Rab geranylgeranyl transferase β subunit is essential for male fertility and tip growth in Arabidopsis

Summary

Rab proteins are post-translationally geranylgeranylated by Rab geranylgeranyl transferase (RGT) αβ. Mutations in each of the RGTB genes cause a tip growth defect whereas the double mutant is male sterile.

Abstract

Rab proteins, key players in vesicular transport in all eukaryotic cells, are post-translationally modified by lipid moieties. Two geranylgeranyl groups are attached to the Rab protein by the heterodimeric enzyme Rab geranylgeranyl transferase (RGT) αβ. Partial impairment in this enzyme activity in Arabidopsis, by disruption of the AtRGTB1 gene, is known to influence plant stature and disturb gravitropic and light responses. Here it is shown that mutations in each of the RGTB genes cause a tip growth defect, visible as root hair and pollen tube deformations. Moreover, FM 1–43 styryl dye endocytosis and recycling are affected in the mutant root hairs. Finally, it is demonstrated that the double mutant, with both AtRGTB genes disrupted, is non-viable due to absolute male sterility. Doubly mutated pollen is shrunken, has an abnormal exine structure, and shows strong disorganization of internal membranes, particularly of the endoplasmic reticulum system.

Introduction

Eukaryotic cells are dependent on vesicular transport, employing protein machinery that is conserved throughout all Eukarya. Crucial players in this process are small GTPases, especially Rab proteins. Rabs possess a GTP-binding site and low intrinsic GTPase activity. In the yeast Saccharomyces cerevisiae the Rab protein family has only seven members, but in higher eukaryotes the diversification of Rab functions in specialized tissues and cell types results in as many as 57 Rabs in Arabidopsis and 60 in mammals (Pereira-Leal and Seabra, 2001). In plants the Rab family is divided into eight subfamilies, depending on the protein localization and general function in the cell (Rutherford and Moore, 2002).

All Rab proteins comprise a globular domain and an unstructured C-terminal tail of ~35 amino acids (Pfeffer, 2005). Structural motifs of the globular domain determine the Rab specificity towards interacting proteins. At the very end of the C-terminal tail lies a double cysteine motif, which serves as the target for geranylgeranylation by Rab geranylgeranyl transferase (RGT) (Rak et al., 2004; Wu et al., 2009). This modification with two 20-carbon isoprenoid chains enables anchoring of Rab proteins to membranes. A lack of this modification (due to mutations of these particular cysteines) has a disastrous effect on Rab function, since unprenylated Rabs are soluble and therefore cannot play their roles in vesicle formation, transport, and delivery (Gomes et al., 2003).

RGT is a heterodimeric enzyme built of α and β subunits (RGTA and RGTB) (Guo et al., 2008). The RGT substrate, a newly synthesized Rab protein, is initially recognized by Rab escort protein (REP; Rak et al., 2004). REP escorts the Rab to the RGT heterodimer, where the two adjacent cysteines close to the C-terminus of Rab are prenylated (Guo et al., 2008). Only the rat RGT has been crystallized so far (Pylypenko et al., 2003). The lipid substrate-binding β subunit of this enzyme (RGTB) is highly conserved in all eukaryotes (Rasteiro and Pereira-Leal, 2007). It is a one-domain protein of α-barrel fold with a helical lid at the very C-terminus covering the entrance to the lipid-binding cavity (Pylypenko et al., 2003). A model of the Rab prenylation reaction has been proposed recently (Guo et al., 2008). In this model RGTB does not contribute substantially to either the recognition or the binding affinity of the Rab protein.

The yeast S. cerevisiae null mutant in the RGTB gene, bet2, is non-viable (Ferro-Novick et al., 1991; Rossi et al., 1991), similarly to mutants in the RGTA or REP genes (bet4 and mrs6, respectively). A conditional mutant in the RGTB gene is thermosensitive for growth and accumulates endoplasmic reticulum (ER) membrane (Newman and Ferro-Novick, 1987). This mutant shows pleiotropic defects in protein transport at many different steps such as secretion to the periplasm and the vacuole or transport from the ER. Also the Rab proteins Ypt1 and Sec4 are mislocalized in this mutant (Rossi et al., 1991).

Apart from yeast, effects of loss-of-function mutations in RGTB have been studied so far only in Arabidopsis thaliana (Hala et al., 2010). Duplication of the RGTB gene has been found in several plant species, among them Arabidopsis (Rasteiro and Pereira-Leal, 2007). The AtRGTB1 and AtRGTB2 coding sequences are very similar to each other and to their mammalian homologues (56% identity for AtRGTB1) (Hala et al., 2010). According to the Genevestigator database, the AtRGTB1 transcript is abundant in all vegetative and generative tissues, and AtRGTB2 mRNA is less abundant than AtRGTB1 in the sporophyte, but is expressed at a similar level in pollen. Disruption of AtRGTB1 disturbs the growth and development of the plant shoot (Hala et al., 2010). The plants are dwarfed, show loss of apical dominance, and have abnormally developed flowers. The Atrgtb1 mutants show a gravitropic defect of the shoot and do not etiolate in the dark. Deregulation of both exo- and endocytosis as well as accumulation of unprenylated Rab proteins in the cytosol of the mutant plant hypocotyls have been observed. The lack of AtRGTB1 protein results in the reduction of Rab geranylgeranylation activity in plant extracts towards RabA proteins to ~25% that of the wild type. The effect of AtRGTB2 loss-of-function mutation has not been studied so far.

