• We are sorry, but NCBI web applications do not support your browser and may not function properly. More information
Logo of plntphysLink to Publisher's site
Plant Physiol. Apr 2011; 155(4): 2066–2080.
Published online Feb 11, 2011. doi:  10.1104/pp.110.169813
PMCID: PMC3091125

Whole Genome Analysis of Gene Expression Reveals Coordinated Activation of Signaling and Metabolic Pathways during Pollen-Pistil Interactions in Arabidopsis1,[C][W]


Plant reproduction depends on the concerted activation of many genes to ensure correct communication between pollen and pistil. Here, we queried the whole transcriptome of Arabidopsis (Arabidopsis thaliana) in order to identify genes with specific reproductive functions. We used the Affymetrix ATH1 whole genome array to profile wild-type unpollinated pistils and unfertilized ovules. By comparing the expression profile of pistils at 0.5, 3.5, and 8.0 h after pollination and applying a number of statistical and bioinformatics criteria, we found 1,373 genes differentially regulated during pollen-pistil interactions. Robust clustering analysis grouped these genes in 16 time-course clusters representing distinct patterns of regulation. Coregulation within each cluster suggests the presence of distinct genetic pathways, which might be under the control of specific transcriptional regulators. A total of 78% of the regulated genes were expressed initially in unpollinated pistil and/or ovules, 15% were initially detected in the pollen data sets as enriched or preferentially expressed, and 7% were induced upon pollination. Among those, we found a particular enrichment for unknown transcripts predicted to encode secreted proteins or representing signaling and cell wall-related proteins, which may function by remodeling the extracellular matrix or as extracellular signaling molecules. A strict regulatory control in various metabolic pathways suggests that fine-tuning of the biochemical and physiological cellular environment is crucial for reproductive success. Our study provides a unique and detailed temporal and spatial gene expression profile of in vivo pollen-pistil interactions, providing a framework to better understand the basis of the molecular mechanisms operating during the reproductive process in higher plants.

Seeds develop as a result of sexual reproduction in plants, a process relying on a series of complex signaling interactions collectively known as the progamic phase. Despite apparent anatomical simplicity, the pistil plays a central role in the success of this process. Its structure is precisely adapted to bear the female gametophyte and to act in a way that influences pollen tube growth (Boavida et al., 2005a, 2005b; Feijó, 2010). The first pollen-stigma recognition event involves molecules present on both partner surfaces to promote pollen adhesion and subsequent hydration (Hiscock and Allen, 2008). Upon germination, the pollen tube grows from the stigma through the style and ovary tissues, where localized cellular interactions potentially define unique phases or checkpoints for pollen tube guidance. In flowering plants, compatible signaling molecules and chemical gradients produced by the female diploid tissues were identified as playing major roles supporting pollen tube growth and guidance along their way within the pistil (Cheung et al., 1995; Wu et al., 1995; Palanivelu et al., 2003; Dong et al., 2005), while more precise signals emitted by the female gametophyte should act as short-range attractants guiding pollen tubes into their final target, the embryo sac (Shimizu and Okada, 2000; Higashiyama et al., 2006). Specific signal interactions between pollen tubes and the embryo sac determine the final guidance steps toward sperm cell release into the embryo sac (Huck et al., 2003; Rotman et al., 2003; Higashiyama et al., 2006), a process that seems to be at least partially controlled by the female gametophyte (Escobar-Restrepo et al., 2007).

Knowledge about signaling pathways that operate during pollen tube growth following self-incompatible and compatible pollinations has increased considerably in recent years (Hiscock and Allen, 2008), but the molecular basis underlying the production of female signals, and how pollen tubes perceive and decode them to correctly target the embryo sac, remain largely unknown. The transcriptional profiles of pollen (Becker et al., 2003; Honys and Twell, 2003, 2004; Pina et al., 2005; for review, see Becker and Feijó, 2007), embryo sac (Yu et al., 2005; Johnston et al., 2007; Jones-Rhoades et al., 2007; Steffen et al., 2007), pistil (Scutt et al., 2003; Tung et al., 2005), and embryo or seed developmental stages (Chen et al., 2001; Hennig et al., 2004; Yoshida et al., 2005, Le et al., 2010) were recently analyzed. More notably, recent progress in the isolation of Arabidopsis (Arabidopsis thaliana) gametes allowed genome-wide expression profiling of purified sperm cells (Borges et al., 2008) as well as of isolated egg and central cells (Wuest et al., 2010). In addition, the transcriptomes of in vitro pollen tube growth (Wang et al., 2008) and of pollen tubes growing in a semi-in vitro system (Qin et al., 2009) unfolded a new level of complexity of gene regulation occurring during the reproductive process. However, the analysis of individual partners or particular cellular processes cannot provide a complete outline of the molecular events acting during plant reproduction, in that they do not fully represent the way that individual elements relate with each other in vivo in a precise timing and developmental context. To address this question, we used the Affymetrix ATH1 whole genome array to profile gene expression in unpollinated pistils (UP) and dissected unfertilized ovules, based on comparative transcriptomics with different tissues. In addition, the same technology was used to analyze the kinetics of gene regulation along several time points that could represent the most significant developmental events from pollination to fertilization. By combining these approaches with thorough bioinformatics analysis, we could identify 1,373 genes whose behavior would be compatible with crucial roles needed to ensure fertilization. This study represents, to our knowledge, the first microarray-based approach on pollen-pistil interactions using a complete in vivo system, thus providing a more comprehensive view into the complex signaling and genetic networks underlying sexual plant reproduction.


Prediction of Stage-Specific and Reproductive Organ-Enriched Transcripts

The reproductive process involves the regulation of cellular interactions that occur between the male gametophyte (pollen/male gametes), diploid female sporophytic tissues, and the female gametophyte (embryo sac/female gametes). Our first approach aimed to identify stage-specific and/or stage-enriched transcription in UP and unfertilized ovules, which are the more relevant organs in terms of cellular interactions occurring after pollination. The UP expression profile should include transcripts that are abundantly expressed in stigmatic and transmitting tissue (TT) cells that may function to support and modulate pollen tube growth. Similarly, the expression profiles of ovules should show enrichment for transcripts expressed in the female gametophyte but also in other sporophytic transcripts that may be equally important for pollen tube growth modulation or guidance. A primary transcriptomic comparison of UP, ovules, and siliques enriched the UP and ovule data sets for stage-specific transcripts by excluding common sporophyte-expressed genes potentially involved in carpel and ovule determination, such as SEEDSTICK (STK; Rounsley et al., 1995) and SHATTERPROOF1 (SHP1; Flanagan et al., 1996), a phosphogluconolactonase (At5g24420) that is expressed in ovule integuments and in the ovary wall (Scutt et al., 2003), as well as genes involved in later stages of seed development, such as MEDEA (MEA;Vielle-Calzada et al., 1999), FERTILIZATION INDEPENDENT SEED2 (Luo et al., 1999), and FLOWERING WAGENINGEN (Kinoshita et al., 2004). Using the parameters outlined in “Materials and Methods” and further comparison with publicly available data sets (Zimmermann et al., 2004; Tung et al., 2005; Yu et al., 2005; Steffen et al., 2007; Borges et al., 2008; Wang et al., 2008; Qin et al., 2009; Wuest et al., 2010), a total of 42 genes were considered enriched or preferentially expressed in ovules (Supplemental File S1). As anticipated, 27 out of 42 transcripts preferentially expressed in ovules and 96 out of 1,275 ovule-enriched transcripts were previously reported to be expressed specifically in the embryo sac or enriched in female gametophytic cells (Supplemental File S1; Yu et al., 2005; Johnston et al., 2007; Punwani et al., 2007; Steffen et al., 2007; Wuest et al., 2010). Ovule-expressed transcripts likely include plausible candidates for short-range pollen tube attractants expressed in the embryo sac (Higashiyama et al., 2001, 2003; Chen et al., 2007; Okuda et al., 2009) but also of other modulators expressed in the surrounding sporophytic tissues that could function as long-range pollen tube attractants. UP express the lowest number of enriched transcripts (340), due to the exclusion of overlapping transcript expression with mature siliques. Among these, we confirmed the detection of 17 UP-enriched transcripts previously reported to be expressed in receptive stigma or TT (Supplemental File S1; Scutt et al., 2003; Wellmer et al., 2004; Tung et al., 2005).

