the pollen coat has been deposited (Figure 5C). In contrast, the mutant tapetum and also the tapetal membrane persisted longer (Figure 5F and arrowhead in Figure 5E). In some cases severe deficiencies in the exine sculpturing and abnormal pollen wall development were observed (Figures 5I and 5L), consistent with the results from the SEM analysis (Figures 4I and Figure S4). Contrary to the distorted tapetum development, secondary thickening of the endothecium, degeneration of the middle cell layer, as well as stomium breakdown appeared normal in the mutant (Figure 5).

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Figure 5. TEM analysis of tapetal and pollen development in ashh2 and wt.

(A) Early Ring Stage with free microspores (M) in wt. Note the endothecium (E), tapetum (T) and intact middle cell layer (mc). (B) Pollen Mitosis I to Pollen Mitosis II in wt, degeneration of the middle cell layer has occurred. Note exine (ex) with visible defined bacula. (C) Immediately prior to dehiscence in the wt. Tapetal degeneration and deposition of pollen coat has occurred and endothecium (E) secondary thickening is visible. (D) Early Ring Stage in the ashh2-1 mutant displaying abnormal tapetal (T) enlargement. (E) Pollen Mitosis I to Pollen Mitosis II of ashh2-1 disclosing abnormal accumulations of lipid-like material in membrane bound vesicles (arrows) within the tapetal cells (T). Note that normal tapetal degeneration fails to occur and that the tapetal membrane is clearly visible (arrowhead). (F) Prior to dehiscence in the ashh2-1 mutant, normal endothecium secondary thickening (st) and thinning of the stomium (S) is seen. However the tapetal cells (T) are still present and release of the globular material previously visible (Figure 6E) has not occurred, suggesting that tapetal development is impaired and delayed. (G and J) Pollen Mitosis I to Pollen Mitosis II in the ashh2-2 mutant, note secondary thickening (st) of the endothecium and that degeneration of the middle cell layer has occurred. Exine formation (ex) with well-defined bacula is visible, however, the tapetum (T) appears enlarged with an abnormal accumulation of wall materials. (H and K) As pollen mitosis progresses in ashh2-2 abnormal deposition of pollen wall material is evident (arrow), resulting in agglutination of the immature pollen grains. In some cases a deficiency of the exine sculpturing is observed (arrowheads). (I and L) Prior to dehiscence in ashh2-2 normal breakdown of the stomium occurs, however abnormal pollen wall development is observed (arrow), resulting in some cases in extreme malformation of the pollen wall (L). Bars in A, H: 10 µm; C, D, E, G, L: 5 µm; B, J, K: 2 µm; F, I: 20 µm.

doi:10.1371/journal.pone.0007817.g005

Mutation in ASHH2 leads to substantial changes in inflorescence gene expression

Total RNA from wt and ashh2-1 young flowers and buds was used in a microarray experiment encompassing oligonucleotides representing ~27 000 unique genes aimed at identifying target genes for ASHH2 (see Materials and Methods) (Figure 6A). When controlling the false discovery rate (FDR) [17] in the statistical analysis at a 0.01 level, and using an absolute log2-ratio >0.7 as cut-off (i.e. up- or down-regulation 1.6 times), 348 genes were up-regulated and 637 down-regulated in ashh2-1 compared to wt.

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Figure 6. Changes in gene expression and histone tail methylation in the ashh2-1 mutant.

(A) Functional GO annotation of genes differentially expressed in ashh2-1 inflorescences relative to wt. The inserts depict the developmental stage of the main inflorescences used in the microarray experiment. (B) Number of co-down-regulated genes in the ashh2-1 mutant (>1.6-fold change), ms1 mutant (>2-fold change) and spl/ems-1 mutant (>1.6-fold change). (C) Confirmation of down-regulation of selected genes using real-time reverse transcriptase PCR. Wt levels were set to 1. (D) Gene structures of AtDMC1, AP1 and MYB99. Boxes indicate exons, thin lines introns. The positions of the fragments tested in the ChIP analyses are shown as red lines. (E) Representative results of ChIP analyses on the selected down-regulated genes shown in (D) using antibodies against H3K4me3, H3K36me2 and H3K4me3. Ta3 was used as a control. IN – input; –ab – without antibodies.

doi:10.1371/journal.pone.0007817.g006

These gene sets were analyzed with the TAIR GO annotation tool (http://www.arabidopsis.org/tools/bulk/go​/index.jsp). A higher proportion of the upregulated genes were related to biotic or abiotic stimulus or stress processes (11%) than the down-regulated genes (5%) (Figure 6A and Table S2), and only one of the up-regulated genes, MATERNAL EFFECT EMBRYO ARREST 38 (MEE 38), is known to be involved in reproductive processes [18]. In contrast, a number of the down-regulated genes are known to be involved in such processes (Table 3), e.g. ATDMC1 needed for meiosis [19]; ABORTED MICROSPORES (AMS) and MALE STERILE 2 (MS2), involved in tapetum function and anther dehiscence [20], [21].

