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Open Access

Peer-reviewed

Research Article

HAPLESS13-Mediated Trafficking of STRUBBELIG Is Critical for Ovule Development in Arabidopsis

  • Jia-Gang Wang,

    Affiliation State Key Laboratory of Crop Biology, College of Life Sciences, Shandong Agricultural University, Tai’an, China

    ⨯
  • Chong Feng,

    Affiliation State Key Laboratory of Crop Biology, College of Life Sciences, Shandong Agricultural University, Tai’an, China

    ⨯
  • Hai-Hong Liu,

    Affiliation State Key Laboratory of Crop Biology, College of Life Sciences, Shandong Agricultural University, Tai’an, China

    ⨯
  • Fu-Rong Ge,

    Affiliation State Key Laboratory of Crop Biology, College of Life Sciences, Shandong Agricultural University, Tai’an, China

    ⨯
  • Sha Li,

    Affiliation State Key Laboratory of Crop Biology, College of Life Sciences, Shandong Agricultural University, Tai’an, China

    ⨯
  • Hong-Ju Li,

    Affiliation State Key Laboratory of Molecular Developmental Biology, Institute of Genetics and Developmental Biology, Chinese Academy of Sciences, Beijing, China

    ⨯
  • Yan Zhang

    yzhang@sdau.edu.cn

    Affiliation State Key Laboratory of Crop Biology, College of Life Sciences, Shandong Agricultural University, Tai’an, China

    ⨯

Abstract

Planar morphogenesis, a distinct feature of multicellular organisms, is crucial for the development of ovule, progenitor of seeds. Both receptor-like kinases (RLKs) such as STRUBBELIG (SUB) and auxin gradient mediated by PIN-FORMED1 (PIN1) play instructive roles in this process. Fine-tuned intercellular communications between different cell layers during ovule development demands dynamic membrane distribution of these cell-surface proteins, presumably through vesicle-mediated sorting. However, the way it’s achieved and the trafficking routes involved are obscure. We report that HAPLESS13 (HAP13)-mediated trafficking of SUB is critical for ovule development. HAP13 encodes the μ subunit of adaptor protein 1 (AP1) that mediates protein sorting at the trans-Golgi network/early endosome (TGN/EE). The HAP13 mutant, hap13-1, is defective in outer integument growth, resulting in exposed nucellus accompanied with impaired pollen tube guidance and reception. SUB is mis-targeted in hap13-1. However, unlike that of PIN2, the distribution of PIN1 is independent of HAP13. Genetic interference of exocytic trafficking at the TGN/EE by specifically downregulating HAP13 phenocopied the defects of hap13-1 in SUB targeting and ovule development, supporting a key role of sporophytically expressed SUB in instructing female gametogenesis.

Author Summary

Ovules, being the progenitors of seeds, hold an important role in crop production. Ovule is a complex organ connecting two generations, i.e. diploid sporophytic cells and haploid female gametophytes (FG). Fertilization of female gametes leads to the development of embryo and endosperm while the sporophytic cells of ovules become seed coats. Because of its importance for plant reproduction, the development of ovules is tightly controlled. The integument cells are divided in a polar way so that integument cell layers fully enclose a mature FG, leaving an opening only for pollen tube entrance. The integuments also instruct FG development, synchronizing the two generations. Receptor-like kinases, especially STRUBBELIG (SUB), are crucial both for the establishment of ovular polarity and the intercellular communication between sporophytic and gametophytic cells. However, how SUB is post-translationally regulated, as would be expected for cell-surface proteins, is unclear. We report here that the dynamic trafficking of SUB via a subpopulation of endosomes is crucial for its functionality during ovule development. The membrane association of SUB was impaired when the recycling route from the trans-Golgi network/early endosome to the plasma membrane was disrupted in hap13-1, a mutant of HAPLESS13. We further demonstrate that defects of SUB targeting in the outer integuments compromised FG development, suggesting an intriguing intercellular communication. Our results highlight the importance of vesicular trafficking in the establishment of ovular polarity and in the communications between spatially separated cells.

Citation: Wang J-G, Feng C, Liu H-H, Ge F-R, Li S, Li H-J, et al. (2016) HAPLESS13-Mediated Trafficking of STRUBBELIG Is Critical for Ovule Development in Arabidopsis. PLoS Genet 12(8): e1006269. https://doi.org/10.1371/journal.pgen.1006269

Editor: Venkatesan Sundaresan, UC Davis, UNITED STATES

Received: March 25, 2016; Accepted: July 30, 2016; Published: August 19, 2016

Copyright: © 2016 Wang et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.

Data Availability: All relevant data are within the paper and its Supporting Information files.

Funding: This work was supported by Major Research Plan (2013CB945102) from the Ministry of Science, Technology of China, by Shandong Provincial Natural Science Foundation (ZR2014CM027 to SL), and by Shandong Provincial Funds for Outstanding Young Scientists (to YZ). YZ’s laboratory is partially supported by Tai-Shan Scholar Program by Shandong Provincial Government. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

Competing interests: The authors have declared that no competing interests exist.

Introduction

Tissue or planar polarity that distinguishes multicellular organisms from unicellular ones requires coordinated cell behavior within a tissue or the plane of a tissue layer through intercellular communications and intracellular asymmetry [1,2]. Ovule development in angiosperms manifests the complexity by establishing and maintaining polarity in the proximal-distal axis, along which three morphologically distinct units are observed: the nucellus at the distal end harbors the megaspore mother cell (MMC) that undergoes meiosis to form an embryo sac, i.e. the female gametophyte (FG); from the chalaza at the central region, outer and inner integuments initiate growth, eventually enveloping the nucellus; the proximal funiculus connects the ovule to the placenta [1,3–6]. Fine-tuned intercellular communications are critical for primordium initiation, pattern formation, planar morphogenesis and female gametogenesis, collectively leading to ovule development [1,3,7].

Intercellular communication in plant development is mainly controlled by the phytohormone auxin as well as receptor-like kinases (RLKs) [2,8,9]. Auxin has been attributed as an instructive factor in the establishment and maintenance of tissue or planar polarity, through its asymmetric gradient [2,8,10,11]. Auxin gradient or maximum is a result of local biosynthesis, metabolism, and most importantly, transport facilitated by auxin influx and efflux carriers [8,10,11]. PIN-FORMED (PIN), the auxin efflux carriers, is encoded by 8 genes in Arabidopsis (PIN1-PIN8), whose dynamic distribution, often asymmetric, is essential for auxin gradient [8,10,11]. Among the eight PINs, PIN1 was reported to be critical for ovule development [8,12,13]. Tissue or planar polarity is also regulated by cellular perception and responses of neighboring cells through RLKs, whose extracellular domains enable signal perception while cytoplasmic domains allow intracellular signal relay [9]. Mutations at a few RLK-coding genes, such as STRUBBELIG (SUB), ARABIDOPSIS CRINKLY4 (ACR4), and ERECTA-family genes (ER and ERLs), resulted in defective ovular development [14–16].

The membrane distribution of PINs and RLKs is dynamically regulated by vesicle trafficking-mediated protein sorting [11,17–19]. In the past decade, extensive studies revealed the key role of vesicle trafficking on the dynamic asymmetry of PINs [11,17,19]. RLKs are another dominant class of transmembrane (TM) proteins whose dynamic distribution through vesicles has been under close scrutiny [18]. The internalization of RLKs could be constitutive or induced whereas the internalized RLKs may recycle back to the PM non-selectively or selectively, as well as go to vacuoles for degradation [18]. As a consequence of their differential distributions, intracellular signaling is enhanced, reduced, or switched [18]. Therefore, vesicle trafficking-mediated protein sorting is fundamental to development. However, little is known on vesicle trafficking during ovule development, the trafficking routes involved, the key proteins vesicle-sorted, as well as the regulators of protein sorting.