Analysis of the major functional classes represented in UP-enriched transcripts reveals as predominant classes cell wall biosynthesis and regulation (4.7%), stress- and defense-related transcripts (8.8%), transcription (13.2%), and development (6.3%; Table I). Although much of the constitutive expression in pistils is represented by stress and defense-related genes (Scutt et al., 2003; Lan et al., 2004), these transcripts likely encode proteins that, in addition, may perform functions in the modulation of pollen tube growth. On the other hand, transcription-, cell cycle-, and DNA processing-related transcripts are major functional classes in the ovule-enriched data set. Overrepresented functional categories in transcripts preferentially expressed in ovules include cell wall biosynthesis (8.7%), development (10.9%), and cell fate (4.3%) as well as a significant number of unclassified transcripts (50%; Table I), while components of signal transduction and cellular transport were surprisingly poorly represented in these data sets. Yet, apparently lacking tissue or cell specificity at the expression level, many of these signal transduction components may still perform crucial functions during pollen-pistil interactions. As an example, the FERONIA gene, which encodes a receptor-like kinase required for pollen tube reception (Escobar-Restrepo et al., 2007), is under gametophytic selection, albeit being also expressed in siliques, seedlings, and leaves.

Table I.
Functional classification of UP, ovules, and pollen-expressed transcripts

Gene Regulation Underlying the Progamic Phase

In order to identify genes involved in cell-cell communication, we generated expression profiles for three distinct time points after pollination assumed to represent important time frames for biological switches on the nature of cell-to-cell interactions along the pollen tube pathway. In Arabidopsis, within the first half-hour after pollination (0.5HAP), most pollen grains have hydrated, germinated, and invaded the stigmatic papilla cells. At 3.5HAP, pollen tubes are growing through the style TT cells, and at 8.0HAP, few pollen tubes might be in their final guidance stages to or interacting with the embryo sac, but most ovules are fertilized.

In order to analyze global expression patterns, we used principal component analysis (PCA), projected onto the first three principal components (Fig. 1A). The first principal component captures the highest variance among samples (42.9%) and underlines the unique expression profiles of UP, 0.5/3.5HAP and 8.0HAP, undoubtedly revealing major transcriptional changes occurring in response to pollination. The data sets of 0.5HAP and 3.5HAP are more similar to each other than to any other, suggesting that this particular stage, corresponding to pollen tube growth in the TT of the style, has a distinct transcriptional profile compared with other stages. The second and third principal components explain the remaining variance between samples, accentuating the differences between all time points. A similar separation of the samples could be obtained with clustering analysis (Fig. 1B). The time-course expression profiles were then compared with each other using UP as baseline and a more stringent cutoff (lower confidence bound of fold change [LCB] ≥ 1.5; P < 0.01) to increase biological significance. We found 1,298 genes regulated at least in one of the time points after pollination. Regulated genes include those that showed a significant change in expression between two consecutive time points as well as genes in which the kinetics of regulation was slower. Therefore, a significant change in gene expression was only detected in nonconsecutive time points. We hypothesized that some of the enriched pollen transcripts could be highly diluted in female sporophytic tissues during in vivo growth. Using a lower cutoff (LCB ≥ 1.2), we identified 75 additional transcripts identified initially as enriched or preferentially expressed in the pollen data sets.

Figure 1.
PCA and hierarchical clustering of time-course transcriptome data. A, PCA is an exploratory technique used to describe the structure of high-dimensional data (e.g. derived from microarrays) by reducing its dimensionality. Here, expression values for approximately ...

In total, we detected significant changes in the expression of 1,373 genes from pollination to fertilization. A comparison between tissue and time-course expression allowed us to determine that 78% (1,066) of the regulated transcripts were first expressed before pollination in UP or unfertilized ovules, 7% (96) were exclusively induced by pollination (absent in any other tissue directly involved in the reproductive process), 12% (170) represent transcripts identified initially as preferentially expressed in our pollen data set (absent from UP or ovules), and 3% (36) were enriched (Supplemental File S2). Despite the predominant expression of genes in the pistil at receptivity, only a few proteins expressed in the sporophytic female tissues were identified with functions in pollen-pistil interactions (Wu et al., 2000; de Graaf et al., 2003; Palanivelu et al., 2003; Park and Lord, 2003), and only one gene was identified to be strictly induced by pollination (Bui and O’Neill, 1998).

The comparison of our time-course data set with recently reported transcriptomes of in vitro (Wang et al., 2008) and semi-in vitro pollen tube growth (Qin et al., 2009) confirmed an expected overlap of multiple genes “de novo” transcribed during pollen tube growth and possibly induced due to interactions with the female tissues. This overlap includes 13 genes classified in our data sets as “induced by pollination,” 129 as “expressed before pollination,” and 103 already identified as preferentially expressed and/or enriched in the pollen data sets. Yet, 119 regulated genes classified as pollen enriched and/or preferentially expressed in the initial data sets were not represented in the in vitro or semi-in vitro transcriptomes. These include genes predominantly up- or down-regulated upon interactions with the TT of the style (0.5HAP versus 3.5HAP), genes in which significant changes in gene expression were detected in nonconsecutive time points (i.e. there was a gradual change in expression from 0.5HAP up to 8.0HAP), and genes in which transcriptional changes occur in later stages of pollen tube growth in the ovary (3.5HAP versus 8.0HAP). These may represent either pollen-expressed genes modulated in later stages (Supplemental File S2) or genes elicited in female tissues upon pollen tube interaction with the ovary TT, ovules, or embryo sac (3.5–8.0 HAP), conditions that were not considered in any of the previous studies. These transcripts may thereby function in both pollen and pistil tissues to ensure a proper fertilization.

Using cluster analysis, the 1,373 transcripts were grouped in 16 distinct time-course clusters according to their expression patterns (Fig. 2; Supplemental File S3). Even though it was initially thought that the success of the reproductive process would depend predominantly on down-regulation of pistil-expressed transcripts (Chen et al., 2001; Lan et al., 2004), recent genome-wide analyses in rice (Oryza sativa) and Arabidopsis contributed to change this perspective (Endo et al., 2004; Hennig et al., 2004). Our time-course analysis further reveals that pronounced transcriptional changes take place in response to pollination, and these involve the concerted activity of multiple genes that ultimately follow distinct patterns of regulation. In fact, 46% of the transcripts are regulated at least in one time point after pollination, 38% are consistently up-regulated (clusters 6, 8, and 9), while only 16% (clusters 13 and 14) are continuously down-regulated after pollination (Fig. 2). As an example, clusters 1 and 2 show a biphasic regulation: these transcripts are induced as fast as 0.5HAP, down-regulated during pollen tube growth in TT, and induced again at 8.0HAP. On the other hand, in clusters 7, 10, 11, and 12, transcripts are preferentially induced at 3.5HAP; in clusters 3 and 4, transcripts are slowly down-regulated during pollen tube growth in the stigma and TT but are specifically up-regulated at 8.0HAP; while clusters 15 and 16 seem to include transcripts predominantly down-regulated with a slight induction in later stages of fertilization (Fig. 2). Therefore, each cluster contains a group of dynamically coregulated transcripts, likely performing specific functions in particular cellular interactions between pollen tubes and female tissues (i.e. stigma, style, or ovary). While most clusters consist of genes that are involved in varied biological functions, other clusters seem to contain transcripts involved in more specific functions (Supplemental Table S1). Interestingly, cluster 2 contains a significant representation of metabolism and energy-related transcripts as well as a unique enrichment of unclassified proteins, while cluster 10 is almost exclusively represented by transcripts related to cell wall and cell fate. Clusters 15 and 16 denote a slight up-regulation at 8.0HAP, which is associated with the enrichment of cell wall- and cytoskeleton-related transcripts, cell cycle, DNA processing, and transcription, as well as a large number of unclassified proteins possibly associated with the termination of pollen tube growth, fertilization, or the initiation of early zygote/embryo development.