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Table 3. Down-regulated genes in ashh2 inflorescences encoding transcription factors and factors involved in development.

doi:10.1371/journal.pone.0007817.t003

Twenty-three and 35 genes, respectively, encoding putative transcription factors (TFs) were up- and down-regulated (Figure 6A), however, several of these have undefined functions (Table 3). The most strongly down-regulated gene was the FLC-related MADS-BOX AFFECTING FLOWERING 1 (MAF1), which has been reported down-regulated in ashh2 seedlings [6], [7], [14], [22]. Likewise the highly similar and clustered genes MAF2-MAF5 [14], [22] were all down-regulated in the inflorescence sample (Table 3).

A number of genes are co-down-regulated in ashh2 and ms1 and/or spl/ems1 mutants

A network of genes controls anther development and function, including SPOROCYTELESS (SPL) which act very early in anther development, EXCESS MICROSPOROCYTES 1 (EMS1) involved in early tapetal initiation, and MALE STERILE 1 (MS1) needed for tapetal development and function. As the ashh2 mutants have a clear defect in pollen production we compared ashh2 mutant microarray data with array data for spl, ems1 and ms1 mutants [23], [24]. The expression levels of these genes themselves were not significantly altered in the ashh2 background, indicating that ASHH2 is not acting upstream of these genes, or acts in independent pathways. Only one gene was up-regulated in both the ashh2 and ms1 microarrays and only ten genes were co-upregulated in the ashh2 and spl/ems1 microarrays. In contrast, a significant number of genes showed coordinate down-regulation, suggesting downstream involvement in common pathways. Out of 1030 genes down-regulated in both spl and ems1, 144 (log2>0.7) were also down-regulated in ashh2 (Figure 6B). Of the 240 genes down-regulated more than two fold in ms1 [24], 46.3% (111 genes) were also down-regulated in ashh2 mutant inflorescences (Table S4). These encompass tapetum-specific genes encoding oleosins and lipases that together make up 90% of the detectable pollen coat protein [25], as well as the genes encoding the transcription factors MYB99, AtNAC25 and AtNAC5 suggested to be direct targets of MS1 [24], [26].

Genes associated with the ashh2 phenotype show a reduction in gene expression and H3K36 trimethylation

Genes that were down-regulated in the microarray experiment and potentially involved in different aspects of the ashh2 mutant phenotype showed consistent expression changes by real-time PCR (Figure 6C, Table 3). The expression levels of the AP1 and AP3 genes, encoding A and B floral organ identity factors, respectively, and the QRT3 and AtDMC1 genes, were reduced by 40 to 50%. MEE48 and UNE15 involved in female gametophyte development and function, as well as the tapetal TFs MYB99, AtNAC5 and AtNAC25 were down-regulated 60 to 70%.

Based on the ASHH2 protein's similarity to other ASH1-like proteins working as transcriptional co-activators [27] (Figure S5) and ChIP data from ashh2 non-reproductive tissue [6], [7], [12], [13], we expected genes that are potential direct target of ASHH2 to be down-regulated and to have changes in the level of histone H3 methylation at K4 and/or K36 in ashh2. Chromatin was isolated from inflorescences of young wt and ashh2-1 mutant plants, and precipitated using antibodies against H3K4me3, H3K36me2 and H3K36me3. Two to three biological replicas were used for each precipitation, and genes representing different aspects of the mutant phenotype (AP1 – floral organ identify; AtDMC1 – embryo sac development; MYB99 – pollen development, Figure 6D) were selected for ChIP analysis. In all cases no changes were seen for H3K4me3 or H3K36me2 (Figure 6E and Figure S6). In contrast, substantial reduction of H3K36me3 was revealed (Figure 6E and Figure S6) both relative to the input and the Ta3 retrotransposon used as a control [7], [28]. This suggests that ASHH2 regulates expression of these genes via H3K36 trimethylation.

Discussion

Mutations in ASHH2 lead to early flowering, have an obvious effect on shoot branching and were recently also shown to affect carotenoid composition (Figure 1H, Figure S1A and [6][8], [12], [13]. Here we have focused on the involvement of ASHH2 in the regulation of organ identity in the flower, and its role in ovule and anther development.

Floral homeotic changes correlate to down-regulation of homeotic genes in the first and second whorl

Floral organ identity is governed by the interplay between transcription factors expressed in the four whorls of the flower [29]. Mutations in whorl 1 and 2 expressed AP1 or AP2 genes leads to a spread of AG expression from whorl 3 and 4 and results in carpels in whorl 1 and stamen in whorl 2. Additional mutations in whorl 2 and 3 expressed AP3 or PI genes show a further conversion to carpeloid organs [30]. The observed homeotic changes of the floral organs in the ashh2 Col alleles as well as the esf1-1 Ler allele, with carpeloid organs in whorls 2 and 3, or conversion of sepals to carpels and petals to stamen (Figures 1K to 1M, Table S1), are in accordance with down-regulation of AP1, AP3 and PI in ashh2 inflorescences (Table 3, Figure 6C).

