Arabidopsis Qc-SNARE genes BET11 and BET12 are required for fertility and pollen tube elongation
© Bolaños-Villegas et al. 2015
Received: 11 May 2015
Accepted: 12 August 2015
Published: 2 September 2015
BET11 and 12 are required for pollen tube elongation.
Pollen tubes are rapidly growing specialized structures that elongate in a polar manner. They play a crucial role in the delivery of sperm cells through the stylar tissues of the flower and into the embryo sac, where the sperm cells are released to fuse with the egg cell and the central cell to give rise to the embryo and the endosperm. Polar growth at the pollen tube tip is believed to result from secretion of materials by membrane trafficking mechanisms. In this study, we report the functional characterization of Arabidopsis BET11 and BET12, two genes that may code for Qc-SNAREs (soluble N-ethylmaleimide-sensitive factor attachment protein receptors). Double mutants (bet11/bet12) in a homozygous/heterozygous background showed reduced transmission of the mutant alleles, reduced fertilization of seeds, defective embryo development, reduced pollen tube lengths and formation of secondary pollen tubes. Both BET11 and BET12 are required for fertility and development of pollen tubes in Arabidopsis. More experiments are required to dissect the mechanisms involved.
KeywordsArabidopsis thaliana SNAREs Fertility Pollen tube elongation
Unlike in animals, sperm cells from flowering plants are non-motile and need to be delivered to the ovule by means of a pollen tube (Kawashima and Berger 2011). Once delivered, one sperm fuses with the egg cell to result in the diploid zygote and the other fuses with the secondary nucleus to generate the triploid endosperm (Berger et al. 2008; Kawashima and Berger 2011).
For the pollen tube to perform this task, it needs to elongate in a polar way. This growth mechanism requires highly coordinated interactions between the secretory machinery, the cell wall biosynthetic machinery and the cytoskeleton (Domozych et al. 2013). For instance, newly synthesized proteins first associate with the endoplasmic reticulum (ER), then are transported to the appropriate subcellular compartment (El-Kasmi et al. 2011). This process involves the fusion of ER-derived vesicles with the cis-Golgi cisternae, followed by protein sorting to the plasma membrane or lysosomes at the trans-Golgi network (TGN), a compartment also involved in endocytosis (El-Kasmi et al. 2011; Morita and Shimada 2014). The TGN performs two main functions: it sorts cargo destined for the plasma membrane and endosomes and receives cargo from endosomal compartments (Uemura and Nakano 2013).
Several proteins take part in membrane fusion events that occur in tip-growing plant cells. Examples are Rab-GTPases, which regulate the membrane recruitment and activity of tethering factors; Rab effectors such as phosphatidylinositol kinases; ATP-driven chaperones from the Sec1/Munc18 family, also called SM proteins; and soluble N-ethylmaleimide-sensitive factor attachment protein receptors (SNAREs) (Alpadi et al. 2012; Guo and McCubbin 2012; Karnik et al. 2013; Ohya et al. 2009). SNAREs are believed to be the principal determinants of membrane fusion specificity (De Benedictis et al. 2013). These proteins, 150-300 amino acids long, feature a membrane-anchored C-terminus, α-helical heptad repeats, and a cytosolic SNARE motif that functions during membrane fusion (Guo and McCubbin 2012; Uemura et al. 2012). A fusogenic SNARE complex comprises four SNAREs, including three with a central glutamine (Gln, Q) residue within the SNARE motif (the Q SNAREs), classified as Qa-, Qb-, and Qc-, and the R-SNARE, which features a central arginine residue (Arg, R) (Fujiwara et al. 2014; Uemura et al. 2012). In these complexes, the Q-SNAREs usually reside on the target membrane, whereas the R-SNARE resides on the vesicle membrane (Karnik et al. 2013). trans-QabcR–SNARE complexes are believed to function in individual intracellular fusion steps (Furukawa and Mima 2014), their topology varies in stringency (Alpadi et al. 2012), and formation of a fusion-competent membrane microdomain requires the presence of specific lipids such as sterols, diacylglycerol, and phosphoinositides (Furukawa and Mima 2014).