Figure 2.
Clustering analysis of the time-course profile of pollen-pistil interactions. The expression values of 1,373 genes were normalized to the baseline (UP; time 0), and the ratios were log2 transformed to reveal expression kinetics. Genes were clustered using ...

Microarray Data Validation

For validation of our microarray analyses, we followed distinct approaches: (1) overlapping our microarray data sets with the literature, both in terms of transcriptomics and single gene profile studies; (2) reverse transcription (RT)-PCR analysis of candidate genes to confirm tissue expression or regulatory patterns within different gene clusters (Fig. 3); and (3) characterization of gene and enhancer trap insertion lines (Fig. 4). Among 1,373 genes regulated during the reproductive process, we selected 36 genes with relatively high expression levels and for which the change in expression in consecutive or nonconsecutive time points could potentially be detected by RT-PCR (greater than 1.3-fold change).

Figure 3.
RT-PCR analysis of genes regulated during pollen-pistil interactions. A, Confirmation of changes in expression for several regulated genes during the time course. B, Expression of several time-course-regulated genes classified as EBP (expressed before ...
Figure 4.
Histochemical detection of GUS enzymatic activity in gene trap (DsG) and enhancer trap (DsE) lines. A, Young pistils were emasculated and pollinated 24 h later. GUS activity was assayed at specific time points after pollination (0, 3.5, and 8.0 HAP) for ...

Comparison of our data sets with the literature confirmed that the expression patterns of several of the regulated genes were consistent with the described functions in pollen tube growth or guidance. Such examples include the Arabidopsis plantacyanin (At2g02850; Dong et al., 2005) and the well-known POP2 gene (At3g22200) encoding a transaminase involved in the degradation of γ-aminobutyrate (Palanivelu et al., 2003), which are up-regulated after pollination with a decrease in expression in later stages of pollen tube growth (Fig. 5). Consistently up-regulated are general genes with known functions in pollen germination and tube growth, such as Vanguard1 (At2g47040; Jiang et al., 2005) and No Pollen Germination1 (At2g43040; Golovkin and Reddy, 2003; Fig. 5). Other examples include the RopGEFs known to interact with leucine-rich repeat (LRR) kinases during pollen tube growth in the pistil (Kaothien et al., 2005). In our data sets, we identified two pollen-specific RopGEFs (Zhang and McCormick, 2007), RopGEF12 (At1g79860) and RopGEF11 (At1g52240), both of which are up-regulated during pollen tube growth (cluster 9). Interestingly, two out of six up-regulated LRR kinases are preferentially expressed in pollen and follow a similar regulatory pattern (cluster 9). One is the ortholog of LePRK2 (for pollen receptor-like kinase), AtPRK2a (At2g07040), recently found to interact with RopGEF12 (Zhang and McCormick, 2007). The second pollen LRR (At1g49490; Fig. 3) may represent the ortholog of LePRK1. However, several crucial molecular players in this signaling pathway are still missing (Wengier et al., 2010), namely those expressed in the female partner tissues. It is plausible that this particular gene cluster (cluster 9) may contain other partner components of this complex signaling transduction pathway, namely the most wanted pistil ligand.

Figure 5.
Predictions of subcellular localization for proteins regulated during pollen-pistil interactions. Wedges indicate the percentage of proteins assigned to each subcellular localization according to The Arabidopsis Information Resource 9.0 prediction. Whole ...

The expected expression patterns of several potential candidates encoding unknown, cell wall-, and signaling-related components were confirmed by RT-PCR (Fig. 3). We validated the expected gene expression in 94% of the 144 independent contrast points tested (36 genes in four time points) and confirmed the expected regulatory trend for all four time points in 27 out of the 36 genes. Examples of this validation include transcripts induced in response to pollination, such as a MYB transcription factor (At1g56650, PAP1), which is elicited at 0.5HAP and then down-regulated during pollen tube growth in the TT and ovary, or of a glycosyltransferase (At5g54060, UF3GT) strongly induced by pollination (Fig. 3). We obtained a similar confirmation (94%) for tissue expression. From 132 independent contrasts tested (22 genes in six different tissues), only nine showed discrepancies in expression (approximately 6%), seven of which were in seedlings. We think that the discrepancies observed in seedling expression may reflect biological variation and may be due to different developmental stages used in the microarray data sets and in the RT-PCR. In a few cases, we were able to detect a faint band by RT-PCR in saturation conditions upon 35 cycles of amplification for some transcripts called absent by the MAS5 algorithm, suggesting limitations in the sensitivity of microarrays to detect very low expressed genes. In addition to the RT-PCR, we selected 12 transposon lines from a collection of gene (DsG) and enhancer trap (DsE) lines (Sundaresan et al., 1995; Supplemental Table S2). These lines were selected based on availability, position, and orientation of the GUS construct within the genes as well as differential expression along the time course. No phenotypical defects in plant fertility or deviation in kanamycin resistant/kanamycin sensitive (KanR/KanS) segregation ratios (3:1) were associated with any of the insertion lines. GUS activity was only detected in inflorescence tissue of four lines, GT17927, GT11110, ET222, and ET10301, with insertions in At3g10020, At3g25170 (RAFL26), At4g16146, and At3g49270, respectively (Supplemental Table S2). The changes in gene expression during the time course were confirmed in pollinated pistils and monitored by GUS staining (Fig. 4).

GT17927 corresponds to an insertion in the first exon of At3g10020, an unknown gene that, according to our microarray data, was highly expressed in UP but down-regulated after pollination. GUS expression was detected in stigma and style TT as well as in ovary and weakly in the sporophytic tissues of ovules, consistent with the pathway taken by the pollen tubes. The GUS expression clearly decreases after pollination, being almost undetectable at 8.0HAP (Fig. 4A), suggesting a possible role during pollen tube growth or guidance. A reduction of the expression level expected for At4g16146 was less evident in ET222, where GUS expression was predominant in pollen and stigma throughout the time course analyzed. The transposon was confirmed to be inserted in an intron but in an opposite orientation to the At4g16146 coding region; thus, GUS localization for this line might not be as comprehensible. However, it is possible that the GUS expression could be induced by a proximal enhancer sequence derived, for example, from an antisense transcript. In the GT11110 and ET10301 insertion lines, the transposons are located in the exons of RALFL26 (for rapid alkalinization factor-like family-like 26; At3G25170) and an unknown protein (At3g49270), respectively. In both lines, GUS staining was not detected in UP but was present in mature pollen (Fig. 4B, l and p). A slight GUS activity was detected in the stigma at 3HAP, while at 8HAP, when most pollen tubes have discharged their cytoplasmic contents in the embryo sac, GUS expression significantly increased in stigma papilla (GT11110 and ET10301; Fig. 4, A and B) and in the upper part of the TT (GT11110; Fig. 4A), confirming up-regulation of these genes in female tissues, as expected from the microarray data. The regulation of GUS activity in these insertion lines is compatible with a function of the targeted genes in the support or modulation of pollen tube growth. In the GT11110 and ET10301 insertion lines, the gene function might be associated with postpollination responses such as cell wall modifications or degradation of proteins related to pistil receptivity.

Based on these results, we conclude that our microarray data reflect with confidence the dynamics and strict regulatory control occurring during pollen-pistil interactions and can be used to predict potential molecular interactions associated with specific cellular events during the reproductive process and in terms of temporal clustering patterns (Fig. 2).