In mutants defective in the ATX1 gene encoding a H3K4 HMTase, floral homeotic genes are also down-regulated [10]. This may be an indirect effect, as H3K4me3 marks on the AP1 gene did not decrease in the atx1 flowers [31], [32]. In contrast, the down-regulation of AP1 in the ashh2 mutant was correlated with a reduction of the H3K36me3 level (Figure 6C and E).

ASHH2 is required for normal embryo-sac development

Reciprocal crosses of ASHH2/ashh2 heterozygous plants indicated that ASHH2 is needed for normal development or function of the haploid gametophytes (Figures 2A and 2B, Table 2). The sporophytic effect of a mutation in ASHH2 is, however, much more pronounced (Figures 2A and 2B), and has been the main focus in this work.

In homozygous ashh2 plants, mature ovules were devoid of an embryo sac (Figure 3B) and the majority of the embryo sacs arrested before the first syncytial nuclear division (Figure 3C). At premature stages, however, embryo sacs undergoing nuclear division could be observed (Figures 3D to 3I), and in these cases the embryo sacs were often protruding out of the ovule between underdeveloped integuments (Figures 3G to 3I). This could suggests that when nuclear proliferation takes place, the delayed elongation of outer integuments force the protruding embryo-sac structure out, causing it to eventually degenerate or “burst”. Such expulsion of the female gametophyte has been previously described for the clotho (clo) mutant, and is suggested as a mechanism to hamper allocation of maternal resources to sterile tissue [33]. However, these researchers demonstrated expulsion of mature female gametophytes 3 days after emasculation, and our results indicate that this mechanism also can act at earlier developmental stages. pASHH2:GUS expression was found both in the integuments and in the young nucellus where the MMC form (Figures 2E and 2F), supporting a function for ASHH2 both in ovule development and pre- or post-meiotic sporophytic contribution to the generation of the female gametophyte. Occasionally, however, normal progression through female meiosis occurred in the mutant since homozygous lines could generate a low frequency of vital seeds.

There are hundreds of mutants defective in embryo sac formation [34], but only in a few cases the affected genes have been identified. The observed ashh2 phenotype resembles that of the mutants pretty few seeds 2 (pfs2), sporocyteless/nozzle (spl/nzz) and atdmc1 [19], [35], [36]. Only atdmc1 was down-regulated in our microarray experiment (Table 3 and Figure 6C). We consider it likely, however, that additional down-regulated, yet unidentified genes also contribute to the ashh2 mutant embryo sac and ovule phenotype.

The atdmc1 mutant is defective in female and male sporogenesis due to severely distorted chromosomal segregation, but still allows a low seed set (1.5% of wt) [19], [37]. In ashh2, down-regulation of atdmc1 possibly takes place only in the female reproductive organ as pASHH2:GUS expression was not detected in pollen tetrads (insert Figure 4D), and meiosis appeared normal (Figure S3). Down-regulation of AtDMC1 in the ashh2 female organ is, however, likely since pASHH2:GUS was detected where the MMC form (Figure 2E). The down-regulation is accompanied with a reduction of the H3K36m3 level (Figure 6C and E).

At the fully developed ovule stage the spl/nzz mutant phenotype resembles that of ashh2, but in contrast to ashh2, spl/nzz is characterized by the absence of a MMC at an early stage of ovule development, thus preventing embryo sac formation [36].

ASHH2 is required for normal anther differentiation, tapetum development and pollen maturation

On the male side mutation of SPL/NZZ result in a lack of initial division of the archesporial cells that leads to the primary parietal layer, thus pollen sacs and PMCs do not differentiate [36]. This resembles the ashh2 phenotype, where about a quarter of the anthers do not develop proper locules (Figure 4B and Figure S2). However, we have no indications that ASHH2 works directly through SPL/NZZ as no down-regulation of this gene was seen in our microarray experiment, and locule development and meiosis occur, albeit always producing a reduced number of microspores (Figures 4A and 4B). The defect in pollen production is likely to result from aberrations in tapetal layers from PMI onwards with accumulation of vesicles, abnormalities in the secretion of wall materials and delayed degeneration (Figures 5D to 5L and Figure S2). By the dehiscence stage severe distortions and collapse of pollen wall could be observed with deformed or absent bacula and tectum (Figures 5L, 4I and Figure S4). This may either be due to delayed cell wall deposition or altered wall composition as the expression data showed down-regulation of pollen coat-related genes, e.g. the oleosin genes (Table S4). A similar down-regulation of these genes is seen in the ms1 mutant, which also presents defective late pollen wall and coat development [38]. Delay in tapetal development was not necessarily reflected in delay of other aspects of anther development, like dehiscence (Figure 5, Figure S2A), suggesting a lack of synchrony and coordinated regulation in the development of the different anther tissues.

Transcriptional profiling suggests that ASHH2 has a broad effect on transcription factors controlling development

Ten percent of the genes down-regulated in ashh2 inflorescences encoded either transcription factors or DNA or RNA binding proteins (Figure 6A). Many of these, e.g. the B3 TFs, have not yet been assigned a specific biological function (Table 3), and the significance of their down-regulation in the ashh2 mutant cannot be evaluated at present. Similarly, the function of the most likely redundant MAF genes in the inflorescence is unknown.