Arabidopsis has about 60 different genes in six groups that encode SNARE proteins (Lipka et al. 2007); most are members of protein families with more than one gene (Sanderfoot 2007). This large number of genes may be associated with the need in higher plants for polarized secretion (Sanderfoot 2007). Nonetheless, despite the sheer number of genes, most Q-SNAREs, including the Qa-SNAREs, show partial functional redundancy (Fujiwara et al. 2014; Morita and Shimada 2014). Examples are the Arabidopsis Qa-SNARE genes SYP41, SYP42, and SYP43, which are involved in secretory and vacuolar transport and are needed to maintain the morphology of the Golgi apparatus and the TGN (Uemura et al. 2014). Several other SNARE genes involved in post-Golgi membrane trafficking include the Qb-SNAREs VTI11 and 12 and the Qc-SNAREs SYP51 and 52 (De Benedictis et al. 2013). Transient expression of SYP51 and SYP52 in protoplasts revealed functional redundancy in vesicle sorting to the vacuole, localization to the TGN and endocytic compartments, and an inhibitory effect on fusion when accumulated on the tonoplast (De Benedictis et al. 2013).
In this study, we functionally characterized two Arabidopsis genes, BET11 and BET12 (At3g58170 and At4g14455), believed to encode Qc-SNAREs (Uemura et al. 2004). These genes are Bet1/Sft1-like SNAREs that share 60 % aminoacid sequence identity with yeast Sft1 gene, and when overexpressed are able to suppress the temperature-sensitive growth defect in sft1-1 (Tai and Banfield 2001). A previous study determined that these two Arabidopsis genes (previously known as AtBS14a/b) are expressed in all plant tissues, including flowers, leaves, stem, roots and suspension cells (Uemura et al. 2004). We found that both genes were required for fertility, and that the N-terminal GFP fusion proteins localized to the Golgi apparatus, as observed in WT protoplasts. These results are in agreement with results by Uemura et al. (2004), who found that treatment of protoplasts with BFA, an inhibitor of Arf-GTPase guanine nucleotide exchange factors, caused accumulation of BET11-GFP and BET12-GFP at the Golgi. In that report the Golgi apparatus was labeled with marker Venus-SYP31, and colocalized well with BET11 and BET12 (Uemura et al. 2004). Our characterization of phenotypes in stable T-DNA double mutants suggested that the combined activity of BET11 and BET12 may be required for embryo development and proper pollen tube extrusion. Nonetheless, more work may be required to elucidate mechanistic and regulatory details related to the role the genes play at the Golgi apparatus in pollen tubes.
Molecular analysis of BET11/12
From a screen for potential gametophytic mutants, we chose the Arabidopsis At3g58170 and At4g14455 loci (BET11 and BET12) for study (Additional file 1: Table S1). Then from a subset of 18 mutant lines corresponding to 12 SNARE genes, we chose the Columbia T-DNA lines SAIL_509_C09 (bet11-1) and SALK_124063 (bet12-1) for study. Genes were selected by high expression in Arabidopsis pollen as reported by GENEVESTIGATOR (https://www.genevestigator.com). The respective amino acid sequences were analyzed by T-Coffee, a consistency-based multiple sequence alignment program (Di Tommaso et al. 2011) and the on-line repositories UNIPROT (http://www.uniprot.org) and SWISS-MODEL (swissmodel.expasy.org). Plants from each line were genotyped with specific primer pairs for their corresponding T-DNA inserts and WT locus. Single homozygous lines did not show obvious vegetative or reproductive phenotypes, but homozygous/heterozygous (HM/HZ) double mutants for bet11-1 and bet12-1 (and vice versa) showed reduced seed set. No double HM mutants were recovered.
Plant materials and growth conditions
The WT (ecotype Columbia) and T-DNA insertional lines, SAIL_509_C09 (bet11-1), and SALK_124063 (bet12-1) were obtained from the Arabidopsis Biological Resource Center (Columbus, OH, USA; http://abrc.osu.edu). Seeds were surface-sterilized in 30 % sodium hypochlorite and germinated on half-strength Murashige and Skoog medium without sucrose, then stratified at 4 °C for 96 h in the dark. Seedlings were grown at 21 °C under a 16-h photoperiod and 60 % relative humidity for approximately 5 days after the emergence of the radicle. Seedlings were then transferred to soil and genotyped with specific primer pairs for their corresponding T-DNA inserts and the WT locus. The primer sequences were for BET11-LP, 5′-GAGTAAGCCTGCCTCTGGTTC-3′, BET11-RP: 5′-TAGTACCCTGCCACGGTACAG-3′; BET12-LP: 5′-TCAAGCAAGCGGTTATGATTC-3′, BET12-RP: 5′-CACGAAAACTTACGCTTCTGG-3′, LB1:5′-GCCTTTTCAGAAATGGATAAATAGCCTTGCTTCC-3′, and LBb1.3: 5′-ATTTTGCCGATTTCGGA AC-3′. Complementation lines on the double mutant backgrounds were developed by transformation with the vector pZP221 carrying the native promoters and the full genomic sequence for either BET11 or BET12, with a GFP tag on the N-terminus. Seedlings from the T1 generation were selected on agar based on resistance to antibiotic G418 and genotyped for the corresponding T-DNA insert and GFP sequence. A modified LP primer was used for complemented bet12-1 lines. The sequence was as follows: BET12-modLP: 5′-CGGTTGGTTCACTAGTCTCT-3′.