Swinging Partners: Regulation of Signal Transduction and Cell Wall

Cell-to-cell communication between pollen tubes and their partner cells in the pistil involves signaling events that take place across cell walls. The kinetics of regulation observed in the time-course experiment supports the hypothesis that many of the regulated transcripts (transcripts in which a change in abundance was detected across the different time points; greater than 1.2-fold change) may be locally produced to mediate specific interactions between the pollen tube and particular cell types of the pistil. During pollen tube growth, the pistil extracellular matrix plays a variety of roles in addition to its structural function. It can act as a conductor of signals, as a source of signals, and also as an extracellular domain for plasma membrane receptors (Brownlee, 2002). On the ATH1 genome array, about 17% of the probe sets represent transcripts encoding proteins predicted to contain an N-terminal signal peptide, and according to our data set, 30% of the regulated transcripts encode proteins predicted to follow the secretory pathway (Fig. 5). These are similarly represented in transcripts “expressed before pollination” (27%), “induced after pollination” (38%), or in the subset of transcripts identified in the pollen data sets as “enriched and preferentially expressed” in pollen but that can also have been induced in pistil tissues during pollen tube growth (37%). Many of these genes encode for small proteins that are likely to function as ligands or extracellular signal molecules. Such examples include transcripts belonging to the clavata family (CLE21), the phytosulfokine 1 precursor (PSK1), a low-molecular-weight Cys-rich protein (LCR59), the COBRA-like family (COBL5, COBL6, COBL10), and members of the RALFL family (At4g14020, RALFL4, RALFL9, RALFL18, RALFL26), some of which are preferentially enriched in the female gametic cells and are induced during later stages of pollen tube growth in the ovary (Supplemental File S4; Jones-Rhoades et al., 2007; Wuest et al., 2010). Interestingly, a 15-amino acid secreted peptide (C-terminally encoded peptide 1), which was shown to cause growth arrest when applied externally to roots (Ohyama et al., 2008), seems to be induced at 8.0HAP.

Based on the classification of the Cell Wall Genomics (http://cellwall.genomics.purdue.edu/) database, 131 (9.5%) of the regulated genes represent cell wall-related components. Overrepresented families include members of the polygalacturonase family, glucorosyltransferases, glycosyl hydrolases, expansins, extensins, arabinogalacturans (AGPs) and fasciclins, COBRAs, pectate lyases, and pectinesterases (Fig. 6A). These proteins, in particular glycosylphosphatidylinositol-anchored proteins, are thought to play important roles in cell wall remodeling, cell expansion, or mediating cell-to-cell signaling interactions (Borner et al., 2003). Among these, we identified seven predicted AGPs, four pistil expressed (AGP2, AGP6, AGP7, AGP23) and three preferentially expressed or enriched in pollen (AGP11, AGP22, AGP40). Additionally, we identified five fasciclins, four expressed in the pistil (FLA1, FLA2, FLA7, FLA15) and one pollen specific (FLA3). Fasciclins were implicated in growth cone guidance in Drosophila (Grenningloh et al., 1991) as well as signaling via Tyr kinases (Elkins et al., 1990) and represent good candidates to function as receptors or cell adhesion molecules. We also found that 89 (6.5%) of the regulated transcripts encode signal transduction components. Overrepresented families include the 14-3-3 proteins, calcium- and calmodulin-related proteins, CRPK1L, LRRs, Pro-rich and extensin-like kinases, RALFLs, receptor-like cytoplasmic kinases, and members of the two-component signaling transduction system (Fig. 6B). Receptor kinases located at the plasma membrane are particularly interesting, since they transduce external signals via activated signaling pathways (Morris and Walker, 2003). Such examples include the PRKs belonging to the LRR family involved in the regulation of pollen tube growth in tomato (Solanum lycopersicum) and petunia (Petunia hybrida; Muschietti et al., 1998; Tang et al., 2004), but so far, no receptor kinases were identified in the female tissues. Here, we identify several kinases expressed in female tissues. This induction (or regulation) in different time points and/or expression in a particular tissue is compatible with a possible function in a specific cellular stage during the reproductive process (Fig. 5; Supplemental Table S4).

Figure 6.
Signal transduction and cell wall families regulated during pollen-pistil interactions. A, Cell wall families. B, Signal transduction families. Values represent percentages of genes assigned to each family on the ATH1 array and regulated during pollen-pistil ...

These localized cellular interactions are known to define unique checkpoints along the pollen tube pathway in self-compatible crosses. However, these interactions are also often the reason for the failure of a successful fertilization upon self-incompatible or interspecific and intergeneric crosses (Higashiyama et al., 2006; Escobar-Restrepo et al., 2007). Understanding the molecular basis of postpollination events in compatible crosses will undoubtedly provide new insights in how self-incompatibility and interspecific responses are regulated, as evidence emerges supporting an intrinsic link between the cellular pathways operating in both systems (Samuel et al., 2009).

Signal Integration and Cross Talk: The Key for Reproductive Success?

Several metabolic pathways were differentially regulated during the progamic phase. Components of PSI and PSII light-harvesting complex systems and chlorophyll-associated genes were predominantly down-regulated, indicating a general trend to shut down photosynthesis during pollen tube growth (clusters 13 and 14). Other components of metabolic pathways, such as the glycolytic and starch degradation pathways, general carbohydrate and polysaccharide metabolism, phosphate, amino acid, secondary metabolism (phenylpropanoid, stilbenes, and flavonoids), and hormone metabolism, were positively regulated (clusters 5–9).

Based on the Arabidopsis Transcription Factors Database (http://arabidopsis.med.ohio-state.edu/), 84 transcription factors are regulated during the reproductive process. Several transcription factor families were significantly represented in the data set, such as bHLH, MYB, ARR, GRAS, GRF, SBP, TVP trihelix, and ABI3/VP1, while several other members, such as YABBY and MADS box transcription factor families, which were previously reported to be important during the reproductive process (Hennig et al., 2004), were poorly represented or absent. It is possible that the function of these transcription factors may be related to carpel and ovule development, since the previous study compared immature pistils, fertilized pistils, and siliques, while our analysis was performed on a shorter temporal developmental window (time course of 8 h). Some of these transcription factors are coexpressed in different clusters (Supplemental File S5), suggesting that they might be involved in the regulatory control of particular genetic pathways, alone or through combinatory interactions (Singh, 1998). As an example, TCP21, REM16, and two MYB transcription factors (MYB70 and MYB123) may represent the major regulators of clusters 2 and 3 (Supplemental File S5).

Among the regulated transcripts, we found a significant representation of transcriptional regulators, receptors, response factors, and transporters related to hormonal regulation (Supplemental Fig. S1, A–C). Hormones usually do not function in discrete pathways but rather exhibit extensive cross talk and signal integration with each other and with environmental and developmental signaling pathways (Lorenzo et al., 2003; Nemhauser et al., 2004). Therefore, their dynamic regulation may indicate that a precise control of the local concentrations for defined hormonal metabolites might be essential to regulate downstream signaling events along the pollen tube pathway. Several studies suggested that certain hormones such as ethylene, auxin, brassinosteroids, and methyl jasmonate could act as primary signals in the pollination response (O’Neill, 1997). Supporting an important role of hormones in the success of the reproductive process (Aloni et al., 2006; Chen and Zhao, 2008), we identified several biosynthetic and signaling-related components of the auxin (Supplemental Fig. S1B) and ethylene (Supplemental Fig. S1C) pathways within the classes expressed before pollination, which seem to be differentially regulated or induced in specific stages of pollen tube growth. A good example of auxin/ethylene cross talk is the induction during pollen tube growth in the style of a 1-aminocyclopropane-1-carboxylate synthase (At4g37770), a main component of ethylene biosynthesis and known to be auxin responsive (Supplemental Fig. S1C; Supplemental File S2). Cross talk of cytokinin and auxin in the regulation of cell division is another well-known process, namely in specific cell-cycle transitions (Hartig and Beck, 2006). This cross talk seems to be important for the regulation of expression and activity of CdkA at the G2/M transition (Sorrell et al., 2001) and to induce the expression of the D3 cyclins at the G1/S transition (Riou-Khamlichi et al., 1999). Our data show that the regulatory kinetics of cytokinin-related genes (Supplemental Fig. S1A) resembles mostly that found in cluster 1, where there is also a significant enrichment for transcripts related to cell cycle and DNA processing. According to the classification of Shultz et al. (2007), 16 out of 48 ATH1-represented transcripts encode proteins associated with DNA replication regulated during the reproductive process (Table II). Interestingly, with the recent description of Arabidopsis male and female gamete transcriptomes, we verified that, in fact, many of these transcripts are enriched in sperm cells (Borges et al., 2008) and expressed in the egg and central cell (Wuest et al., 2010; Table II). This is exemplified by a cytokinin-induced CYCD3;1 (At4g34160), known as a key regulatory element for the G1/S transition of the cell cycle (Menges et al., 2006), and a member of CdkA, CYCA2;4 (At1g80370), known as a major regulator of the G1/S checkpoint. Both are down-regulated during early stages of pollen tube growth in the pistil but up-regulated at 8.0HAP. Given this association, an involvement of these transcripts, either in synchronization of female and male gametes in the cell cycle prior to fertilization and karyogamy (Friedman, 1999) or upon successful fertilization during early zygote and endosperm patterning, is plausible.