An exocytic or anterograde trafficking route and an endocytic or retrograde trafficking route operate in plant cells to mediate protein sorting within the endomembrane system [20–22]. The two routes converge on the trans-Golgi network/early endosome (TGN/EE) [23], a likely heterogeneous group of endosomes equal to the combination of metazoan sorting endosomes, early endosomes, and recycling endosomes [21,22]. Protein sorting within the endomembrane system requires adaptor protein (AP) complexes, i.e. tetrameric protein complexes for cargo selection and coat recruitment [20,22,24]. Among the five AP complexes in eukaryotes, AP1 is associated with the TGN/EE and thus plays essential roles in protein sorting in plant cells [25–27]. AP1 consists of two large subunits (γ, β), one medium subunit (μ), and a small subunit (σ) [20,22,24]. We and others previously reported the identification of Arabidopsis AP1μ, HAPLESS13 (HAP13)/AP1MU2 [25–27]. Mutations of HAP13 severely reduced male gametophytic transmission [25,27,28] whereas its homozygous mutants showed growth retardation [27]. Key TM proteins such as PIN2 [25,27], BRI1 [27], and KNOLLE [26] were mis-localized in the mutant of HAP13, hap13-1, demonstrating the key role of HAP13 in TGN/EE-centered protein sorting.

We report here that HAP13-mediated protein sorting at the TGN/EE is critical for ovule development, specifically the asymmetric growth of outer integuments. By scanning electron microscopy (SEM), plastic section, and confocal laser scanning microscopy (CLSM), we show that hap13-1 is defective in outer integument growth, leading to exposed or protruding nucellus. The defect in outer integuments severely affected female gametogenesis such that a large portion of hap13-1 ovules did not contain a well-patterned embryo sac. Consequently, pollen tube guidance and reception were impaired, resulting in reduced female fertility. We further show that the key RLK for ovule development, SUB, was mis-targeted in hap13-1, correlating with the phenotypic similarity in ovules between hap13-1 and SUB mutants. However, unlike PIN2 whose membrane distribution relies on HAP13 [25,27], the asymmetric targeting of PIN1 at the nucellus was intact in hap13-1, suggesting distinct sorting mechanisms for different PINs. Downregulating HAP13 expression by RNA interference (RNAi) specifically in outer integuments phenocopied the ovular defects in hap13-1. Results presented here demonstrate the importance of TGN/EE-centered protein sorting in outer integument growth and provide clues for a deep understanding of molecular mechanisms underlying the establishment and maintenance of ovule polarity.

Results

Expression of HAP13 during ovule development

HAP13 was expressed in various tissues and developmental stages [27]. To determine whether HAP13 was expressed during ovule development, we generated a nuclear-localized YFP reporter line for HAP13 (ProHAP13:NLS-YFP). Confocal laser scanning microscopy (CLSM) revealed that HAP13 was expressed in all cell layers during ovule development (Fig 1A and 1B). Finally, the expression of HAP13 in ovules during development was confirmed by examining the HAP13g-GFP hap13-1 transgenic plants (Fig 1C–1F). The expression of HAP13 in ovules from primordium formation till maturation hinted at the possibility of its function in ovule development.

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Fig 1. Expression of HAP13 during ovule development.

(A-B) Confocal laser scanning micrographs (CLSM) of ProHAP13:NLS-YFP ovules at stage 2-I (A) or at stage 2-III (B). Silhouettes of developing ovular primordia (A) or ovule (B) were indicated with dotted lines. Nu nucellus; ii, inner integument; oi, outer integument. (C-F) CLSM of developing ovules from HAP13g-GFP hap13-1 transgenic plants at stage 2-III (C), 3-I (D), 3-III (E), and 3-V (F). Merge images of the GFP channel and the RFP channel (Lysotracker red, to show cell silhouettes) are at the bottom of corresponding GFP channel images. Bars = 50 μm for (A); 10 μm for (B-F).

https://doi.org/10.1371/journal.pgen.1006269.g001

Ovule developmental defects in hap13-1

To determine whether HAP13 was required for ovule development, we examined hap13-1 pistils by SEM and CLSM analyses. Ovules are connected with the gynoecium through the funiculus (Fig 2A and 2B). At the distal end of the funiculus is a cleft, i.e. micropyle, formed by inner and outer integument cells enveloping the seven-celled embryo sac in wild type (Fig 2A–2D). In comparison, around 80% of hap13-1 ovules (Fig 2H) were abnormal such that the surface cell layers were broken and thus only partially wrapping the inner structure (Fig 2B and 2D). At maturity, wild-type ovules contained well-patterned FGs with a central cell, an egg cell and two synergid cells (Fig 2E). By contrast, FGs were abnormal in over 80% of hap13-1 ovules (Fig 2F and 2G). In addition, due to incomplete growth of outer integuments, embryo sacs in hap13-1 ovules were exposed or protruding (Fig 2B and 2D).

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Fig 2. Ovule development in wild type and hap13-1.

(A-B) Scanning electron micrographs (SEMs) of wild-type (A) or hap13-1 (B) mature pistils at 48 hours after pollination (HAP). The defective hap13-1 ovules are highlighted with arrowheads. (C-D) Close-ups of wild-type (C) or hap13-1 (D) ovules as indicated in the shaded rectangle box in (A-B). An incoming pollen tube (Pt) at the micropyle of a wild-type ovule is false-colored pink. Two ovules with broken or incomplete outer integuments are shown in (D). (E-G) CLSM of a mature ovule from wild type (E), or from a mildly affected (F) or severely affected (G) hap13-1 mutant. Mid-optical sections of stage 3-V ovules are shown. The number of displayed type among all ovules examined is shown at the bottom left. (H) Quantitative analyses of integument development. Results in (H) are means ± standard errors (SE, N = 15). Bars = 100 μm for (A-B); 50 μm for (C); 20 μm for (D); 25 μm for (E-G).

https://doi.org/10.1371/journal.pgen.1006269.g002

Sporophytically controlled female gametophytic function was compromised in hap13-1

Pollination of emasculated hap13-1 pistils with wild-type pollen only yields a few seeds although female transmission of hap13-1 was normal [27]. To determine the cause of the reduced female fertility, we performed aniline blue staining of emasculated wild-type or hap13-1 pistils hand-pollinated with wild-type pollen at different time points. At 4 hours after pollination (HAP), pollen tubes already entered the transmitting track in wild-type pistils but only exited the style in hap13-1 pistils (Fig 3A). It suggested that hap13-1 pistils were compromised in the support of pollen tube growth. At 9 HAP, pollen tubes reached the bottom of both wild-type and hap13-1 pistils (Fig 3A). However, hap13-1 pistils were much shorter than those of wild type due to a reduced number of ovules (Fig 3A). Therefore, pollen tube growth inside hap13-1 pistils was substantially slow. At 48 HAP when wild-type pistils contained enlarged ovules indicative of successful fertilization (Fig 3A and 3B), only few ovules were enlarged in hap13-1 pistils (Fig 3A and 3D). Most hap13-1 ovules were not targeted by pollen tubes (163 out of 213, Fig 3C), indicating compromised pollen tube guidance. Another portion of hap13-1 ovules did attract pollen tubes (26 out of 213, Fig 3E). However, these ovules failed to instruct the cessation of pollen tube growth, resulting in overgrown pollen tubes inside embryo sacs and failed fertilization (Fig 3E).