In contrast to genes upregulated in ashh2 inflorescences, there is a substantial overlap between genes down-regulated in the ms1 and the ashh2 mutants. This overlap might reflect the sum of anther defects, however, all ms1 affected genes are not down-regulated in the ashh2 inflorescences, suggesting that the co-regulated subset is part of a genetic network controlled by both ASHH2 and MS1. Down-regulated genes that are common for ashh2 and spl/nzz, but not ms1, e.g. MS2, AMS and its putative interacting partner ASHR3 [20], [21], [39], can be assumed to partake in genetic networks operating earlier than, or in parallel to, MS1 during anther development.

Since the microarray suggested that MS1 and SPL/NZZ themselves are not down-regulated in the ashh2 mutant one hypothesis could be that the ASHH2 protein works together with MS1 and/or SPL/NZZ to control their direct target genes. Consistent with this hypothesis is the down-regulation in ashh2 background of the presumed direct targets of MS1, the transcription factors MYB99 and AtNAC25 [24], [26] (Figure 6C), as well as reduction of H3K36me3 on MYB99 chromatin (Figure 6E).

Changes in histone tail marks in ashh2 mutant plants suggest ASHH2 to work via H3K36me3 in reproductive development

So far the exact substrate and product specificities of ASHH2 have not been demonstrated in vitro, possibly because some other unknown modification on the histone tails is a prerequisite for ASHH2's activity. ASHH2 has been implicated in H3K4me3 methylation on the CAROTENOID ISOMERASE gene and in the FLC promoter region [6], [13]. The latter has been suggested to be due to collaboration between ASHH2 and ATX1/ATX2 [40]. ASHH2 seem to be of more general importance for H3K36 methylation as substantial reduction in the global levels of H3K36me2 and me3, as well as H3K36me3 reduction in all gene specific regions tested so far in ashh2 mutants have been shown [7], [12], [14]. The reduced H3K36me3 levels we have found for AtDMC1, AP1 and MYB99 in ashh2 mutant inflorescences (Figure 6E) are consistent with a role for ASHH2 in H3K36 trimethylation.

The amino acid sequence of the SET domain and surroundi ng regions of ASHH2 have high similarity to H3K36me3 methyltransferases in yeast (Set2), Drosophila (dSet2) and mammals (Setd2/HYBP) [41][44] (Figure S5), which have been implicated in inhibition of transcriptional initiation within coding regions, DNA replication check-pointing, prevention of spreading of neighboring heterochromatin, and involvement with pre-mRNA splicing [45], [46]. These Set2 homologues interact with the C-terminal domain (CTD) of DNA Polymerase II via their Set2 Rpb1-interacting (SRI) region [47], which is not conserved in plant ASHH2 homologues. Thus it remains to be seen whether ASHH2 functions in the same way as any of these enzymes in its control of reproductive organ formation and other aspects of Arabidopsis growth and development.

Materials and Methods

Plant material

Arabidopsis plants were normally cultivated in growth chambers at 20°C for 8h of dark and 16 h of light (100 µE·m−2 s−1). The T-DNA insertion lines SALK_65480, SALK_026442, SALK_36941 and SALK_040477 were genotyped to establish homozygous lines, and these were designated ashh2-1, ashh2-2, ashh2-5 and ashh2-6. ashh2-1 and -2 are identical to lines designated sdg8-1 and -2 by [7]. The exact positions of the T-DNA insertions were identified from sequenced PCR products of the T-DNA/plant DNA junctions.

pASHH2:GUS lines

An ASHH2 promoter fragment encompassing 1211 bp upstream of the ATG start codon was amplified using the primers prom-GUS Ashh2 attB1 and prom-GUS Ashh2 attB2 and introduced into the pDONR/Zeo Gateway entry vector and thereafter recombined into the promoterless GUS destination vector pMDC162 [48], generating the construct pASHH2:GUS. Transgenic Arabidopsis plants were produced by the floral dip method [49].

GUS staining and whole-mount clearing preparations of plant organs were performed as described [50].

n situ hybridization

For in situ hybridization, an ASHH2 1 kb PCR product generated with the primers 2135L and 3115R was cloned into the vector pCR IV-TOPO (Invitrogen, Carlsbad, CA) and used as templates for dioxigenin-11-UTP labelling (Roche Molecular Biochemicals, Indianapolis, IN) of RNA probes. The ASHH2 antisense RNA probe was synthesized using T3 RNA polymerase after linearization with NotI, and the sense control probe was synthesized with T7 RNA polymerase after linearization with SpeI. Plant fixation and in situ hybridization were performed according to [51].

Microscopy

For Scanning Electron Microscopy (SEM) pollen grains from homozygous ashh2 plants and wt pollen were harvested directly on a stub, coated with gold palladium in a sputter-coater, and inspected using a high-vacuum Scanning Electron Microscope (SEM) JEOL JSM 6400.