Table II.
Time-course regulation of genes assigned to cell cycle and DNA processing


A spatial and temporal transcriptional study was performed in order to follow variations in gene expression and de novo transcription through different cellular events occurring from pollination to fertilization. This way, we could complement earlier work that focused on individual transcriptomes of isolated gametophytes or on specific aspects of pollen tube growth with that of a complete in vivo time-series profiling that analyzes the regulation of genes of all biological players in specific cellular events. Consequently, we were able to identify 1,373 transcripts differentially regulated up to 8 h after pollination. Namely, we identified several signaling and cell wall-related transcripts whose regulation over time and preferential expression in a particular reproductive tissue may be correlated with activation in a specific cellular event during the reproductive process. Our results also suggest that pathways responsible for the production of certain metabolites and hormones require a precise molecular control and balanced distribution, ensuring the correct physiological and metabolic cellular environment for the success of the reproductive process. We believe that our results can provide a roadmap to detailed genetic dissection of the progamic phase.


Plant Material and Growth Conditions

Seeds of Arabidopsis (Arabidopsis thaliana ecotype Columbia [Nottingham Arabidopsis Stock Centre]) were sown on soil and kept for 3 d at 4°C in the dark to promote seed stratification. Seedlings were grown in short-day conditions (8 h of light/16 h of dark at 22°C–24°C) for 2 weeks and then transferred to long-day conditions (16 h of light/8 h of dark at 22°C–24°C) to induce flowering. Flowers at developmental stage 12c (Smyth et al., 1990) were emasculated 24 h before pollination. Pistils were collected at 0, 0.5, 3.5, and 8 HAP and immediately frozen in liquid nitrogen. Two pistils from each time point were collected and stained with 0.1% decolorized aniline blue (Martin, 1959) as a control for pollen tube growth. Unfertilized ovules were collected by the funiculus from dissected UP and immediately frozen in liquid nitrogen. To minimize biological variation, 20 pistils were collected from a minimum of 10 plants, and for ovule isolation, 50 pistils were used from about 30 plants to isolate approximately 1,500 ovules for each replicate experiment.

RNA Isolation, Target Synthesis, and Hybridization to Affymetrix GeneChips

Total RNA was extracted from tissues using the RNeasy Mini Plant Kit (Qiagen). Concentration and purity were determined by spectrophotometry, and integrity was confirmed using an Agilent 2100 Bioanalyzer with an RNA 6000 Nano assay (Agilent Technologies). RNA was processed for use on Affymetrix Arabidopsis ATH1 Genome Arrays, according to the manufacturer’s Small Sample Labeling Protocol version II, described by Pina et al. (2005). Arrays were scanned in Affymetrix GeneChip scanner 2500.

GeneChip Data Analysis

We used the Arabidopsis ATH1 GeneChip representing 22,392 unique genes to obtain the transcriptional profiles of UP and unfertilized ovules and of pistils at 0.5, 3.5, and 8.0 HAP. Scanned arrays were analyzed first with Affymetrix MAS 5.0 software to obtain absent/present calls, and subsequent analysis was performed with dChip 1.3 (http://www.dchip.org; Wong Laboratory, Harvard University), applying the normalization parameters described by Pina et al. (2005). To ensure reliability of the analyses, each GeneChip experiment was performed with two biological replicates.

For the identification of reproductive organ-specific and -enriched genes, we combined our samples with data sets from leaves, seedlings, pollen, and siliques (Pina et al., 2005) to identify stage-specific reproductive organ-enriched genes.

Two main criteria were used to define with high stringency the set of genes showing differential expression between these experimental data sets. As an independent analysis method, significance analysis of microarrays (http://www-stat.stanford.edu/~tibs/SAM; Department of Statistics, Stanford University; Tusher et al., 2001; Storey, 2002, Leek et al., 2006) was used in the normalized signal intensities to detect significant differences in gene expression using pairwise comparisons, with a false discovery rate cutoff of 0.5% or less, to reveal genes showing differential gene expression. Next, to conservatively choose genes that showed consistent expression changes between tissues, we selected transcripts for which the absolute value of the LCB was above 1.2-fold, as discussed elsewhere (Pina et al., 2005; Johnston et al., 2007), to identify 18,413 genes showing significant expression changes for organ-enriched genes. Genes preferentially expressed in particular tissues were defined if present in only one of the tissues analyzed, based on comparisons of our samples with previous microarray data (Pina et al., 2005). Genes considered preferentially expressed were then uploaded on Genevestigator software (Zimmermann et al., 2004) and compared with high-quality arrays from the AtGenExpress database (Schmid et al., 2005), from experiments representing different developmental stages of Arabidopsis. Samples containing carpels, flowers, seeds, and siliques were excluded. Using the Digital Northern tool, genes called present with P < 0.05 in at least two of the three replicates were excluded from the preferentially expressed organ data sets. Transcripts that fulfilled the first criterion but were called present in at least one other tissue were classified as enriched. The remaining genes were scored as expressed. However, for the ovule data sets, a careful analysis was performed to identify genes preferentially expressed in a particular organ due to a possible overlap in gene expression between the UP and ovule data sets. We hypothesized that highly expressed transcripts in ovule would be detected in UP with a relative dilution effect. To identify those genes, we estimated the relative contribution of ovule gene expression to UP, based on genes only called present in ovules (43 genes). The average expression value was calculated and compared with the value obtained for the same set of genes in UP. Based on this difference, the contribution of genes preferentially expressed in ovules was estimated at 46% ± 13%. Thus, ovule-enriched transcripts in which the ratio UP-ovule was less than the threshold (less than 46%) and called present in UP and ovules represent transcripts preferentially expressed in ovules (48 genes). For the time-course analysis, significant analysis of microarrays for time-course experiments (EDGE; Leek et al., 2006) and a false discovery rate of 0.5% or less were used to identify 5,225 genes with significant expression changes in the time-course data set. A more stringent value of LCB ≥ 1.5 was used for the time-course analysis to better ensure biological significance. The LCB index was used rather than “fold change” because LCB takes the spread of the data into account and thus is a more robust index for the prediction of transcriptional changes (Li and Hung Wong, 2001). The coefficient of variation obtained after statistical treatment was found to be less than 0.05 between each pair of biological replicate experiments, revealing consistently good quality of the data.

PCA and hierarchical clustering of time-course experiments was performed using Partek Genomics Suite 6.07 (Partek). For hierarchical clustering analysis, Pearson’s dissimilarity was used to calculate row dissimilarity and Ward’s method was used for row clustering. To group genes with similar expression patterns, clustering analysis was performed using the Self-Organizing Tree Algorithm (SOTA; Herrero et al., 2001), available as a Web-based resource in GEPAS (for Gene Expression Profile Analysis Suite 1.1; http://gepas.bioinfo.cipf.es/; Herrero et al., 2003). Annotations for the 22,325 genes represented on the Arabidopsis ATH1 Genome Array are based on Gene Ontology annotations of The Arabidopsis Information Resource release 8. Genes were classified into functional categories using the Munich Information Center for Protein Sequences functional classification scheme using Virtual Plant 1.0 (http://virtualplant.bio.nyu.edu/cgi-bin/vpweb2/).

Time-course regulation of auxin and ethylene-related transcripts were represented using an adapted version of the auxin (Lau et al., 2008) and ethylene (Olmedo et al., 2006) pathways and displayed using MAPMAN application software (Thimm et al., 2004).