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Fig 3. Pollen tube guidance and reception are compromised in the homozygous hap13-1.

(A) Aniline blue staining of wild-type or hap13-1 pistils emasculated and hand-pollinated with wild-type pollen at 4, 9, or 48 hours after pollination (HAP). Arrows indicate the growth front of pollen tubes. (B-E) Close-ups of a wild-type ovule (B) and hap13-1 ovules of different categories, including hap13-1 ovules unable to attract pollen tubes (C), those pollinated and fertilized (D), or those with overgrown pollen tubes (E) at 48 HAP. Frequency of displayed ovules in total ovules examined is shown on top. Arrowheads point at the micropylar region. (F-G) Immunofluorescence staining of a mature wild-type (F) or hap13-1 ovule (G) using an anti-LURE antibody. Bars = 100 μm for 4 HAP images in (A), 200 μm for 9 HAP or 48 HAP in (A), 50 μm for (B-E), 20 μm for (F-G).

https://doi.org/10.1371/journal.pgen.1006269.g003

To determine the reason of reduced pollen tube guidance in hap13-1, we performed immunofluorescence staining on wild-type and hap13-1 ovules using an anti-LURE antibody [29]. Because LURE is a key peptide secreted by synergid cells to attract pollen tubes [30,31], we wanted to test whether hap13-1 ovules were compromised in the production of LURE. In mature wild-type ovules, strong signals were detected in the micropylar region (Fig 3F), indicative of LURE secretion. By contrast, hap13-1 ovules (45 out of 57 examined) showed a substantial reduction of fluorescence signals (Fig 3G). This result explained the reduced pollen tube guidance of hap13-1 ovules. Next, we introduced an egg cell-specific reporter ProDD45:GUS [32] into hap13-1. By histochemical analysis of the homozygous transgene ProDD45:GUS in the heterozygous and homozygous hap13-1, we found that egg cells were present in almost all ovules of the heterozygous hap13-1 pistils, comparable to those of wild type (S1 Fig). However, only a few ovules of the homozygous hap13-1 pistils showed GUS signals (S1 Fig). These results demonstrated that defective patterning of hap13-1 FGs was caused by defects in surrounding sporophytic tissues.

Planar polarity during ovule development was compromised in hap13-1

To determine at which stage hap13-1 was defective during ovule development, we performed semi-thin plastic sections and CLSM on ovules at different developmental stages. The phenotype of hap13-1 in ovule development was variable, ranging from severely affected to normal and fertile ovules. Seventy percent of ovules from hap13-1 mutants displayed developmental irregularities (N = 256 of hap13-1 ovules for percentage calculation). Developmental defects of hap13-1 started at stage 2-III (Fig 4B), immediately after outer integuments were initiated [5,6]. Upon initiation at an abaxial position, outer integuments in hap13-1 sometimes failed to spread around the circumference of ovules, resulting in incomplete outer integuments (Fig 4B and 4F), unlike those in wild type where outer integuments fully covered inner integuments (Fig 4A and 4E). Cell expansion in outer integuments of hap13-1 was impaired (Fig 4C and 4D). This irregular cell growth and possibly division in hap13-1 resulted in ovules with exposed inner integuments, enveloped by fragmented outer integuments (Fig 4B and 4F). The two-cell-layered organization of outer integuments was also disrupted (Fig 4B and 4F), likely caused by mis-oriented division planes (Fig 4B and 4F). About 80% ovules in hap13-1 contained abnormal FGs, which always correlated with abnormal growth of outer integuments (Fig 4F).

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Fig 4. Planar polarity during ovule integument growth is compromised in hap13-1.

(A-B) Semi-thin sections of wild-type (A) or hap13-1 ovules (B) at developmental stage 2-I, 2-III, 3-I, or 3-V. ac, archesporial cell; dm, degenerating megaspore; fm, functional megaspore. Yellow-shaded areas are cells of inner integuments. Blue-shaded areas are cells of outer integuments. Pink-shaded areas indicate the embryo sacs. (C-D) Cell number and size of wild-type (C) or hap13-1 (D) outer integuments. Each column represents one stage 3-V ovule; the number of cubes in each column indicates the number of countable outer integument cells in a stage 3-V ovule; green cubes indicate small cells (area between 0.2 and 0.4, a.u.) while yellow cubes indicate large cells (are between 0.4 and 1, a.u.). (E-F) CLSMs of wild-type (E) or hap13-1 ovules (F) at stage 3-II, 3-III, or 3-IV. Ovules were stained with PI and mid-optical sections were shown. Because some hap13-1 ovules were completely avoid of embryo sac patterning and thus impossible to determine developmental stages, only hap13-1 ovules with visible nuclei are shown in (F). cn, chalazal nucleus; fu, funiculus; ii, inner integument; oi, outer integument; mn, micropylar nucleus. Bars = 10 μm.

https://doi.org/10.1371/journal.pgen.1006269.g004

SUB is mis-targeted during ovule development in hap13-1

The phenotypic defects of hap13-1 ovules resembled that of sub mutants to a great extent [14] and an earlier study showed that SUB could be internalized upon treating root cells with Brefeldin A (BFA) [33], a fungal toxin that inhibits post-Golgi secretion [34]. We thus hypothesized that membrane distribution of SUB relied on HAP13-mediated protein sorting at the TGN/EE. To test this hypothesis, we analyzed the distribution of SUB in hap13-1 by introducing a YFP-translational fusion of SUB genomic fragment driven by its endogenous promoter, SUBg-YFP [35]. A post-transcriptional regulation was proposed earlier based on the differential distribution patterns of a full SUB genomic fusion and a fusion with the coding sequence of SUB [33,36,37]. Nevertheless, both were able to fully restore ovular defects of sub mutants [33,36,37].

In ovules of the SUBg-YFP transgenic lines, YFP was barely detectable in the nucellus but present at both inner and outer integuments during early stages of ovule development as well as in all cell types in mature ovules (Fig 5A–5E), as reported [33,36,37]. Immediately after ovular primordia formation, YFP was distributed evenly at the plasma membrane (PM) of epidermal cell layer and also in a few vesicles (Fig 5A). With the development of ovules, YFP signals became asymmetric, i.e. excluded from the outward PM of the epidermal cell layer (Fig 5B and 5C). Punctate vesicles were still detectable (Fig 5B–5D). At later stages when outer integuments began rapid asymmetric elongation and finally wrapped embryo sacs, punctate vesicles labeled by YFP could hardly be detected (Fig 5E). Also YFP was more evenly distributed at the PM of the epidermal cell layer (Fig 5D and 5E). By contrast, YFP signals were mostly diffused in the cytoplasm rather than at the PM of hap13-1 ovules (Fig 5F–5J). Punctate vesicles, much larger than those in wild type, were visible despite the cytosolic signals (Fig 5F–5I). The asymmetry of YFP signals observed in wild type was often compromised such that it labeled the outward PM of the epidermal cell layer (Fig 5I). These results indicated that SUB is dynamically trafficked during ovule development and this process relies on HAP13. Interestingly, YFP signals were substantially reduced in hap13-1 despite that the same transgene was analyzed (Figs 5H and S2). Transcript analysis confirmed that the mRNA abundance of SUB was comparable between wild type and hap13-1 (S2 Fig), suggesting a post-transcriptional regulation of SUB. Indeed, a post-translational regulation was proposed earlier because treatment of the 26S proteasome inhibitor MG132 reduced the protein level of SUB [33].