For Transmission Electron Microscopy (TEM) whole inflorescences were fixed and processed according to [38]. Individual buds were embedded in LR White resin (TAAB) and ultra-thin (50–70 nm) sections were cut and collected on uncoated 200 hexagonal mesh copper grids (TAAB). Sections were double stained with saturated uranyl acetate in 50% (v/v) ethanol and Reynolds lead citrate and examined under a FEI Tecnai 12 Biotwin TEM. Semi-thin sections (0.5 µm) were cut and stained with toluidine blue (0.05% w/v) for light microscopy observation of anthers using a Nikon OPTIPHOT.

For ovule and embryo sac morphology, material was fixed and processed as described previously [50] and analyzed by differential interference contrast light microscopy (DIC).

For anther and pollen morphology, whole inflorescences were fixed in 4% paraformaldehyde in 1x PBS, pH 6.9 at room temperature and 10 mmHg for 1 h, washed twice for 10 min in 1 x PBS. Single anthers were mounted in staining buffer (1xPBS, 5% DMSO, and 0.01% Tween 20) containing combinations of 0.1 mg/mL propidium iodide, 2 mg/mL DAPI, or 0.01% (w/v) aniline blue and inspected in a Zeiss Axioplan2 imaging microscope equipped with epifluorescence. Pollen viability was confirmed by Alexander staining [52].

Microarray experiment and data analysis

Five biological replicas with 12 plants each, of both wt and the ashh2-1 mutant were sown out on soil and grown under the following conditions; 22°C day and 18°C night, 16 h day length with 30 min adjustment of light to on and off, and 85 µE m−2 s−1 in light intensity. The inflorescences of each biological repeat were harvested in bulk at same developmental stage (Figure 6A) and total RNA was extracted using RNeasy midi kit (Qiagen).

Gene expression profiles for ashh2 inflorescences were compared to their wt counterparts using two-color microarrays and statistical analysis according to [53]. Differentially expressed genes (Table S5) identified using the limma software package [54]. All parts of the data analysis were performed using R [55]. All data are MIAME compliant and that the raw data has been deposited in the MIAME compliant database GEO (http://www.ncbi.nlm.nih.gov/geo/query/ac​c.cgi?acc=GSE18325).

Real-time quantitative PCR

Total RNA was treated with DNase I (Takara) followed by RNA Cleanup with RNeasy (Qiagen). Ten µg DNase treated total RNA were used for a double cDNA synthesis reaction with oligo-dT primers and SuperScript™ III Reverse Transcriptase (Invitrogen). RNA was removed from the cDNA by adding 2u of E. coli RNaseH (Takara). PCR reactions (5 µL diluted cDNA, 0.3 µM forward and reverse primers, 10.0 µL SYBR® Premix Ex Taq™ (Takara)) were performed on a LC480 Light Cycler (Roche). The cycling conditions were: 10 s 95°C followed by 45 cycles of 4 s 95°C, 20 s 60°C, 15 s 72°C. Experiments were performed in three biological replicates, two technical replicates and cDNA dilution series of 50 ng, 20 ng and 5 ng. Crossing point (CP) values were generated using 2nd derivative calculation software (LC480). Expression levels of target genes in the ashh2 mutant were calculated relative to wt levels with normalization to ACTIN2, using the formula RE = EtargetΔCPtarget (wt- ashh2)]/Eactin[(ΔCPactin (wt – ashh2)], where target represents the target gene analyzed.

Gene specific primers for real-time PCR were designed using Roche Probe Library Primer Design or the Primer Design tool in the Vector NTI software (Invitrogen) (see Table S6).

ChIP

ChIP was essentially performed as described in [56]. 1.5 g of inflorescences from young plants was put under vacuum for 40 min in 37 ml of 1% formaldehyde to crosslink the chromatin. After addition of 2.5 ml 2M Glycine, the inflorescences were put under vacuum for additional 5 min to stop crosslinking and then rinsed twice in water, frozen in liquid N2 and grinded in a mortar. After extraction from the inflorescences, the chromatin was sonicated for 4 min on setting H (15 sec on, 15 sec off) in a Bioruptor UCD-200 sonicator (Diagenode). Chromatin was precleared using Protein A agarose beads (Upstate) and immunoprecipitated over night using 5 µl of antibody against H3K4me3 (#07-473, Upstate), H3K36me2 (#07-369, Upstate) or H3K36me3 (ab9050, Abcam). Immunoprecipitated DNA was analyzed by RT-PCR using primers against MYB99, AtDMC1 and AP1 (Table S5). The Ta3 retrotransposon was used as a control [7], [28] for equal precipitation of non-target chromatin with the different antibodies. Two to three biological replicas were used for each antibody. Two to three PCR replicas were used per primer set.

Accession Numbers

ASHH2 - At1g77300, SPL/NZZ – At4g27330, EMS1 - At5g07280, MS1 - At5g22260, FLC - At5g10140. Accession numbers of other genes discussed, are found in Table 3.

Supporting Information

Figure S1.

Phenotype of ashh2 mutant plants.

doi:10.1371/journal.pone.0007817.s001

(0.12 MB PDF)

Figure S2.

Light microscopy of ashh2-1 mutant anthers immediately prior to dehiscence.

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(0.14 MB PDF)

Figure S3.

Pollen meiosis in ashh2 mutants.