RT-PCR Analysis

Nonhybridized complementary RNA from one replicate of each sample used for the time-course analysis (UP and pistils at 0.5HAP, 3.5HAP, and 8.0HAP) and additionally from ovules, pollen, silique, leaf, and seedling samples were reverse transcribed using the SuperScript II system (Invitrogen) according to the manufacturer’s instructions with random primers in a 20-μL reaction. Five nanograms of each template cDNA was used in a standard PCR of 35 cycles. The sequences of all primers and the description of the genes tested by RT-PCR are available in Supplemental Table S2.

GUS Staining

Twelve genes represented in the time-course clusters were selected according to significant variation of gene expression pattern and availability in the collection of DsE and DsG trap lines at Cold Spring Harbor Laboratory (http://genetrap.cshl.org/; Sundaresan et al., 1995). The tagged genes were confirmed by TAIL-PCR using degenerated and Ds-specific primers as described by Liu et al. (1995; Supplemental Table S2). Time-course pollinations were performed as described before for the microarray experiments, and the GUS expression pattern was monitored in dissected pistils at 0, 3.5, and 8.0 HAP. For GUS staining, the samples were processed as described previously by Sundaresan et al. (1995) but excluding the potassium ferricyanide and ferrocyanide agents.

All microarray data were submitted to Gene Expression Omnibus (http://www.ncbi.nlm.nih.gov/geo/) under the series accession number GSE27281.

Supplemental Data

The following materials are available in the online version of this article.