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Fig 5. Dynamic localization of SUB is disrupted in hap13-1 ovules.

(A-E) Representative CLSM of ovules at different developmental stages from the SUBg-YFP transgenic plants. Dotted lines illustrate the shape of either megaspore mother cell (mmc), nucellus (nu), or of developing ovules (B-C). Arrows point at inner integuments (ii), outer integuments (oi), or punctate vesicles (without labeling). Note that SUBg-YFP was asymmetrically distributed in epidermal cell layers, i.e. excluded from the outward plasma membrane in (B-C). (F-J) Representative CLSM of ovules at different developmental stages from the SUBg-YFP;hap13-1 transgenic plants. Dotted lines illustrate the shape of either megaspore mother cell (mmc) or of developing ovules (G-H), and (J). Arrows point at inner integuments (ii), outer integuments (oi), or punctate vesicles (without labeling). Note that SUBg-YFP was more randomly distributed intracellularly and in larger vesicles. Four independent experiments involving 40 ovules at various developmental stages showed similar results. (H) Fluorescence intensity plots along the red lines across a typical outer integument cell in (B), (E), (G), and (J) are shown. The y-axis values represent signal intensity. The arrows indicate the signal accumulation at the plasma membrane. Bars = 10 μm.

https://doi.org/10.1371/journal.pgen.1006269.g005

To further verify that the subcellular targeting of SUB depends on HAP13, we analyzed SUB dynamic targeting in roots by using the fluorescence lipophilic dye FM4-64 together with pharmacological treatments. FM4-64 enters cells via endocytosis, labeling various endomembrane compartments over time and finally reaching vacuolar membrane, i.e. the tonoplast [38]. As shown in ovules, SUB was localized at the PM of wild-type root cells, overlapping with FM4-64 immediately after pulse labeling (S3 Fig). Treatment of roots with BFA at the presence of cycloheximide (CHX) resulted in the accumulation of SUB signals into BFA compartments co-labeled by FM4-64 (S3 Fig). Because BFA compartments formed at the presence of CHX contain only proteins internalized from the PM [27], the result indicated that SUB was constitutively internalized from the PM. The internalization of SUB upon BFA treatment was comparable between wild type and hap13-1 (S3 Fig), which is consistent with the intact endocytosis in hap13-1 [27]. Washout of BFA with CHX caused complete re-distribution of SUB from the BFA compartments to the PM in wild type, when FM4-64 labeled the tonoplast via vacuolar trafficking (S3 Fig). By contrast, the internalized SUB was insensitive to BFA washout in hap13-1 (S3 Fig). Instead, it remained sequestered at the BFA compartments together with FM4-64 (S3 Fig). These results suggested that the recycling of SUB from the TGN/EE to the PM requires HAP13.

PIN1 localization and auxin responses during ovule development in hap13-1

Except for SUB, PIN1 is another key component for ovule development by channeling auxin flux to the primordia tip [8,13]. We and others previously showed that the dynamic targeting of PIN2 relies on HAP13 whose mutations resulted in defective gravitropism due to mis-targeting of PIN2 [25,27]. In addition, both PIN1 and PIN2 belong to the same subgroup of PINs with a long hydrophilic loop [39]. We thus hypothesized that PIN1 dynamic targeting also relied on HAP13. To test this hypothesis, we introduced the PIN1 genomic-GFP translation fusion, PIN1::GFP [8], into hap13-1 and followed its membrane distribution at different developmental stages in ovules. PIN1 was detected at the outer cell layer of the nucellus, pointing toward the distal tip (Fig 6A and 6B). Surprisingly, the asymmetric membrane localization of PIN1 was comparable between wild type and hap13-1 despite the abnormal integument growth of hap13-1 (Fig 6C and 6D). Consistent with the intact PIN1 distribution in the nucellus, auxin responses at the nucellus (Fig 6E and 6F) as indicated by the activity of DR5:GFP [40] also did not show abnormality in hap13-1 (Fig 6G and 6H).

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Fig 6. Auxin maximum and polar localization of PIN1 in hap13-1 ovules.

(A-D) PIN1::GFP in wild-type (A, B) or in hap13-1 (C, D) ovules at stage 2-II (A, C) or at stage 3-I (B, D) by CLSM. (E-H) DR5:GFP in wild-type (E, F) or in hap13-1 (G, H) ovules at stage 2-III (E, G) or at stage 3-II (F, H) by CLSM. Merges of bright-field and fluorescent images are placed at the right of corresponding fluorescent images. Bars = 10 μm.

https://doi.org/10.1371/journal.pgen.1006269.g006

To determine whether the HAP13-independent PIN1 targeting also applied to other cells, we examined the localization of PIN1 in the roots of hap13-1. No substantial difference of PIN1 distribution was found between wild type and hap13-1 in root cells (S4 Fig), confirming the HAP13-independency of PIN1 targeting.

Genetic interference of HAP13 in outer integuments mimics hap13-1 in ovule development

We previously showed that a full length HAP13 genomic fragment fully restored developmental and cellular defects in hap13-1 [27], confirming the mutant identity of hap13-1. Indeed, HAP13g-GFP completely restored ovule development of hap13-1 (Fig 1C–1F). However, HAP13 is constitutively expressed and its mutations results in a full spectrum of developmental defects [27]. Thus, the defects in outer integument growth of hap13-1 might be non-cell-autonomous. To exclude the possibility, we used an RNAi approach. We generated ProUBQ10:HAP13-RNAi and analyzed the transcript level of HAP13 in seedlings as well as examined the effect of HAP13-RNAi on vesicle trafficking. Six out of twenty ProUBQ10:HAP13-RNAi transgenic lines were randomly selected. Real-time quantitative PCRs (qPCRs) verified a significant reduction of HAP13 transcripts by ProUBQ10:HAP13-RNAi (S5 Fig). In addition, hap13-1 was insensitive to BFA washout [27], which was confirmed in root epidermal cells of ProUBQ10:HAP13-RNAi transgenic lines by an uptake experiment using the lipophilic dye FM4-64 (S5 Fig). These results verified the efficient down-regulation of HAP13 by RNAi.

To downregulate the expression of HAP13 specifically in outer integuments, we generated a construct containing HAP13-RNAi driven by the promoter of INNER NO OUTER (ProINO). ProINO was reported previously for its specific expression in ovules based on RNA in situ hybridization [41]. To test whether ProINO was specific for outer integuments where severe growth defects were observed in hap13-1, we performed histochemical GUS staining on ProINO:GUS transgenic ovules at different stages. GUS signals were first observed at the stage 2-I in cells to be differentiated into outer integuments (S6 Fig). The asymmetrically distributed GUS signals, correlating with the asymmetric growth of outer integuments, were getting stronger during development. GUS signals were nearly undetectable when embryo sacs were fully formed (S6 Fig). Although ProINO showed a slightly wider spatial activity than the transcripts of INO based on in situ hybridization [42], the histochemical GUS analysis nevertheless demonstrated that ProINO was able to driven gene expression specific in outer integuments during ovule development.