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(0.07 MB PDF)

Figure S4.

Scanning electron micrographs of ashh2-2, ashh2-5 and ashh2-6 pollen grains and exine layers.

doi:10.1371/journal.pone.0007817.s004

(0.69 MB PDF)

Figure S5.

Alignment of the ASHH2 SET domain to SET domains of related proteins.

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(0.41 MB PDF)

Figure S6.

Changes in histone tail methylation in the ashh2-1 mutant.

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(0.09 MB PDF)

Table S1.

Frequency of homeotic transformations in different ashh2 alleles.

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(0.03 MB PDF)

Table S2.

Up-regulated genes in ashh2 inflorescences encoding transcription factors and factors involved in development.

doi:10.1371/journal.pone.0007817.s008

(0.10 MB PDF)

Table S3.

Percentage of pollen showing abnormal exine layers.

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(0.02 MB PDF)

Table S4.

Genes down-regulated in ashh2 inflorescences and ms1 young buds.

doi:10.1371/journal.pone.0007817.s010

(0.13 MB PDF)

Table S5.

Up- and down-regulated genes in inflorescences from the ashh2 mutant compared to wt.

doi:10.1371/journal.pone.0007817.s011

(0.87 MB XLS)

Table S6.

List of primers.

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(0.13 MB PDF)

Acknowledgments

We thank Barbro Sæther, Roy Falleth, Charles Albin-Amiot and Solveig H. Engebretsen for technical assistance, Francois Roudier and Vincent Colot for introducing V.A. to their ChIP protocol, and Tove Bakar and Torill M. Rolfsen at the Electron Microscopy Laboratory at Department of Molecular Biosciences, University of Oslo, where the SEM work has been performed. We are grateful for the effort of Torfinn Sparstad, Herman Midelfart, Per Winge and Atle Bones at the microarray service unit of the Norwegian Arabidopsis Research Centre (NARC, http://www.narc.no/).

Author Contributions

Conceived and designed the experiments: PEG TT VA RBA. Performed the experiments: PEG TT VA GVB SSW. Analyzed the data: PEG TT VA GVB SSW TJ ZW RBA. Wrote the paper: PEG ZW RBA.