  • Aloni R, Aloni E, Langhans M, Ullrich CI. (2006) Role of auxin in regulating Arabidopsis flower development. Planta 223: 315–328 [PubMed]
  • Becker JD, Boavida LC, Carneiro J, Haury M, Feijó JA. (2003) Transcriptional profiling of Arabidopsis tissues reveals the unique characteristics of the pollen transcriptome. Plant Physiol 133: 713–725 [PMC free article] [PubMed]
  • Becker JD, Feijó JA. (2007) How many genes are needed to make a pollen grain? Lessons from transcriptomics. Ann Bot (Lond) 100: 1117–1123 [PMC free article] [PubMed]
  • Boavida LC, Becker JD, Feijó JA. (2005a) The making of gametes in higher plants. Int J Dev Biol 49: 595–614 [PubMed]
  • Boavida LC, Vieira AM, Becker JD, Feijó JA. (2005b) Gametophyte interaction and sexual reproduction: how plants make a zygote. Int J Dev Biol 49: 615–632 [PubMed]
  • Borges F, Gomes G, Gardner R, Moreno N, McCormick S, Feijó JA, Becker JD. (2008) Comparative transcriptomics of Arabidopsis sperm cells. Plant Physiol 148: 1168–1181 [PMC free article] [PubMed]
  • Borner GH, Lilley KS, Stevens TJ, Dupree P. (2003) Identification of glycosylphosphatidylinositol-anchored proteins in Arabidopsis: a proteomic and genomic analysis. Plant Physiol 132: 568–577 [PMC free article] [PubMed]
  • Brownlee C. (2002) Role of the extracellular matrix in cell-cell signalling: paracrine paradigms. Curr Opin Plant Biol 5: 396–401 [PubMed]
  • Bui AQ, O’Neill SD. (1998) Three 1-aminocyclopropane-1-carboxylate synthase genes regulated by primary and secondary pollination signals in orchid flowers. Plant Physiol 116: 419–428 [PMC free article] [PubMed]
  • Chen D, Zhao J. (2008) Free indole-3-acetic acid in stigmas and styles during pollen germination and pollen tube growth of Nicotiana tabacum. Physiol Plant 234: 202–215 [PubMed]
  • Chen W, Tang D, Suo J, Zhang Y, Xue Y. (2001) Expressional profiling of genes related to pollination and fertilization in rice. C R Acad Sci III 324: 1111–1116 [PubMed]
  • Chen Y-H, Li H-J, Shi D-Q, Yuan L, Liu J, Sreenivasan R, Baskar R, Grossniklaus U, Yang W-C. (2007) The central cell plays a critical role in pollen tube guidance in Arabidopsis. Plant Cell 19: 3563–3577 [PMC free article] [PubMed]
  • Cheung AY, Wang H, Wu HM. (1995) A floral transmitting tissue-specific glycoprotein attracts pollen tubes and stimulates their growth. Cell 82: 383–393 [PubMed]
  • de Graaf BH, Knuiman BA, Derksen J, Mariani C. (2003) Characterization and localization of the transmitting tissue-specific PELPIII proteins of Nicotiana tabacum. J Exp Bot 54: 55–63 [PubMed]
  • Dong J, Kim ST, Lord EM. (2005) Plantacyanin plays a role in reproduction in Arabidopsis. Plant Physiol 138: 778–789 [PMC free article] [PubMed]
  • Elkins T, Zinn K, McAllister L, Hoffmann FM, Goodman CS. (1990) Genetic analysis of a Drosophila neural cell adhesion molecule: interaction of fasciclin I and Abelson tyrosine kinase mutations. Cell 60: 565–575 [PubMed]
  • Endo M, Tsuchiya T, Saito H, Matsubara H, Hakozaki H, Masuko H, Kamada M, Higashitani A, Takahashi H, Fukuda H. et al. (2004) Identification and molecular characterization of novel anther-specific genes in japonica rice, Oryza sativa L. by using cDNA microarray. Genes Genet Syst 70: 213–226 [PubMed]
  • Escobar-Restrepo JM, Huck N, Kessler S, Gagliardini V, Gheyselinck J, Yang WC, Grossniklaus U. (2007) The FERONIA receptor-like kinase mediates male-female interactions during pollen tube reception. Science 317: 656–660 [PubMed]
  • Feijó JA. (2010) The mathematics of sexual attraction. J Biol 9: 18–22 [PMC free article] [PubMed]
  • Flanagan CA, Hu Y, Ma H. (1996) Specific expression of the AGL1 MADS-box gene suggests regulatory functions in Arabidopsis gynoecium and ovule development. Plant J 10: 343–353 [PubMed]
  • Friedman WE. (1999) Expression of the cell cycle in sperm of Arabidopsis: implications for understanding patterns of gametogenesis and fertilization in plants and other eukaryotes. Development 126: 1065–1075 [PubMed]
  • Golovkin M, Reddy AS. (2003) A calmodulin-binding protein from Arabidopsis has an essential role in pollen germination. Proc Natl Acad Sci USA 100: 10558–10563 [PMC free article] [PubMed]
  • Grenningloh G, Rehm EJ, Goodman CS. (1991) Genetic analysis of growth cone guidance in Drosophila: fasciclin II functions as a neuronal recognition molecule. Cell 67: 45–57 [PubMed]
  • Hartig K, Beck E. (2006) Crosstalk between auxin, cytokinins, and sugars in the plant cell cycle. Plant Biol (Stuttg) 8: 389–396 [PubMed]
  • Hennig L, Gruissem W, Grossniklaus U, Köhler C. (2004) Transcriptional programs of early reproductive stages in Arabidopsis. Plant Physiol 135: 1765–1775 [PMC free article] [PubMed]
  • Herrero J, Al-Shahrour F, Díaz-Uriarte R, Mateos A, Vaquerizas JM, Santoyo J, Dopazo J. (2003) GEPAS: a web-based resource for microarray gene expression data analysis. Nucleic Acids Res 31: 3461–3467 [PMC free article] [PubMed]
  • Herrero J, Valencia A, Dopazo J. (2001) A hierarchical unsupervised growing neural network for clustering gene expression patterns. Bioinformatics 17: 126–136 [PubMed]
  • Higashiyama T, Inatsugi R, Sakamoto S, Sasaki N, Mori T, Kuroiwa H, Nakada T, Nozaki H, Kuroiwa T, Nakano A. (2006) Species preferentiality of the pollen tube attractant derived from the synergid cell of Torenia fournieri. Plant Physiol 142: 481–491 [PMC free article] [PubMed]
  • Higashiyama T, Kuroiwa H, Kuroiwa T. (2003) Pollen-tube guidance: beacons from the female gametophyte. Curr Opin Plant Biol 6: 36–41 [PubMed]
  • Higashiyama T, Yabe S, Sasaki N, Nishimura Y, Miyagishima S, Kuroiwa H, Kuroiwa T. (2001) Pollen tube attraction by the synergid cell. Science 293: 1480–1483 [PubMed]
  • Hiscock SJ, Allen AM. (2008) Diverse cell signalling pathways regulate pollen-stigma interactions: the search for consensus. New Phytol 179: 286–317 [PubMed]
  • Honys D, Twell D. (2003) Comparative analysis of the Arabidopsis pollen transcriptome. Plant Physiol 132: 640–652 [PMC free article] [PubMed]
  • Honys D, Twell D. (2004) Transcriptome analysis of haploid male gametophyte development in Arabidopsis. Genome Biol 5: R85. [PMC free article] [PubMed]
  • Huck N, Moore JM, Federer M, Grossniklaus U. (2003) The Arabidopsis mutant feronia disrupts the female gametophytic control of pollen tube reception. Development 130: 2149–2159 [PubMed]
  • Jiang L, Yang SL, Xie LF, Puah CS, Zhang XQ, Yang WC, Sundaresan V, Ye D. (2005) VANGUARD1 encodes a pectin methylesterase that enhances pollen tube growth in the Arabidopsis style and transmitting tract. Plant Cell 17: 584–596 [PMC free article] [PubMed]
  • Johnston AJ, Meier P, Gheyselinck J, Wuest SE, Federer M, Schlagenhauf E, Becker JD, Grossniklaus U. (2007) Genetic subtraction profiling identifies genes essential for Arabidopsis reproduction and reveals interaction between the female gametophyte and the maternal sporophyte. Genome Biol 8: R204. [PMC free article] [PubMed]
  • Jones-Rhoades MW, Borevitz JO, Preuss D. (2007) Genome-wide expression profiling of the Arabidopsis female gametophyte identifies families of small, secreted proteins. PLoS Genet 3: 1848–1861 [PMC free article] [PubMed]
  • Kaothien P, Ok SH, Shuai B, Wengier D, Cotter R, Kelley D, Kiriakopolos S, Muschietti J, McCormick S. (2005) Kinase partner protein interacts with the LePRK1 and LePRK2 receptor kinases and plays a role in polarized pollen tube growth. Plant J 42: 492–503 [PubMed]
  • Kinoshita T, Miura A, Choi Y, Kinoshita Y, Cao X, Jacobsen SE, Fischer RL, Kakutani T. (2004) One-way control of FWA imprinting in Arabidopsis endosperm by DNA methylation. Science 303: 521–523 [PubMed]
  • Lan L, Chen W, Lai Y, Suo J, Kong Z, Li C, Lu Y, Zhang Y, Zhao X, Zhang X, et al. (2004) Monitoring of gene expression profiles and isolation of candidate genes involved in pollination and fertilization in rice (Oryza sativa L.) with a 10K cDNA microarray. Plant Mol Biol 54: 471–487 [PubMed]
  • Lau S, Jürgens G, De Smet I. (2008) The evolving complexity of the auxin pathway. Plant Cell 20: 1738–1746 [PMC free article] [PubMed]
  • Le BH, Cheng C, Bui AQ, Wagmaister JA, Henry KF, Pelletier J, Kwong L, Belmonte M, Kirkbride R, Horvath S, et al. (2010) Global analysis of gene activity during Arabidopsis seed development and identification of seed-specific transcription factors. Proc Natl Acad Sci USA 107: 8063–8070 [PMC free article] [PubMed]
  • Leek JT, Monsen E, Dabney AR, Storey JD. (2006) EDGE: extraction and analysis of differential gene expression. Bioinformatics 22: 507–508 [PubMed]
  • Li C, Hung Wong W. (2001) Model-based analysis of oligonucleotide arrays: model validation, design issues and standard error application. Genome Biol 2: RESEARCH0032. [PMC free article] [PubMed]
  • Liu YG, Mitsukawa N, Oosumi T, Whittier RF. (1995) Efficient isolation and mapping of Arabidopsis thaliana T-DNA insert junctions by thermal asymmetric interlaced PCR. Plant J 8: 457–463 [PubMed]
  • Lorenzo O, Piqueras R, Sánchez-Serrano JJ, Solano R. (2003) ETHYLENE RESPONSE FACTOR1 integrates signals from ethylene and jasmonate pathways in plant defense. Plant Cell 15: 165–178 [PMC free article] [PubMed]
  • Luo M, Bilodeau P, Koltunow A, Dennis ES, Peacock WJ, Chaudhury AM. (1999) Genes controlling fertilization-independent seed development in Arabidopsis thaliana. Proc Natl Acad Sci USA 96: 296–301 [PMC free article] [PubMed]