Quantitative PCR (qPCR)
Total RNA was extracted with the RNAeasy Plant Minikit (Qiagen, http://www.qiagen.com/) from WT, bet11-1 and bet12-1 seedlings. First-stranded cDNA was prepared from total RNA with the murine leukemia virus reverse transcriptase system (Promega, http://www.promega.com/). For quantitative PCR, a Power SYBR Green I Master Mix (Applied Biosystems, http://www.appliedbiosystems.com) was used with 150–200 nM primers, 20 ng/μL cDNA, and 50 μL reverse transcriptase reaction product. Reactions were run and analyzed on the AB 7500 Real Time PCR System (Applied Biosystems). Melting curve analyses and negative controls were used to exclude artifacts and low specificity. Reactions were performed in triplicate and averaged. Primers specific for the 3′ end of transcripts were designed by use of PRIMER EXPRESS 3.0 (Applied Biosystems). The primer sequences were for BET11, forward, 5′-CCATAGATCCAGGTGAATTCTGG-3′, and reverse, 5′-GCGGTTATGAGTATCGACCTCTTC-3′; BET12, forward, 5′-AGAGACTAGTGAACCAACCGA-3′, and reverse, 5′-ACAAAACTGCTAACATGAACCCA-3′; and ACT2, forward, 5′-GGCTCCTCTTAACCCAAAGGC-3′, and reverse, 5′-CACACCATCACCAGAATCCAGC-3′ as a normalization control.
Analysis of subcellular localization of BET11 and BET12
Protoplasts prepared from leaves of 4-week-old Arabidopsis plants were co-transformed with proBET11:BET11:GFP, proBET12:BET12:GFP, Golgi marker construct 35S:Man1:GFP and nuclear marker construct 35S:ERF4:mRFP (not shown). Transformed protoplasts were observed by two-photon laser confocal microscopy and analyzed with use of Zeiss LSM Image Browser 3.5. In planta observations were not carried out.
BET11/12 double HM/HZ or HZ/HM mutants (bet11/−bet12/+, bet11/+bet12/−) were cross-pollinated with the WT to determine transmission efficiency of bet11-1 and bet12-1 alleles. The mutants were used as pollen receptors and donors. Transmission of the T-DNA alleles was analyzed by PCR with sampling of 100 progenies per cross with the WT and negative controls. Results were used to calculate the expected Mendelian segregation rate (E), the actual observed segregation rate (O) and the transmission efficiency rate (O/E × 100).
Morphological characterization of bet11-1 and bet12-1 single and double mutants
Images of seed sets were recorded after dissection of at least 30 siliques from 7-week-old plants under a Lumar V12 fluorescence stereomicroscope (Zeiss, http://microscopy.zeiss.com/microscopy) connected to an AxioCam MRc5 CCD unit. In vitro pollen germination was performed according to Lin et al. (2014). Pollen was incubated in the dark for 4 h at 25 °C, then observed under a light microscope. Pollen was collected from at least three different plants, and 100 pollen grains were used to estimate pollen viability, with three replicates. Analysis of in vivo pollen-tube growth was as described (Szumlanski and Nielsen 2009; Lin et al. 2014). Emasculated pistils from (a) WT, (b) single homozygous bet11-1 and bet12-1, (c) bet11/− bet12/+ and (d) bet11/+ bet12/− were cross-pollinated and collected after 48 h. Mature pollen morphology was analyzed by staining with 1.5 mg/mL 4′, 6-diamino-2-phenylindole (DAPI) (Vector Laboratories, http://www.vectorlabs.com) solution for 15 min in the dark, then observed under an Olympus BX51 epifluorescence microscope coupled to an Olympus DP70 CCD unit (Olympus, http://www.olympus-global.com/en/corc/company/lifescience).