References

  1. 1. Turner BM (2002) Cellular memory and the histone code. Cell 111: 285–291.
  2. 2. Zegerman P, Canas B, Pappin D, Kouzarides T (2002) Histone H3 lysine 4 methylation disrupts binding of nucleosome remodeling and deacetylase (NuRD) repressor complex. J Biol Chem 277: 11621–4.
  3. 3. Rozovskaia T, Tillib S, Smith S, Sedkov Y, Rozenblatt RO, et al. (1999) Trithorax and ASH1 interact directly and associate with the trithorax group-responsive bxd region of the Ultrabithorax promoter. Mol Cell Biol 19: 6441–6447.
  4. 4. Jenuwein T, Laible G, Dorn R, Reuter G (1998) SET domain proteins modulate chromatin domains in eu- and heterochromatin. Cell Mol Life Sci 54: 80–93.
  5. 5. Baumbusch LO, Thorstensen T, Krauss V, Fischer A, Naumann K, et al. (2001) The Arabidopsis thaliana genome contains at least 29 active genes encoding SET domain proteins that can be assigned to four evolutionarily conserved classes. Nucl Acids Res 29: 4319–4333.
  6. 6. Kim SY, He Y, Jacob Y, Noh YS, Michaels S, et al. (2005) Establishment of the vernalization-responsive, winter-annual habit in Arabidopsis requires a putative histone H3 methyl transferase. Plant Cell 17: 3301–3310.
  7. 7. Zhao Z, Yu Y, Meyer D, Wu C, Shen WH (2005) Prevention of early flowering by expression of FLOWERING LOCUS C requires methylation of histone H3 K36. Nat Cell Biol 7: 1156–1160.
  8. 8. Soppe WJ, Bentsink L, Koornneef M (1999) The early-flowering mutant efs is involved in the autonomous promotion pathway of Arabidopsis thaliana. Develop 126: 4763–4770.
  9. 9. Dennis ES, Peacock WJ (2007) Epigenetic regulation of flowering. Curr Opin Plant Biol 10: 520–527.
  10. 10. Alvarez-Venegas R, Pien S, Sadder M, Witmer X, Grossniklaus U, et al. (2003) ATX-1, an Arabidopsis homolog of Trithorax, activates flower homeotic genes. Curr Biol 13: 627–37.
  11. 11. He Y, Doyle MR, Amasino RM (2004) PAF1-complex-mediated histone methylation of FLOWERING LOCUS C chromatin is required for the vernalization-responsive, winter-annual habit in Arabidopsis. Genes Devel 18: 2774–2784.
  12. 12. Dong G, Ma D-P, Li J (2008) The histone methyltransferase SDG8 regulates shoot branching in Arabidopsis. Biochemi Biophys Res Commun 373: 659–664.
  13. 13. Cazzonelli CI, Cuttriss AJ, Cossetto SB, Pye W, Crisp P, et al. (2009) Regulation of carotenoid composition and shoot branching in Arabidopsis by a chromatin modifying histone methyltransferase, SDG8. Plant Cell 21: 39–53.
  14. 14. Xu L, Zhao Z, Dong A, Soubigou-Taconnat L, Renou J-P, et al. (2008) Di- and tri- but not monomethylation on histone H3 lysine 36 marks active transcription of genes involved in flowering time regulation and other processes in Arabidopsis thaliana. Mol Cell Biol 28: 1348–1360.
  15. 15. Howden R, Park SK, Moore JM, Orme J, Grossniklaus U, et al. (1998) Selection of T-DNA-tagged male and female gametophytic mutants by segregation distortion in Arabidopsis. Genetics 149: 621–631.
  16. 16. Schneitz K, Hülskamp M, Pruitt RE (1995) Wild-type ovule development in Arabidopsis thaliana: a light microscope study of cleared whole-mount tissue. Plant J 7: 731–749.
  17. 17. Benjamini Y, Hochberg Y (1995) Controlling the false discovery rate: a practical and powerful approach to multiple testing. J R Stat Soc Ser B 57: 289–300.
  18. 18. Pagnussat GC, Yu HJ, Ngo QA, Rajani S, Mayalagu S, et al. (2005) Genetic and molecular identification of genes required for female gametophyte development and function in Arabidopsis. Develop 132: 603–614.
  19. 19. Couteau F, Belzile F, Horlow C, Grandjean O, Vezon D, et al. (1999) Random chromosome segregation without meiotic arrest in both male and female meiocytes of a dmc1 mutant of Arabidopsis. Plant Cell 11: 1623–1634.
  20. 20. Aarts MG, Hodge R, Kalantidis K, Florack D, Wilson ZA, et al. (1997) The Arabidopsis MALE STERILITY 2 protein shares similarity with reductases in elongation/condensation complexes. Plant J 12: 615–623.
  21. 21. Sorensen AM, Krober S, Unte US, Huijser P, Dekker K, et al. (2003) The Arabidopsis ABORTED MICROSPORES (AMS) gene encodes a MYC class transcription factor. Plant J 33: 413–23.
  22. 22. Ratcliffe OJ, Kumimoto RW, Wong BJ, Riechmann JL (2003) Analysis of the Arabidopsis MADS AFFECTING FLOWERING gene family: MAF2 prevents vernalization by short periods of cold. Plant Cell 15: 1159–1169.
  23. 23. Wijeratne AJ, Zhang W, Sun Y, Liu W, Albert R, et al. (2007) Differential gene expression in Arabidopsis wild-type and mutant anthers: insights into anther cell differentiation and regulatory networks. Plant J 52: 14–29.
  24. 24. Yang C, Vizcay-Barrena G, Conner K, Wilson ZA (2007) MALE STERILITY1 is required for tapetal development and pollen wall biosynthesis. Plant Cell 19: 3530–3548.
  25. 25. Mayfield JA, Fiebig A, Johnstone SE, Preuss D (2001) Gene families from the Arabidopsis thaliana pollen coat proteome. Science 292: 2482–2485.
  26. 26. Ito T, Nagata N, Yoshiba Y, Ohme-Takagi M, Ma H, et al. (2007) Arabidopsis MALE STERILITY1 encodes a PHD-type transcription factor and regulates pollen and tapetum development. Plant Cell 19: 3549–3562.
  27. 27. Kouzarides T (2007) Chromatin modifications and their function. Cell 128: 693–705.
  28. 28. Schmitz RJ, Tamada Y, Doyle MR, Zhang X, Amasino RM (2009) Histone H2B deubiquitination is required for transcriptional activation of FLOWERING LOCUS C and for proper control of flowering in Arabidopsis. Plant Physiol 149: 1196–1204.