Over 20 independent ProINO:HAP13-RNAi transgenic lines were generated, all of which showed reduced fertility to different extents as compared to wild type (Fig 7B). Two lines with strong or medium defects of ovule development were analyzed by qPCRs using maturing ovules as the materials (floral stage 11–12) (Fig 7A). These two ProINO:HAP13-RNAi lines representing medium or strong reduction of HAP13 expression (RNAi-1 and RNAi-6) were used for further analysis by CLSM and SEM. SEM of developing ovules revealed that HAP13-RNAi resulted in severe reduction of outer integument growth (Fig 7E–7F), similar to and sometimes severer than that in hap13-1, which is a weak rather than null allele of HAP13 [27,28]. At stage 3-I, the mild knockdown line showed regular two-cell-layer inner integuments symmetrically surrounding the nucellus (Fig 7G). By contrast, the growth of outer integuments, although initiated, was severely reduced (Fig 7G). For the severe knockdown line, the growth of outer integuments was arrested immediately after initiation, i.e. the enlarged cells of initiating outer integuments failed to proliferate or grow (Fig 7I). As a result, ovules at maturation stage resembled stubby tubules with only inner integuments enveloping the nucellus (Fig 7J). Downregulating HAP13 specifically in outer integuments phenocopied hap13-1, indicating that defects in ovule development in hap13-1 were not a secondary effect of HAP13 through constitutive expression elsewhere.

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Fig 7. Genetic interference of HAP13 phenocopies hap13-1 in ovule development.

(A) Relative transcript abundance of HAP13 in wild type or two ProINO:HAP13-RNAi transgenic lines (RNAi-1 and RNAi-6) by qPCRs. RNAs were extracted from maturing ovules at flower stage 11–12. Results shown are means ± SE (N = 3). Means with different letters are significantly different (One way ANOVA, Tukey-Kramer method, P<0.05). (B-D) Representative inflorescence from wild type (B) or two ProINO:HAP13-RNAi transgenic lines (C-D). Note numerous non-elongating siliques at the inflorescence of the ProINO:HAP13-RNAi transgenic lines. (E-F) SEMs of developing ovules from RNAi-1 (E) or RNAi-6 (F) transgenic line. Arrowheads point at the micropylar region. The number of displayed type among all ovules examined is shown at the bottom left. (G-J) Optical sections of developing ovules from RNAi-1 (G, H) or RNAi-6 (I, J) ProINO:HAP13-RNAi transgenic line at stage 3-I (G, I) or stage 3-V (H, J). Arrows indicate functional megaspore (FM). es, embryo sac; ii, inner integument; oi, outer integument. Dotted lines highlight the embryo sacs. The number of displayed type among all ovules examined is shown at the bottom left. Bars = 50 μm for (E-F); 10 μm for (G), (I); 25 μm for (H), (J).

https://doi.org/10.1371/journal.pgen.1006269.g007

Specifically downregulating HAP13 in outer integuments resulted in defects of embryo sac patterning such that most ovules of the ProINO:HAP13-RNAi transgenic plants contained extruding nucellus without the embryo sac at maturation (Fig 7), similar to that shown in hap13-1 (Fig 4). However, it was also possible that genetic interference of HAP13 affected ovule development and thus altered the expression specificity of ProINO, leading to the defects in embryo sac patterning. To exclude the possibility, we generated a binary vector containing two independent expression cassettes, ProINO:HAP13-RNAi and ProINO:NLS-YFP. We generated transgenic plants and applied CLSM to verify the spatial specificity of ProINO in the transgenic lines. In severely affected lines where outer integuments failed to extend, hardly any NLS-YFP signals could be observed in either cell layers within the ovules (S7 Fig). In mildly affected lines where outer integuments showed incomplete extension and wrapped inner integuments partially, NLS-YFP signals were specifically present in outer integuments (S7 Fig). These results confirmed the specific expression of ProINO even when the growth of outer integuments was compromised by downregulating HAP13.

DISCUSSIONS

We show here that the hap13-1 mutant was compromised in the asymmetric growth of outer integuments, as a result of both division and elongation defects (Figs 2 and 4). Although HAP13 is expressed in all cells during ovule development (Fig 1), its function does not seem to be crucial for inner integuments because transgenic plants expressing HAP13-RNAi in outer integuments mimicked the hap13-1 mutant (Fig 7). Despite the fact that hap13-1 contained a large portion of ovules with disrupted FGs (Fig 2) and was compromised in pollen tube guidance and reception (Fig 3), HAP13 is also not crucial for female gametogenesis because the heterozygous hap13-1 plants has normal female gametogenesis and female transmission [27] comparable to those in wild type (S1 Fig).

As a subunit of the AP1 complex, HAP13 is critical for vesicle-mediated protein sorting from the TGN/EE to the PM and to vacuoles [25,27]. SUB is the most extensively studied RLK regulating ovule development [14,33,37], in addition to its roles in epidermal patterning and cell fate determination in roots [36,43]. It was reported that SUB accumulates into BFA compartments [33]. However, it was unclear whether SUB within the BFA compartments was trapped during its secretion to the PM or from the PM through constitutive recycling, like ACR4 [44], another RLK regulating epidermal patterning [15]. By using BFA treatment at the presence of CHX, we demonstrated that SUB is constitutively internalized from the PM (S3 Fig). BFA washout resulted in the disappearance of SUB from the BFA compartments in wild type but not in hap13-1 (S3 Fig), suggesting that SUB recycles from the TGN/EE to the PM and this process depends on HAP13. The PM association of SUB was substantially affected in hap13-1 ovules (Fig 5), suggesting that HAP13-mediated SUB recycling plays a role in its PM association in ovules. Intriguingly, in root epidermal cells, no substantial difference was observed on the PM association of SUB between wild type and hap13-1 (S3 Fig), implying that the recycling pathway might be cell- or tissue-specific.

Although it is tempting to propose that HAP13-mediated sorting of SUB at the TGN/EE is critical for pattern formation during ovule development, we can not exclude the possibility that the mis-targeting of other transmembrane proteins also contributes to the observed ovule defects of hap13-1. SUB is the best studied and likely most important RLK regulating integument growth [14]. However, other RLKs such as ACR4 and ER family members are also involved in this process [15,16]. ACR4 was present both at the PM and at endosomes via vesicle trafficking [44] and thus is likely sorted via AP1. Whether ER and ERLs are dynamically trafficked via vesicles is currently unknown. However, the hap13-1 mutant showed compact inflorescence architecture as contrast to that of the ecotype Ws in which the mutant was generated [27]. Because mutations at ER and ER family members impaired cell proliferation in aerial organs and led to similar inflorescence architecture [45], it implies HAP13-dependency of ER function. Indeed, hap13-1 showed abnormal cell division during ovule development (Fig 4), which was less severe in the sub mutants [14]. A key protein involved in cytokinesis, KNOLLE, was reported to rely on HAP13 for its dynamic targeting during cell division [26]. Similar regulators during ovule development may rely on HAP13 for cell division to be properly executed.

Because PIN2 was mis-targeted in hap13-1 [25,27], while PIN1 is another long-hydrophilic looped PIN similar to PIN2 [39], it turned out to be a surprise that the asymmetric localization of PIN1 is not affected in hap13-1, either during ovule development or in roots (Figs 6 and S4). Consistently, auxin response, which plays an instructive role in ovule polarity [8,13], is not compromised in hap13-1 ovules (Fig 6), unlike the case in roots during gravitropic response [27]. The differential requirement of HAP13 for the dynamic targeting of PIN1 and PIN2 suggested distinct trafficking routes involved. Indeed, a previous report showed that Endosidin1, a chemical inducing endocytosis, defines a compartment involved in the endocytosis of PIN2 but not that of PIN1 [19]. The differential requirement of PIN1 and PIN2 on HAP13 indicates that the recycling of PIN1 and PIN2 to the PM also adopts different routes, probably through distinct regulators.