The mutant alleles bet11-1 and bet12-1 show distorted segregation rates
Our analyses of the phenotype of bet11-1 and bet12-1 single homozygous plants did not reveal any obvious defects in vegetative or reproductive growth. Moreover, PCR genotyping indicated that the mutants segregated in a 3:1 Mendelian ratio, which suggests that transmission of the T-DNA allele was more or less efficient. We could not isolate double homozygous bet11/bet12 mutants. In fact, the corresponding homozygous/heterozygous mutants segregated in highly distorted, non-Mendelian ratios. In the bet11/−bet12/+ mutant (HM/HZ), the bet11-1 T-DNA allele segregated with P = 1.49 × 10−7, and in the bet11/+ bet12/− mutant (HZ/HM), the bet12-1 T-DNA allele segregated with P = 2.79 × 10−10 (Fig. 1c). These extremely significant values suggested reduced efficiency in the transmission of the T-DNA alleles caused by gametophyte or embryo lethality.
To better understand the reason for these defects, we analyzed the expression of the BET11 and BET12 genes in the WT and corresponding complementation lines, which carried the full genomic sequence driven by the native promoter. The expression of both genes was lower in the mutants than the WT (Fig. 1d). For instance, for homozygous bet11-1, the expression of BET11 was reduced to 0.35 ± 0.04 (vs. 1.00 ± 0.10 in the WT) and 0.82 ± 0.09 in the heterozygous background, whereas for homozygous bet12-1, the expression of BET12 was reduced to 0.23 ± 0.15 (vs. 0.90 ± 0.10 in the WT), and 0.77 ± 0.07 in the heterozygous background. For the complementation lines, the expression of both genes was increased to 0.54 ± 0.06 and 0.64 ± 0.12, respectively (Fig. 1d). Therefore, the bet11/− and bet12/− alleles appeared to be knockdown alleles that show reduced expression at the 3′ end.
BET11 and BET12 proteins may reside at the Golgi apparatus
To better understand the function of the putative BET11 and BET12 proteins, we examined the localization patterns of their respective N-terminal, GFP-fusion proteins in Arabidopsis leaf protoplasts isolated from 4-week old Arabidopsis plants. Both GFP-tagged proteins showed some level of colocalization with the Golgi marker Man1 (Man1:RFP), especially BET12, which suggests that both proteins may reside at the Golgi apparatus (Fig. 1e). These results are in line with previous work (Uemura et al. 2012) and are in agreement with bioinformatic modeling of the function of both genes. For instance, alignment of amino acid sequences by use of T-Coffee suggested conservation between the putative Arabidopsis BET11 and BET12 proteins compared to the yeast homolog Sft1 (Additional file 2: Figure S1a). Results from the UNIPROT database indicated that both loci appear to encode canonical Qc-SNARE proteins that feature a SNARE coiled-coil domain, a transmembrane domain, a vesicular topological domain, and for BET12, a predicted phospho-serine site at residue 56 (Additional file 2: Figure S1b–c) that may regulate posttranslational dynamics. Moreover, SWISS-MODEL results suggest that each locus encodes a single chain able to assemble as a heterotetramer (Additional file 2: Figure S1b–c). This high level of similarity between both predicted proteins may indicate functional redundancy.
Transmission of the homozygous mutant alleles is reduced in pollen
Transmission of the heterozygous bet11-1 and bet12-1 alleles is impaired in bet11/12 double mutants
Segregating T-DNA allele
Expected segregation rate (E)
Observed segregation rate (O)
Transmission efficiency (O/E) × 100 (%)
bet11 HM/bet12 HZ (female) × WT (male)
WT (female) × bet11 HM/bet12 HZ
bet12 HM/bet11 HZ (female) × WT (male)
WT (female) × bet12 HM/bet11 HZ
BET11 and BET12 genes are required for fertilization
BET11 and BET12 genes are required for pollen tube elongation
Moreover, in vivo pollen germination experiments with WT pollen in single and double mutant bet11/bet12 flowers did not reveal any apparent defects in the germination and elongation of pollen tubes within female tissues (Additional file 3: Figure S2a, upper panel). Use of the single mutants bet11/− and bet12/− as pollen donors and WT flowers as the female did not reveal any defects (Additional file 3: Figure S2a, lower panel). Nonetheless pollen from the bet11/−bet12/+ and bet11/+ bet12/− double mutants appeared to show poor germination and elongation; in fact, few pollen tubes were observed within female tissues after 48 h (Additional file 3: Figure S2a, lower panel, right side). Moreover, staining with DAPI indicated no significant differences in the morphology of mutant pollen grains; most grains (98–99 %) were tricellular and contained an identifiable vegetative cell and two sperm nuclei (Additional file 3: Figure S2b–c).