  • Martin FW. (1959) Staining and observing pollen tubes in the style by means of fluorescence. Stain Technol 34: 125–128 [PubMed]
  • Menges M, Samland AK, Planchais S, Murray JA. (2006) The D-type cyclin CYCD3;1 is limiting for the G1-to-S-phase transition in Arabidopsis. Plant Cell 18: 893–906 [PMC free article] [PubMed]
  • Morris ER, Walker JC. (2003) Receptor-like protein kinases: the keys to response. Curr Opin Plant Biol 6: 339–342 [PubMed]
  • Muschietti J, Eyal Y, McCormick S. (1998) Pollen tube localization implies a role in pollen-pistil interactions for the tomato receptor-like protein kinases LePRK1 and LePRK2. Plant Cell 10: 319–330 [PMC free article] [PubMed]
  • Nemhauser JL, Mockler TC, Chory J. (2004) Interdependency of brassinosteroid and auxin signaling in Arabidopsis. PLoS Biol 2: E258. [PMC free article] [PubMed]
  • Ohyama K, Ogawa M, Matsubayashi Y. (2008) Identification of a biologically active, small, secreted peptide in Arabidopsis by in silico gene screening, followed by LC-MS-based structure analysis. Plant J 55: 152–160 [PubMed]
  • Okuda S, Tsutsui H, Shiina K, Sprunck S, Takeuchi H, Yui R, Kasahara RD, Hamamura Y, Mizukami A, Susaki D, et al. (2009) Defensin-like polypeptide LUREs are pollen tube attractants secreted from synergid cells. Nature 458: 357–361 [PubMed]
  • Olmedo G, Guo H, Gregory BD, Nourizadeh SD, Aguilar-Henonin L, Li H, An F, Guzmán P, Ecker JR. (2006) ETHYLENE-INSENSITIVE5 encodes a 5′→3′ exoribonuclease required for regulation of the EIN3-targeting F-box proteins EBF1/2. Proc Natl Acad Sci USA 103: 13286–13293 [PMC free article] [PubMed]
  • O’Neill SD. (1997) Pollination regulation of flower development. Annu Rev Plant Physiol Plant Mol Biol 48: 547–574 [PubMed]
  • Palanivelu R, Brass L, Edlund AF, Preuss D. (2003) Pollen tube growth and guidance is regulated by POP2, an Arabidopsis gene that controls GABA levels. Cell 114: 47–59 [PubMed]
  • Park SY, Lord EM. (2003) Expression studies of SCA in lily and confirmation of its role in pollen tube adhesion. Plant Mol Biol 51: 183–189 [PubMed]
  • Pina C, Pinto F, Feijó JA, Becker JD. (2005) Gene family analysis of the Arabidopsis pollen transcriptome reveals biological implications for cell growth, division control, and gene expression regulation. Plant Physiol 138: 744–756 [PMC free article] [PubMed]
  • Punwani JA, Rabiger DS, Drews GN. (2007) MYB98 positively regulates a battery of synergid-expressed genes encoding filiform apparatus localized proteins. Plant Cell 19: 2557–2568 [PMC free article] [PubMed]
  • Qin Y, Leydon AR, Manziello A, Pandey R, Mount D, Denic S, Vasic B, Johnson MA, Palanivelu R. (2009) Penetration of the stigma and style elicits a novel transcriptome in pollen tubes, pointing to genes critical for growth in a pistil. PLoS Genet 5: 1–19 [PMC free article] [PubMed]
  • Riou-Khamlichi C, Huntley R, Jacqmard A, Murray JA. (1999) Cytokinin activation of Arabidopsis cell division through a D-type cyclin. Science 283: 1541–1544 [PubMed]
  • Rotman N, Rozier F, Boavida L, Dumas C, Berger F, Faure JE. (2003) Female control of male gamete delivery during fertilization in Arabidopsis thaliana. Curr Biol 13: 432–436 [PubMed]
  • Rounsley SD, Ditta GS, Yanofsky MF. (1995) Diverse roles for MADS box genes in Arabidopsis development. Plant Cell 7: 1259–1269 [PMC free article] [PubMed]
  • Samuel MA, Chong YT, Haasen KE, Aldea-Brydges MG, Stone SL, Goring DR. (2009) Cellular pathways regulating responses to compatible and self-incompatible pollen in Brassica and Arabidopsis stigmas intersect at Exo70A1, a putative component of the exocyst complex. Plant Cell 21: 2655–2671 [PMC free article] [PubMed]
  • Schmid M, Davison TS, Henz SR, Pape UJ, Demar M, Vingron M, Schölkopf B, Weigel D, Lohmann JU. (2005) A gene expression map of Arabidopsis thaliana development. Nat Genet 37: 501–506 [PubMed]
  • Scutt CP, Vinauger-Douard M, Fourquin C, Ailhas J, Kuno N, Uchida K, Gaude T, Furuya M, Dumas C. (2003) The identification of candidate genes for a reverse genetic analysis of development and function in the Arabidopsis gynoecium. Plant Physiol 132: 653–665 [PMC free article] [PubMed]
  • Shimizu KK, Okada K. (2000) Attractive and repulsive interactions between female and male gametophytes in Arabidopsis pollen tube guidance. Development 127: 4511–4518 [PubMed]
  • Shultz RW, Tatineni VM, Hanley-Bowdoin L, Thompson WF. (2007) Genome-wide analysis of the core DNA replication machinery in the higher plants Arabidopsis and rice. Plant Physiol 144: 1697–1714 [PMC free article] [PubMed]
  • Singh KB. (1998) Transcriptional regulation in plants: the importance of combinatorial control. Plant Physiol 118: 1111–1120 [PMC free article] [PubMed]
  • Smyth DR, Bowman JL, Meyerowitz EM. (1990) Early flower development in Arabidopsis. Plant Cell 2: 755–767 [PMC free article] [PubMed]
  • Sorrell DA, Menges M, Healy JM, Deveaux Y, Amano C, Su Y, Nakagami H, Shinmyo A, Doonan JH, Sekine M, Murray JA.(2010) Cell cycle regulation of cyclin-dependent kinases in tobacco cultivar Bright Yellow-2 cells. Plant Physiol 126: 1214–1223 [PMC free article] [PubMed]
  • Steffen JG, Kang IH, Macfarlane J, Drews GN. (2007) Identification of genes expressed in the Arabidopsis female gametophyte. Plant J 51: 281–292 [PubMed]
  • Storey JD. (2002) A direct approach to false discovery rates. J R Stat Soc B Stat Method 64: 479–498
  • Sundaresan V, Springer P, Volpe T, Haward S, Jones JDG, Dean C, Ma H, Martienssen RA. (1995) Patterns of gene action in plant development revealed by enhancer trap and gene trap transposable elements. Genes Dev 9: 1797–1810 [PubMed]
  • Tang W, Kelley D, Ezcurra I, Cotter R, McCormick S. (2004) LeSTIG1, an extracellular binding partner for the pollen receptor kinases LePRK1 and LePRK2, promotes pollen tube growth in vitro. Plant J 39: 343–353 [PubMed]
  • Thimm O, Bläsing O, Gibon Y, Nagel A, Meyer S, Krüger P, Selbig J, Müller LA, Rhee SY, Stitt M. (2004) MAPMAN: a user-driven tool to display genomics data sets onto diagrams of metabolic pathways and other biological processes. Plant J 37: 914–939 [PubMed]
  • Tung CW, Dwyer KG, Nasrallah ME, Nasrallah JB. (2005) Genome-wide identification of genes expressed in Arabidopsis pistils specifically along the path of pollen tube growth. Plant Physiol 138: 977–989 [PMC free article] [PubMed]
  • Tusher VG, Tibshirani R, Chu G. (2001) Significance analysis of microarrays applied to the ionizing radiation response. Proc Natl Acad Sci USA 98: 5116–5121 [PMC free article] [PubMed]
  • Vielle-Calzada JP, Thomas J, Spillane C, Coluccio A, Hoeppner MA, Grossniklaus U. (1999) Maintenance of genomic imprinting at the Arabidopsis medea locus requires zygotic DDM1 activity. Genes Dev 13: 2971–2982 [PMC free article] [PubMed]
  • Wang Y, Zhang WZ, Song LF, Zou JJ, Su Z, Wu WH. (2008) Transcriptome analyses show changes in gene expression to accompany pollen germination and tube growth in Arabidopsis. Plant Physiol 148: 1201–1211 [PMC free article] [PubMed]
  • Wellmer F, Riechmann JL, Alves-Ferreira M, Meyerowitz EM. (2004) Genome-wide analysis of spatial gene expression in Arabidopsis flowers. Plant Cell 16: 1314–1326 [PMC free article] [PubMed]
  • Wengier DL, Mazzella MA, Salem TM, McCormick S, Muschietti JP. (2010) STIL, a peculiar molecule from styles, specifically dephosphorylates the pollen receptor kinase LePRK2 and stimulates pollen tube growth in vitro. BMC Plant Biol 10: 33. [PMC free article] [PubMed]
  • Wu HM, Wang H, Cheung AY. (1995) A pollen tube growth stimulatory glycoprotein is deglycosylated by pollen tubes and displays a glycosylation gradient in the flower. Cell 82: 395–403 [PubMed]
  • Wu HM, Wong E, Ogdahl J, Cheung AY. (2000) A pollen tube growth-promoting arabinogalactan protein from Nicotiana alata is similar to the tobacco TTS protein. Plant J 22: 165–176 [PubMed]
  • Wuest SE, Vijverberg K, Schmidt A, Weiss M, Gheyselinck J, Lohr M, Wellmer F, Rahnenführer J, von Mering C, Grossniklaus U. (2010) Arabidopsis female gametophyte gene expression map reveals similarities between plant and animal gametes. Curr Biol 20: 506–512 [PubMed]
  • Yoshida KT, Endo M, Nakazono M, Fukuda H, Demura T, Tsuchiya T, Watanabe M. (2005) cDNA microarray analysis of gene expression changes during pollination, pollen-tube elongation, fertilization and early embryogenesis in rice pistils. Sex Plant Reprod 17: 269–275
  • Yu HJ, Hogan P, Sundaresan V. (2005) Analysis of the female gametophyte transcriptome of Arabidopsis by comparative expression profiling. Plant Physiol 139: 1853–1869 [PMC free article] [PubMed]
  • Zhang Y, McCormick S. (2007) A distinct mechanism regulating a pollen-specific guanine nucleotide exchange factor for the small GTPase Rop in Arabidopsis thaliana. Proc Natl Acad Sci USA 104: 18830–18835 [PMC free article] [PubMed]
  • Zimmermann P, Hirsch-Hoffmann M, Hennig L, Gruissem W. (2004) GENEVESTIGATOR: Arabidopsis microarray database and analysis toolbox. Plant Physiol 136: 2621–2632 [PMC free article] [PubMed]

Articles from Plant Physiology are provided here courtesy of American Society of Plant Biologists
PubReader format: click here to try


Related citations in PubMed

See reviews...See all...

Cited by other articles in PMC

See all...


Recent Activity

Your browsing activity is empty.

Activity recording is turned off.

Turn recording back on

See more...