Another interesting point to note is sporophytic control of female gametogenesis. The defective pollen tube guidance and reception shown by hap13-1 suggested a compromised female gametophytic function [46,47]. However, female transmission of the hap13-1 heterozygous plants was comparable to that of wild type [27], suggesting that the female gametophytic defect of the homozygous hap13-1 plants was sporophytic. Indeed, only in the homozygous hap13-1 mutant did we observed defective FG, consistent with the result obtained by using the egg cell-specific marker ProDD45:GUS (S1 Fig). Indeed, it’s known that gametophytic development relies on surrounding sporophytic tissues [3,7,48,49]. Mutations at genes controlling integument growth, such as SUB, often interfered with the formation of embryo sacs [14]. Our results seem to suggest that outer integuments play a key role in the sporophytic controlled female gametogenesis because manipulation of vesicle trafficking routes by ProINO:HAP13-RNAi was sufficient to disrupt the patterning of FGs, suggesting a non-cell-autonomous mechanism. Interestingly, in this case, inner integuments were morphologically intact. How signals from outer integuments transmit through inner integuments to instruct the development of FG is unknown. In addition, inner integuments were suggested sufficient for female gametogenesis [50]. Whether specific signaling pathways are involved in the communication between two generations in hap13-1 will certainly be a topic for future investigations.

Materials and Methods

Plant materials and growth conditions

Arabidopsis mutants and transgenic lines, including hap13-1 [27], SUBg-YFP [35], PIN1::GFP [8], and DR5:GFP [40] were described. Arabidopsis Ws ecotype was used as the wild type. Arabidopsis plants were grown as described [51]. Stable transgenic plants were selected on half-strength MS supplemented with 30 μg/ml Basta salts, 25 μg/ml Hygromycin B, or 50 μg/ml Kanamycin.

RNA-extraction and real time quantitative PCR

Total RNAs for detecting HAP13 transcripts in ProINO:HAP13-RNAi lines were extracted from mature unfertilized ovules using a Qiagen RNeasy plant mini kit according to manufacture’s instructions. Oligo(dT)-primed cDNAs were synthesized using Superscript III reverse transcriptase with on-column DNase II digestion (Invitrogen). Real time quantitative PCRs were performed as described [51]. Primers are listed in S1 Table.

Plasmid construction

All constructs were generated using the Gateway technology (Invitrogen) except the RNAi construct. Entry vectors were generated using pENTR/D/TOPO (Invitrogen). Coding sequences or promoter sequences were cloned with the following primer pairs: ZP1781/ZP1782 for ProINO (2012 bp before the start codon of INO); ZP96/ZP97 for ProDD45 (1003 bp before the start codon of DD45). The destination vector used to generate ProDD45:GUS and ProINO:GUS were described previously [52]. Expression vectors were obtained by combining respective entry vectors and destination vectors in LR reactions using LR Clonase II (Invitrogen). HAP13-RNAi fragment (401 bp to 700 bp of its coding sequence) was amplified with the primer pair ZP1650/ZP1651. The resultant PCR products were sub-cloned into the RNAi vector pTCK303 [53] to obtain the ProUBQ10:HAP13-RNAi construct. Later, ProUBQ10 was replaced with ProINO to generate ProINO:HAP13-RNAi. A ProINO:NLS-YFP expression cassette was amplified with primers ZP3872/ZP3873 containing the restriction enzyme site SacI and EcoRI, respectively. The PCR fragment was inserted into the expression vector to generate the ProINO:HAP13-RNAi ProINO:NLS-YFP construct. Primers are listed in S1 Table.

Phenotype and histochemical analyses

Histochemical GUS staining, ovule whole-mount clearing, semi-thin sections, and SEMs were performed as described [51]. Aniline blue staining of pollen tubes growing inside pistils was performed as described [54].

Immunofluorescence labeling and fluorescence microscopy

Whole-mount immuno-fluorescence staining of ovules using an anti-LURE antibody [29] was performed as described [55]. Briefly, unfertilized mature pistils were placed in a fixative solution (3.7% paraformaldehyde, 1 mM CaCl2, 1 mM MgSO4, 50 mM HEPES (pH 7.4), 5% sucrose, pH8.0 with NaOH) for 10 min with vacuum desiccation at room temperature (RT). The fixative solution was then removed and pistils were washed three times for 10 min each with the PME buffer (50 mM PIPES, 1 mM MgCl2, 5 mM EGTA, pH6.8 with NaOH). The fixed pistils were treated further for permeation sequentially with a PME buffer, cellulose solution, and 3% IGEPAL CA-630. After permeation, pistils were sequentially incubated with the primary antibody (anti-LURE antibody, 1:300) and second antibody (FITC-labeled goat anti mouse, 1:100), followed by tissue mounting and CLSM examination. Uptake of FM4-64, BFA treatment and CLSM were performed as described [27]. Optical sectioning of ovules was performed as described [7,56].

Accession numbers

Sequence data from this article can be found in the GenBank databases under the following accession numbers: At1g60780 for HAP13, At2g21750 for DD45, At1g23420 for INO, At5g43510 for LURE1.2.

Supporting Information

S1 Fig. Defective embryo sac formation of hap13-1 is sporophytic.

(A-C) Histochemical analysis of wild-type (A), heterozygous hap13-1 (B), or homozygous hap13-1 (C) pistils transformed with ProDD45:GUS. Percentage of ovules showing GUS signals is shown on top of each image. Results are means ± standard error (s.e.m). In total, 18 pistils were analyzed for each genotype. Bars = 200 μm.

https://doi.org/10.1371/journal.pgen.1006269.s001

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S2 Fig. Protein but not transcript abundance of SUB is reduced in hap13-1.

(A-B) CLSM of a representative stage 2-III ovule from SUBg-YFP in wild type (A) or in hap13-1 (B) with the same illumination. The output images have not been brightened. Bars = 10 μm. (C) Relative transcript abundance of SUB by quantitative real-time PCRs. Results shown are means ± s.e.m. Three biological replicates were analyzed. No significant difference was observed (One-way ANOVA, Tukey-Kramer test, P>0.05).

https://doi.org/10.1371/journal.pgen.1006269.s002

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S3 Fig. Recycling of SUB to the plasma membrane requires HAP13.

CLSM of SUBg-YFP in roots of 4 DAG wild-type or hap13-1 seedlings. Con, controls; WO, washout. Arrows point at BFA compartments. Bars = 10 μm.

https://doi.org/10.1371/journal.pgen.1006269.s003

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S4 Fig. Dynamic targeting of PIN1 is independent of HAP13.

(A-F) CLSM of PIN1:GFP in roots of 4 DAG wild-type (A, C, E) or hap13-1 seedlings (B, D, F) upon 1 min FM4-64 uptake (A, B), upon BFA treatment for 50 min (C, D), or after BFA washout (E, F). Bars = 25 μm.

https://doi.org/10.1371/journal.pgen.1006269.s004

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S5 Fig. Verification of HAP13 downregulation by ProUBQ10:HAP13-RNAi.