Plant reproduction starts with the deposition of pollen grains onto the stigma of the pistil. After the grains germinate, the pollen tubes grow through the transmitting tract of the style and septum to reach the embryo sac, where double fertilization takes place (Kaya et al. 2014). Pollen tubes expand by tip growth, whereby the apex of the cell grows much faster than the other sides, thereby generating an elongated structure (Kaya et al. 2014). In this study we show that two putative, highly similar Qc-SNARE genes, BET11 and BET12, are involved in pollen tube growth and that double mutants in a homozygous/heterozygous condition show reduced transmission of the heterozygous alleles (Table 1), defects in fertilization and embryo development (Fig. 2), reduced pollen tube elongation and the extrusion of secondary pollen tubes (Fig. 3), which suggests possible loss of polarity. The respective N-terminal GFP-tagged proteins mostly localized to the Golgi in protoplasts, so they may play a role during endomembrane trafficking (Fig. 1).
The SNAREs and other fusogenic determinants have important roles during pollen tube development. For instance, development of secondary pollen tubes (as in bet11/bet12 mutants) has been linked to reduced expression of the PIP5K4 gene, which encodes the phosphatidylinositol-4-monophosphate 5-kinase 4, an enzyme in charge of the conversion of phosphatidylinositol (4,5)-bisphosphate (or PtdIns(4,5)P2). This molecule plays key roles in actin dynamics, vesicle trafficking, and ion transport (Sousa et al. 2008). Lily pollen tubes overexpressing the actin-binding protein (ABP) LILIM1 showed protrusion of multiple tubes from one pollen grain and aggregation of FM4-64-labeled compartments, which suggests possible cross-talk between endomembrane trafficking and cytoskeletal organization (Wang et al. 2008). In fact, Rho GTPases such as ROP1 and interacting protein RIC3 are believed to function as spatial regulators of ABPs including F-actin, profilin and formin and thus help determine growth polarity (Chebli et al. 2013; Cheung et al. 2010).
Within the Ras superfamily of proteins, Rab GTPases are thought to be required for selective vesicle attachment to target vesicles (Carr and Rizo 2010). When bound to GDP, RABs are inactive, but when bound to GTP, they become activated and interact with several effector proteins (Ung et al. 2013), including SNAREs, during the tethering of cargo at post-Golgi compartments (Cai et al. 2007). In pollen tubes, loss of Arabidopsis RABA4D expression led to disrupted polar growth and changes in cell wall patterning and compromised in vivo pollen tube growth and guidance (Szumlanski and Nielsen 2009). Conversely, overexpression of C-terminal–truncated versions of the Rho guanine exchange factor AtRopGEF12 also caused disturbed pollen tube growth, including isotropic growth (Zhang and McCormick 2007).
Moreover systems biology model based on the behavior of Arabidopsis RABA4D required the activity of SNAREs for vesicle fusion and GTPases for budding (Kato et al. 2010). In this model, specific GTPases favor budding from specific compartments at specific rates, whereas the rate of vesicle fusion depends on the rate of SNARE pairing between the vesicle and the target (Kato et al. 2010). However it is not known whether this model applies to bet11/bet12 mutants.
Recent work has shown that the Arabidopsis Qc-SNARE SYP61 and Qa-SNARE SYP121 are required for coordinated targeting to the plasma membrane of aquaporin PIP2;7, a process that requires anteroretrogade passage through the TGN during secretion or during retrograde uptake from the plasma membrane (Hachez et al. 2014). This process also appears to mediate expansion of root hairs (Hachez et al. 2014), which are cells well known for showing SNARE-dependent polarized tip growth (Larson et al. 2014).