  29. 29. Coen ES, Meyerowitz EM (1991) The war of the whorls: genetic interactions controlling flower development. Nature 353: 31–37.
  30. 30. Robles P, Pelaz S (2005) Flower and fruit development in Arabidopsis thaliana. Int J Dev Biol 49: 633–643.
  31. 31. Saleh A, Al-Abdallat A, Ndamukong I, Alvarez-Venegas R, Avramova Z (2007) The Arabidopsis homologs of Trithorax (ATX1) and Enhancer of zeste (CLF) establish ‘bivalent chromatin marks’ at the silent AGAMOUS locus. Nucl Acids Res 35: 6290–6296.
  32. 32. Saleh A, Alvarez-Venegas R, Avramova Z (2008) Dynamic and stable histone H3 methylation patterns at the Arabidopsis FLC and AP1 loci. Gene 423: 43–47.
  33. 33. Moll C, von Lyncker L, Zimmermann S, Kägi C, Baumann N, et al. (2008) CLO/GFA1 and ATO are novel regulators of gametic cell fate in plants. Plant J 56: 913–921.
  34. 34. Schneitz K, Hulskamp M, Kopczak SD, Pruitt RE (1997) Dissection of sexual organ ontogenesis: a genetic analysis of ovule development in Arabidopsis thaliana. Development 124: 1367–1376.
  35. 35. Park SO, Zheng Z, Oppenheimer DG, Hauser BA (2005) The PRETTY FEW SEEDS2 gene encodes an Arabidopsis homeodomain protein that regulates ovule development. Development 132: 841–849.
  36. 36. Schiefthaler U, Balasubramanian S, Sieber P, Chevalier D, Wisman E, et al. (1999) Molecular analysis of NOZZLE, a gene involved in pattern formation and early sporogenesis during sex organ development in Arabidopsis thaliana. Proc Natl Acad Sci USA 96: 11664–11669.
  37. 37. Klimyuk VI, Jones JDG (1997) AtDMC1, the Arabidopsis homologue of the yeast DMC1 gene: characterization, transposon-induced allelic variation and meiosis-associated expression. The Plant Journal 11: 1–14.
  38. 38. Vizcay-Barrena G, Wilson ZA (2006) Altered tapetal PCD and pollen wall development in the Arabidopsis ms1 mutant. J Exp Bot 57: 2709–2717.
  39. 39. Thorstensen T, Grini PE, Mercy IS, Alm V, Erdahl S, et al. (2008) The Arabidopsis SET domain protein ASHR3 is involved in stamen development and interacts with the bHLH transcription factor ABORTED MICROSPORES (AMS). Plant Mol Biol 66: 47–59.
  40. 40. Pien S, Fleury D, Mylne JS, Crevillen P, Inze D, et al. (2008) ARABIDOPSIS TRITHORAX1 dynamically regulates FLOWERING LOCUS C activation via histone 3 lysine 4 trimethylation. Plant Cell 20: 580–588.
  41. 41. Adhvaryu KK, Morris SA, Strahl BD, Selker EU (2005) Methylation of histone H3 lysine 36 is required for normal development in Neurospora crassa. Eukar Cell 4: 1455–1464.
  42. 42. Chu Y, Sutton A, Sternglanz R, Prelich G (2006) The Bur1 cyclin-dependent protein kinase is required for the normal pattern of histone methylation by Set2. Mol Cell Biol 26: 3029–3038.
  43. 43. Morris SA, Shibata Y, Noma K-i, Tsukamoto Y, Warren E, et al. (2005) Histone H3 K36 methylation is associated with transcription elongation in Schizosaccharomyces pombe. Eukar Cell 4: 1446–1454.
  44. 44. Stabell M, Larsson J, Aalen RB, Lambertsson A (2007) Drosophila dSet2 functions in H3-K36 methylation and is required for development. Biochemical and Biophysical Research Communications 359: 784–789.
  45. 45. Kim HS, Rhee DK, Jang YK (2008) Methylations of histone H3 lysine 9 and lysine 36 are functionally linked to DNA replication checkpoint control in fission yeast. Biochem Biophys Res Commun 368: 419–425.
  46. 46. Tompa R, Madhani HD (2007) Histone H3 lysine 36 methylation antagonizes silencing in Saccharomyces cerevisiae independently of the Rpd3S histone deacetylase complex. Genetics 175: 585–593.
  47. 47. Kizer KO, Phatnani HP, Shibata Y, Hall H, Greenleaf AL, et al. (2005) A novel domain in Set2 mediates RNA polymerase II interaction and couples histone H3 K36 methylation with transcript elongation. Mol Cell Biol 25: 3305–3316.
  48. 48. Curtis MD, Grossniklaus U (2003) A Gateway cloning vector set for high-throughput functional analysis of genes in planta. Plant Physiol 133: 462–469.
  49. 49. Clough SJ, Bent AF (1998) Floral dip: a simplified method for Agrobacterium-mediated transformation of Arabidopsis thaliana. Plant J 16: 735–743.
  50. 50. Grini PE, Jurgens G, Hulskamp M (2002) Embryo and endosperm development is disrupted in the female gametophytic capulet mutants of Arabidopsis. Genetics 162: 1911–1925.
  51. 51. Jackson D (1992) In situ hybridization in plants. In: Bowles DJ, editor. Plant molecular pathology: a practical approach. Oxford, UK: Oxford University Press. pp. 163–174.
  52. 52. Alexander MP (1969) Differential staining of aborted and nonaborted pollen. Stain technol 44: 117–122.
  53. 53. Kusnierczyk A, Winge P, Midelfart H, Armbruster WS, Rossiter JT, et al. (2007) Transcriptional responses of Arabidopsis thaliana ecotypes with different glucosinolate profiles after attack by polyphagous Myzus persicae and oligophagous Brevicoryne brassicae. J Exp Bot 58: 2537–2552.
  54. 54. Smyth GK (2004) Linear models and empirical Bayes methods for assessing differential expression in microarray experiments. Statistical Applications in Genetics and Molecular Biology 3:
  55. 55. R Development Core Team (2007) R: A language and environment for statistical computing. r foundation for statistical computing, vienna, austria (http://www.r-project.org), ISBN 3-900051-07-0.
  56. 56. Gendrel A-V, Lippman Z, Martienssen R, Colot V (2005) Profiling histone modification patterns in plants using genomic tiling microarrays. Nat Meth 2: 213–218.