(A-D) CLSM of 4 DAG roots of wild type (A, C) or of ProUBQ10:HAP13-RNAi transgenics (B, D) upon 1 min FM4-64 uptake followed by BFA treatment for 50 min (A, B) or after BFA washout (C, D). BFA washout in wild type (WT BFA wo) leads to tonoplast targeting of FM4-64 as seen by reduced signals at BFA compartments while in ProUBQ10:HAP13-RNAi transgenics (HAP13-RNAi BFA wo) FM4-64 is still largely trapped in BFA compartments. (E) Relative transcript abundance of HAP13 in wild type or six ProUBQ10:HAP13-RNAi transgenic lines by quantitative real-time PCRs. RNAs were extracted from 4 DAG seedlings. Results shown are means ± s.e.m. (N = 3). Means with different letters are significantly different (One way ANOVA, Tukey-Kramer test, P<0.05). Bars = 10 μm.

https://doi.org/10.1371/journal.pgen.1006269.s005

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S6 Fig. Histochemical analysis of ProINO:GUS during ovule development.

(A-F) Transverse sections of ProINO:GUS pistils at various developmental stages. Arrowheads point at outer integuments. Bars = 20 μm for (A-C); 10 μm for (D-F).

https://doi.org/10.1371/journal.pgen.1006269.s006

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S7 Fig. The specific expression of ProINO is not compromised by ProINO:HAP13-RNAi.

Representative severely (A) or mildly (B) affected ovules from the ProINO:HAP13-RNAi;ProINO:NLS-YFP transgenic plants. Shaded areas are either outer integuments (oi) or inner integuments (ii). The bright-field and YFP channel overlays are side-by-side with their corresponding YFP channel images. Hardly any signal was detected in the inner integuments. Bars = 20 μm.

https://doi.org/10.1371/journal.pgen.1006269.s007

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S1 Table. Primers used in this work.

https://doi.org/10.1371/journal.pgen.1006269.s008

(DOC)

Acknowledgments

We thank Dr. Zuhua He for the SUBg::YFP line, Dr. Xian Sheng Zhang for the pTCK303 vector and the PIN1::GFP transgenic lines.

Author Contributions

  1. Conceptualization: YZ JGW SL.
  2. Formal analysis: JGW CF HHL FRG.
  3. Funding acquisition: YZ SL.
  4. Investigation: JGW CF HHL FRG.
  5. Resources: HJL.
  6. Supervision: YZ.
  7. Writing - original draft: YZ JGW.
  8. Writing - review & editing: YZ JGW SL.