In Arabidopsis, defects in the expression of SNARE genes induce collapse of Golgi compartments into the endoplasmic reticulum (ER) (Chatre et al. 2005). A similar phenomenon was reported for the R-SNARE gene SEC22 in Arabidopsis mutants (El-Kasmi et al. 2011), which show fragmentation of Golgi stacks, presumably because of blocked membrane fusion during anterograde or retrograde ER to Golgi trafficking (El-Kasmi et al. 2011). A similar process might occur in bet11/bet12 double mutant pollen tubes. Nonetheless, examination of endomembrane compartments by transmission electron microscopy is required to address this question and help determine whether bet11/bet12 mutants are required for maintenance of proper structure of the Golgi or TGN in pollen tubes.
Protein-driven membrane fusion events are essential in all organisms (Pérez-Vargas et al. 2014). They are crucial to achieve intracellular trafficking, neurotransmitter secretion, cell mating and fertilization. They are also key to the development of tissues and organs in multicellular organisms (Pérez-Vargas et al. 2014).
In this study, we characterized the role of two putative Arabidopsis Qc-SNARE genes, BET11 and BET12, in plant growth. Results from the characterization of T-DNA double mutants strongly suggest that these two genes perform largely overlapping functions during fertilization. Both are required during polarized extrusion of pollen tubes, as evidenced by reduced pollen tube length and the development of secondary pollen tubes (Table 1). Genetic data also suggests a role for both genes during embryo development, especially for BET12 (Table 1). These roles seem to be a departure from the role that bet11p plays in yeast, in which the bet1-1 allele leads only to minor growth defects as compared with the WT (Rogers et al. 2013). This difference in behavior could be interpreted as an evolutionary gain of function for BET Qc-SNAREs in multicellular eukaryotes. If so, BET11/BET12 homologs in plants and metazoans may have a specialized role during polarized growth and embryo development.
In conclusion, Arabidopsis BET11 and BET12 genes are required for polarized growth in pollen and for embryo development. Nonetheless, more work is required to identify the role of the BET11 and BET12 in anterograde and retrograde traffic, whether fragmentation of the Golgi apparatus occurs in bet11/bet12 mutants, and to determine the type of cargo specified by BET11 and BET12 in vesicles. We believe that this study may pave the way for further characterization of the function played by these two genes during reproduction and uncover interactions unknown at the present time.
PBV and GYJ designed the research. PBV and AG performed the experiments. PBV and GYJ analyzed data. PBV and GYJ wrote the article. All authors read and approved the final manuscript.
The authors thank Ms. Mei-Jane Fang for assistance with DNA sequencing and capillary PCR (DNA Analysis Core Laboratory, Academia Sinica, Taiwan). The authors also thank Dr. Frédéric Berger for valuable input at the initial stages of this project. This work was supported by research grants from Academia Sinica (Taiwan), the National Science and Technology Program for Agricultural Biotechnology (NSTP/AB, 098S0030055-AA), Taiwan, and the National Science Council (NSF; 99-2321-B-001-036-MY3), Taiwan, to G.Y. Jauh; and a study-abroad contract from the University of Costa Rica to P. Bolaños-Villegas.
Compliance with ethical guidelines
Competing interests The authors declare that they have no competing interests.
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- Alpadi K, Kulkarni A, Comte V, Reinhardt M, Schmidt A, Namjoshi S, Mayer A, Peters C (2012) Sequential analysis of Trans-SNARE formation in intracellular fusion. PLoS Biol 10:e1001243PubMedView ArticlePubMed CentralGoogle Scholar
- Berger F, Hamamura Y, Ingouff M, Higashiyama T (2008) Double fertilization: caught in the act. Trends Plant Sci 13:437–443PubMedView ArticleGoogle Scholar
- Cai H, Reinisch K, Ferro-Novick S (2007) Coats, tethers, Rabs, and SNAREs work together to mediate the intracellular destination of a transport vesicle. Dev Cell 12:671–682PubMedView ArticleGoogle Scholar
- Carr CM, Rizo J (2010) At the junction of SNARE and SM protein function. Curr Opin Cell Biol 22:488–495PubMedView ArticlePubMed CentralGoogle Scholar
- Chatre L, Brandizzi F, Hocquellet A, Hawes C, Moreau P (2005) Sec22 and Memb11 are v-SNAREs of the anterograde endoplasmic reticulum-Golgi pathway in tobacco leaf epidermal cells. Plant Physiol 139:1244–1254PubMedView ArticlePubMed CentralGoogle Scholar
- Chebli Y, Kroeger J, Geitmann A (2013) Transport logistics in pollen tubes. Mol Plant 6:1037–1052PubMedView ArticleGoogle Scholar
- Cheung AY, Niroomand S, Zou YJ, Wu HM (2010) A transmembrane formin nucleates subapical actin assembly and controls tip-focused growth in pollen tubes. Proc Natl Acad Sci USA 107:16390–16395PubMedView ArticlePubMed CentralGoogle Scholar
- De Benedictis M, Bleve G, Faraco M, Stigliano E, Grieco F, Piro G, Dalessandro G, Di Sansebastiano GP (2013) AtSYP51/52 functions diverge in the post-Golgi traffic and differently affect vacuolar sorting. Mol Plant 6:916–930PubMedView ArticleGoogle Scholar
- Di Tommaso P, Moretti S, Xenarios I, Orobitg M, Montanyola A, Chang JM, Taly JF, Notredame C (2011) T-Coffee: a web server for the multiple sequence alignment of protein and RNA sequences using structural information and homology extension. Nucleic Acids Res 39:W13–W17PubMedView ArticlePubMed CentralGoogle Scholar
- Domozych DS, Fujimoto C, LaRue T (2013) Polar expansion dynamics in the plant kingdom: a diverse and multifunctional journey on the path to pollen tubes. Plants 2:148–173View ArticleGoogle Scholar
- El-Kasmi F, Pacher T, Strompen G, Stierhof YD, Muller LM, Koncz C, Mayer U, Jurgens G (2011) Arabidopsis SNARE protein SEC22 is essential for gametophyte development and maintenance of Golgi-stack integrity. Plant J 66:268–279PubMedView ArticleGoogle Scholar
- Fujiwara M, Uemura T, Ebine K, Nishimori Y, Ueda T, Nakano A, Sato MH, Fukao Y (2014) Interactomics of Qa-SNARE in Arabidopsis thaliana. Plant Cell Physiol 55:781–789PubMedView ArticleGoogle Scholar
- Furukawa N, Mima J (2014) Multiple and distinct strategies of yeast SNAREs to confer the specificity of membrane fusion. Sci Rep 4:4277. doi:10.1038/srep04277 PubMedView ArticlePubMed CentralGoogle Scholar
- Guo F, McCubbin AG (2012) The pollen-specific R-SNARE/longin PiVAMP726 mediates fusion of endo- and exocytic compartments in pollen tube tip growth. J Exp Bot 63:3083–3095PubMedView ArticlePubMed CentralGoogle Scholar
- Hachez C, Laloux T, Reinhardt H, Cavez D, Degand H, Grefen C, De Rycke R, Inzé D, Blatt MR, Russinova E, Chaumont F (2014) Arabidopsis SNAREs SYP61 and SYP121 coordinate the trafficking of plasma membrane aquaporin PIP2;7 to modulate the cell membrane water permeability. Plant Cell. doi:10.1105/tpc.114.127159 Google Scholar
- Karnik R, Grefen C, Bayne R, Honsbein A, Kohler T, Kioumourtzoglou D, Williams M, Bryant NJ, Blatt MR (2013) Arabidopsis Sec1/Munc18 protein SEC11 is a competitive and dynamic modulator of SNARE binding and SYP121-dependent vesicle traffic. Plant Cell 25:1368–1382PubMedView ArticlePubMed CentralGoogle Scholar
- Kato N, He HY, Steger AP (2010) A systems model of vesicle trafficking in Arabidopsis pollen tubes. Plant Physiol 152:590–601PubMedView ArticlePubMed CentralGoogle Scholar
- Kawashima T, Berger F (2011) Green love talks; cell-cell communication during double fertilization in flowering plants. AoB Plants plr015. doi: 10.1093/aobpla/plr015
- Kaya H, Nakajima R, Iwano M, Kanaoka MM, Kimura S, Takeda S, Kawarazaki T, Senzaki E, Hamamura Y, Higashiyama T, Takayama S, Abe M, Kuchitsu K (2014) Ca2+-activated reactive oxygen species production by Arabidopsis RbohH and RbohJ is essential for proper pollen tube tip growth. Plant Cell 26:1069–1080PubMedView ArticlePubMed CentralGoogle Scholar