References

  1. 1. Enugutti B, Kirchhelle C, Schneitz K (2013) On the genetic control of planar growth during tissue morphogenesis in plants. Protoplasma 250: 651–661. pmid:22983223
  2. 2. Nakamura M, Kiefer CS, Grebe M (2012) Planar polarity, tissue polarity and planar morphogenesis in plants. Curr Opin Plant Biol 15: 593–600. pmid:22906885
  3. 3. Chevalier E, Loubert-Hudon A, Zimmerman EL, Matton DP (2011) Cell-cell communication and signalling pathways within the ovule: from its inception to fertilization. New Phytol 192: 13–28. pmid:21793830
  4. 4. Grossniklaus U, Schneitz K (1998) The molecular and genetic basis of ovule and megagametophyte development. Semin Cell Dev Biol 9: 227–238. pmid:9599420
  5. 5. 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. pmid:9118807
  6. 6. 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.
  7. 7. Shi DQ, Yang WC (2011) Ovule development in Arabidopsis: progress and challenge. Curr Opin Plant Biol 14: 74–80. pmid:20884278
  8. 8. Benkova E, Michniewicz M, Sauer M, Teichmann T, Seifertova D, et al. (2003) Local, efflux-dependent auxin gradients as a common module for plant organ formation. Cell 115: 591–602. pmid:14651850
  9. 9. Shiu SH, Bleecker AB (2001) Plant receptor-like kinase gene family: diversity, function, and signaling. Sci STKE 2001: re22. pmid:11752632
  10. 10. Boutte Y, Ikeda Y, Grebe M (2007) Mechanisms of auxin-dependent cell and tissue polarity. Curr Opin Plant Biol 10: 616–623. pmid:17720615
  11. 11. Kleine-Vehn J, Friml J (2008) Polar targeting and endocytic recycling in auxin-dependent plant development. Annu Rev Cell Dev Biol 24: 447–473. pmid:18837671
  12. 12. Bencivenga S, Simonini S, Benkova E, Colombo L (2012) The transcription factors BEL1 and SPL are required for cytokinin and auxin signaling during ovule development in Arabidopsis. Plant Cell 24: 2886–2897. pmid:22786869
  13. 13. Ceccato L, Masiero S, Sinha Roy D, Bencivenga S, Roig-Villanova I, et al. (2013) Maternal control of PIN1 is required for female gametophyte development in Arabidopsis. PLoS One 8: e66148. pmid:23799075
  14. 14. Chevalier D, Batoux M, Fulton L, Pfister K, Yadav RK, et al. (2005) STRUBBELIG defines a receptor kinase-mediated signaling pathway regulating organ development in Arabidopsis. Proc Natl Acad Sci U S A 102: 9074–9079. pmid:15951420
  15. 15. Gifford ML, Dean S, Ingram GC (2003) The Arabidopsis ACR4 gene plays a role in cell layer organisation during ovule integument and sepal margin development. Development 130: 4249–4258. pmid:12900442
  16. 16. Pillitteri LJ, Bemis SM, Shpak ED, Torii KU (2007) Haploinsufficiency after successive loss of signaling reveals a role for ERECTA-family genes in Arabidopsis ovule development. Development 134: 3099–3109. pmid:17652352
  17. 17. Dhonukshe P, Aniento F, Hwang I, Robinson DG, Mravec J, et al. (2007) Clathrin-mediated constitutive endocytosis of PIN auxin efflux carriers in Arabidopsis. Curr Biol 17: 520–527. pmid:17306539
  18. 18. Geldner N, Robatzek S (2008) Plant receptors go endosomal: a moving view on signal transduction. Plant Physiol 147: 1565–1574. pmid:18678748
  19. 19. Robert HS, Offringa R (2008) Regulation of auxin transport polarity by AGC kinases. Curr Opin Plant Biol 11: 495–502. pmid:18640868
  20. 20. Bassham DC, Brandizzi F, Otegui MS, Sanderfoot AA (2008) The secretory system of Arabidopsis. Arabidopsis Book 6: e0116. pmid:22303241
  21. 21. Richter S, Voss U, Jurgens G (2009) Post-Golgi traffic in plants. Traffic 10: 819–828. pmid:19416470
  22. 22. Robinson DG, Pimpl P (2014) Clathrin and post-Golgi trafficking: a very complicated issue. Trends Plant Sci 19: 134–139. pmid:24263003
  23. 23. Viotti C, Bubeck J, Stierhof YD, Krebs M, Langhans M, et al. (2010) Endocytic and secretory traffic in Arabidopsis merge in the trans-Golgi network/early endosome, an independent and highly dynamic organelle. Plant Cell 22: 1344–1357. pmid:20435907
  24. 24. Boehm M, Bonifacino JS (2001) Adaptins: the final recount. Mol Biol Cell 12: 2907–2920. pmid:11598180
  25. 25. Park M, Song K, Reichardt I, Kim H, Mayer U, et al. (2013) Arabidopsis μ-adaptin subunit AP1M of adaptor protein complex 1 mediates late secretory and vacuolar traffic and is required for growth. Proc Nat Acad Sci USA
  26. 26. Teh OK, Shimono Y, Shirakawa M, Fukao Y, Tamura K, et al. (2013) The AP-1 μ adaptin is required for KNOLLE localization at the cell plate to mediate cytokinesis in Arabidopsis. Plant Cell Physiol 54: 838–847. pmid:23543752
  27. 27. Wang JG, Li S, Zhao XY, Zhou LZ, Huang GQ, et al. (2013) HAPLESS13, the Arabidopsis mu1 adaptin, is essential for protein sorting at the trans-Golgi network/early endosome. Plant Physiol 162: 1897–1910. pmid:23766365
  28. 28. Johnson MA, von Besser K, Zhou Q, Smith E, Aux G, et al. (2004) Arabidopsis hapless mutations define essential gametophytic functions. Genetics 168: 971–982. pmid:15514068
  29. 29. Wang T, Liang L, Xue Y, Jia PF, Chen W, et al. (2016) A receptor heteromer mediates the male perception of female attractants in plants. Nature 531: 241–244. pmid:26863186
  30. 30. Takeuchi H, Higashiyama T (2012) A species-specific cluster of defensin-like genes encodes diffusible pollen tube attractants in Arabidopsis. PLoS Biol 10: e1001449. pmid:23271953
  31. 31. Okuda S, Tsutsui H, Shiina K, Sprunck S, Takeuchi H, et al. (2009) Defensin-like polypeptide LUREs are pollen tube attractants secreted from synergid cells. Nature 458: 357–361. pmid:19295610
  32. 32. Steffen JG, Kang IH, Macfarlane J, Drews GN (2007) Identification of genes expressed in the Arabidopsis female gametophyte. Plant J 51: 281–292. pmid:17559508
  33. 33. Yadav RK, Fulton L, Batoux M, Schneitz K (2008) The Arabidopsis receptor-like kinase STRUBBELIG mediates inter-cell-layer signaling during floral development. Dev Biol 323: 261–270. pmid:18771664
  34. 34. Lam SK, Cai Y, Tse YC, Wang J, Law AH, et al. (2009) BFA-induced compartments from the Golgi apparatus and trans-Golgi network/early endosome are distinct in plant cells. Plant J 60: 865–881. pmid:19709389
  35. 35. Lin L, Zhong SH, Cui XF, Li J, He ZH (2012) Characterization of temperature-sensitive mutants reveals a role for receptor-like kinase SCRAMBLED/STRUBBELIG in coordinating cell proliferation and differentiation during Arabidopsis leaf development. Plant J 72: 707–720. pmid:22805005
  36. 36. Kwak SH, Schiefelbein J (2008) A feedback mechanism controlling SCRAMBLED receptor accumulation and cell-type pattern in Arabidopsis. Curr Biol 18: 1949–1954. pmid:19097902
  37. 37. Vaddepalli P, Fulton L, Batoux M, Yadav RK, Schneitz K (2011) Structure-function analysis of STRUBBELIG, an Arabidopsis atypical receptor-like kinase involved in tissue morphogenesis. PLoS One 6: e19730. pmid:21603601
  38. 38. Bolte S, Talbot C, Boutte Y, Catrice O, Read ND, et al. (2004) FM-dyes as experimental probes for dissecting vesicle trafficking in living plant cells. J Microsc 214: 159–173. pmid:15102063
  39. 39. Zazimalova E, Murphy AS, Yang H, Hoyerova K, Hosek P (2010) Auxin transporters—why so many? Cold Spring Harbor perspectives in biology 2: a001552. pmid:20300209
  40. 40. Ulmasov T, Murfett J, Hagen G, Guilfoyle TJ (1997) Aux/IAA proteins repress expression of reporter genes containing natural and highly active synthetic auxin response elements. Plant Cell 9: 1963–1971. pmid:9401121
  41. 41. Balasubramanian S, Schneitz K (2002) NOZZLE links proximal-distal and adaxial-abaxial pattern formation during ovule development in Arabidopsis thaliana. Development 129: 4291–4300. pmid:12183381
  42. 42. Hejatko J, Blilou I, Brewer PB, Friml J, Scheres B, et al. (2006) In situ hybridization technique for mRNA detection in whole mount Arabidopsis samples. Nat Protoc 1: 1939–1946. pmid:17487180
  43. 43. Kwak SH, Shen R, Schiefelbein J (2005) Positional signaling mediated by a receptor-like kinase in Arabidopsis. Science 307: 1111–1113. pmid:15618487
  44. 44. Gifford ML, Robertson FC, Soares DC, Ingram GC (2005) ARABIDOPSIS CRINKLY4 function, internalization, and turnover are dependent on the extracellular crinkly repeat domain. Plant Cell 17: 1154–1166. pmid:15772284
  45. 45. van Zanten M, Snoek LB, Proveniers MC, Peeters AJ (2009) The many functions of ERECTA. Trends Plant Sci 14: 214–218. pmid:19303350
  46. 46. Beale KM, Johnson MA (2013) Speed dating, rejection, and finding the perfect mate: advice from flowering plants. Curr Opin Plant Biol 16: 590–597. pmid:24021868
  47. 47. Kessler SA, Grossniklaus U (2011) She's the boss: signaling in pollen tube reception. Curr Opin Plant Biol 14: 622–627. pmid:21855398
  48. 48. Sundaresan V, Alandete-Saez M (2010) Pattern formation in miniature: the female gametophyte of flowering plants. Development 137: 179–189. pmid:20040485
  49. 49. Bencivenga S, Colombo L, Masiero S (2011) Cross talk between the sporophyte and the megagametophyte during ovule development. Sex Plant Reprod 24: 113–121. pmid:21298290
  50. 50. Figueiredo DD, Kohler C (2016) Bridging the generation gap: communication between maternal sporophyte, female gametophyte and fertilization products. Curr Opin Plant Biol 29: 16–20. pmid:26658334
  51. 51. Zhou L-Z, Li S, Feng Q-N, Zhang Y-L, Zhao X, et al. (2013) PROTEIN S-ACYL TRANSFERASE10 is critical for development and salt tolerance in Arabidopsis. Plant Cell 25: 1093–1107. pmid:23482856
  52. 52. Curtis MD, Grossniklaus U (2003) A gateway cloning vector set for high-throughput functional analysis of genes in planta. Plant Physiol 133: 462–469. pmid:14555774
  53. 53. Guo J, Wang F, Song J, Sun W, Zhang XS (2010) The expression of Orysa;CycB1;1 is essential for endosperm formation and causes embryo enlargement in rice. Planta 231: 293–303. pmid:19921249
  54. 54. Li S, Ge FR, Xu M, Zhao XY, Huang GQ, et al. (2013) Arabidopsis COBRA-LIKE 10, a GPI-anchored protein, mediates directional growth of pollen tubes. Plant J 74: 486–497. pmid:23384085
  55. 55. Sauer M, Paciorek T, Benkova E, Friml J (2006) Immunocytochemical techniques for whole-mount in situ protein localization in plants. Nat Protoc 1: 98–103. pmid:17406218
  56. 56. Christensen CA, King EJ, Jordan JR, Drews GN (1997) Megagametogenesis in Arabidopsis wild type and the Gf mutant. Sex Plant Reprod 10: 49–64.