- Larson ER, Domozych DS, Tierney ML (2014) SNARE VTI13 plays a unique role in endosomal trafficking pathways associated with the vacuole and is essential for cell wall organization and root hair growth in arabidopsis. Ann Bot 114:1147–1159PubMedView ArticlePubMed CentralGoogle Scholar
- Lin SY, Chen PW, Chuang MH, Juntawong P, Bailey-Serres J, Jauh GY (2014) Profiling of translatomes of in vivo-grown pollen tubes reveals genes with roles in micropylar guidance during pollination in Arabidopsis. Plant Cell 26:602–618PubMedView ArticlePubMed CentralGoogle Scholar
- Lipka V, Kwon C, Panstruga R (2007) SNARE-ware: the role of SNARE-domain proteins in plant biology. Ann Rev Cell Dev Biol 23:147–174View ArticleGoogle Scholar
- Morita M, Shimada T (2014) The plant endomembrane system—a complex network supporting plant development and physiology. Plant Cell Physiol 55:667–671PubMedView ArticleGoogle Scholar
- Ohya T, Miaczynska M, Coskun U, Lommer B, Runge A, Drechsel D, Kalaidzidis Y, Zerial M (2009) Reconstitution of Rab- and SNARE-dependent membrane fusion by synthetic endosomes. Nature 459:1091–1097PubMedView ArticleGoogle Scholar
- Pérez-Vargas J, Krey T, Valansi C, Avinoam O, Haouz A, Jamin M, Raveh-Barak H, Podbilewicz B, Rey FA (2014) Structural basis of eukaryotic cell-cell fusion. Cell 157:407–419PubMedView ArticleGoogle Scholar
- Rogers JV, Arlow T, Inkellis ER, Koo TS, Rose MD (2013) ER-associated SNAREs and Sey1p mediate nuclear fusion at two distinct steps during yeast mating. Mol Biol Cell 24:3896–3908PubMedView ArticlePubMed CentralGoogle Scholar
- Sanderfoot A (2007) Increases in the number of SNARE genes parallels the rise of multicellularity among the green plants. Plant Physiol 144:6–17PubMedView ArticlePubMed CentralGoogle Scholar
- Sousa E, Kost B, Malhó R (2008) Arabidopsis phosphatidylinositol-4-monophosphate 5-kinase 4 regulates pollen tube growth and polarity by modulating membrane recycling. Plant Cell 20:3050–3064PubMedView ArticlePubMed CentralGoogle Scholar
- Szumlanski AL, Nielsen E (2009) The Rab GTPase RabA4d regulates pollen tube tip growth in Arabidopsis thaliana. Plant Cell 21:526–544PubMedView ArticlePubMed CentralGoogle Scholar
- Tai WCS, Banfield DK (2001) AtBS14a and AtBS14b, two Bet1/Sft1-like SNAREs from Arabidopsis thaliana that complement mutations in the yeast SFT1 gene. FEBS Lett 500:177–182PubMedView ArticleGoogle Scholar
- Uemura T, Nakano A (2013) Plant TGNs: dynamics and physiological functions. Histochem Cell Biol 140:341–345PubMedView ArticleGoogle Scholar
- Uemura T, Ueda T, Ohniwa RL, Nakano A, Takeyasu K, Sato MH (2004) Systematic analysis of SNARE molecules in Arabidopsis: dissection of the post-Golgi network in plant cells. Cell Struct Funct 29:49–65PubMedView ArticleGoogle Scholar
- Uemura T, Kim H, Saito C, Ebine K, Ueda T, Schulze-Lefert P, Nakano A (2012) Qa-SNAREs localized to the trans-Golgi network regulate multiple transport pathways and extracellular disease resistance in plants. Proc Natl Acad Sci USA 109:1784–1789PubMedView ArticlePubMed CentralGoogle Scholar
- Uemura T, Suda Y, Ueda T, Nakano A (2014) Dynamic behavior of the trans-Golgi network in root tissues of Arabidopsis revealed by super-resolution live imaging. Plant Cell Physiol 55:694–703PubMedView ArticleGoogle Scholar
- Ung N, Brown MQ, Hicks GR, Raikhel NV (2013) An approach to quantify endomembrane dynamics in pollen utilizing bioactive chemicals. Mol Plant 6:1202–1213PubMedView ArticleGoogle Scholar
- Wang HJ, Wan AR, Jauh GY (2008) An actin-binding protein, LlLIM1, mediates calcium and hydrogen regulation of actin dynamics in pollen tubes. Plant Physiol 147:1619–1636PubMedView ArticlePubMed CentralGoogle Scholar
- 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 104:18830–18835PubMedView ArticlePubMed CentralGoogle Scholar