Rabs play vital roles in cells (Pfeffer, 2013). They recruit membrane-tethering and docking factors that facilitate membrane fusion (Hala et al., 2008; Heider and Munson, 2012; Kim and Brandizzi, 2012), interact with motor proteins on transport vesicles, enable vesicle motility on actin cables (Voigt et al., 2005; Samaj et al., 2006; Pei et al., 2012), and interact with enzymes of phosphatidylinositol metabolism modulating the membrane curvature and fluidity (Thole and Nielsen, 2008; Delage et al., 2013). Moreover, Rabs define the compartment identity and gather integral and peripheral membrane proteins (e.g. lipid kinases) into specific domains on an organelle by regulating protein–lipid and protein–protein interactions (Cole and Fowler, 2006).

Importantly, the Rab-dependent vesicle traffic is essential for establishing and maintaining polarity in plant cells, particularly those involved in tip growth (Voigt et al., 2005; Samaj et al., 2006; Cole and Fowler, 2006; Fu, 2010; Pei et al., 2012). Root hairs and pollen tubes are polar tubular outgrowths of trichoblasts (root hair-forming epidermal root cells) and pollen grains, respectively, which grow exclusively at their tip. Rabs are highly abundant in tip-growing cells, and defects in their synthesis or function lead to a loss of cell polarity and defects of the cell shape (Cheung et al., 2002; de Graaf et al., 2005; Preuss et al., 2006; Thole et al., 2008; Camacho et al., 2009; Szumlanski and Nielsen, 2009; Peng et al., 2011).

Here a detailed phenotypic characterization of A. thaliana mutants in the two genes encoding the β subunit of Rab geranylgeranyl transferase, Atrgtb1 and Atrgtb2, is provided. It is shown that the single mutants differ significantly from each other in flower morphology. Both Atrgtb1 and Atrgtb2 show affected polar growth of pollen tubes and root hairs. Finally, it is shown that double mutation of the two AtRGTB genes, completely abolishing Rab prenylation, results in absolute male sterility. This defect is due to impaired structure of membranes in the pollen grain and abnormal pollen exine formation.

Materials and methods

Plant material

Arabidopsis thaliana ecotype Columbia was used throughout the work. Insertion lines Atrgtb1-1 SALK_015871 and Atrgtb1-2 SALK_125416, Atrgtb2-1 SALK_027208C and Atrgtb2-2 SALK_149200 from the SALK Institute Collection were ordered from the Nottingham Arabidopsis Stock Center. Genotyping was performed with the primers designed by the T-primer design tool and LBb1.3 primer. The Atrgtb1 lines were maintained as heterozygous segregating lines due to reduced fertility of the homozygote. Homozygous plants for further experiments were identified due to the characteristic phenotype and/or genotyping. The Atrgtb2 lines were maintained as homozygous lines.

Growth conditions and media

Plants were grown in a greenhouse under a long-day (16h light) photoperiod. Plants for RNA extraction and reverse transcription–PCR (RT–PCR) were grown in a hydroponic culture in Gilbert medium in a growth chamber (AR-66L CLF Plant Climatics). Seedlings for microscopic observations of root hairs were grown on vertical plates with half-strength Murashige and Skoog (MS) medium supplemented with vitamins and 1% sucrose, solidified with 1.2% agar. In vitro pollen germination and growth were performed on solid medium overnight (16h) at 22 °C according to Boavida and McCormick (2007).

RNA extraction and RT–PCR

RNA was isolated from plant organs with the RNeasy Plant Mini Kit (Qiagen) according to the manufacturer’s protocol. After normalization of the amount of RNA, reverse transcription was carried out with an RT SuperScript II kit (Invitrogen) with an oligo(dT) primer. Semi-quantitative PCR to estimate the relative expression levels of AtRGTB1 and AtRGTB2 was carried out with the following pairs of primers: 5ʹ-AGCCTTGCGGCCATATTGTT-3ʹ and 5ʹ-CGAATTCATGAGCTCTACGTCTTCCTC-3ʹ for AtRGTB1, and 5’-GTCTAACTCCAACGCCTAAC-3ʹ and 5ʹ-CGAATTCGCG ATGGCAGACAAGCTCGT-3ʹ for AtRGTB2. Actin gene expression measured with the primer pair 5ʹ-ATTCGATCACTCAGA GCTAC-3ʹ and 5ʹ-AAGGAAGTACAGTGTCTGGA-3ʹ was used for normalization. All primers were designed with Clone Manager Suite 3 (SciEd Central) and synthesized at the Laboratory of DNA sequencing and oligonucleotide synthesis, IBB Warsaw, Poland (http://oligo.ibb.waw.pl/).

Light microscopy

The morphology of flowers and siliques was studied under an SMZ1500 stereomicroscope (Nikon Instruments) equipped with a colour camera. Image acquisition was done with Lucia software (Laboratory Imaging). The morphology of root hairs and pollen germinating in vitro was observed under an Eclipse E800 microscope (Nikon Instruments) equipped with a CCD camera (Hamamatsu). Image acquisition was performed with Lucia software (Laboratory Imaging). At least 10 visual fields of material derived from 10 different plants obtained from three independent plant cultivations were used for scoring in each case (several hundreds individual root hairs/pollen tubes in total).

In vivo pollen germination

Pollen germination in vivo was performed as follows: pistils of mature wt Col-0 flowers were prepared for manual pollination and 24h later were pollinated with appropriate pollen. After 16h, the pistils were treated with Alexander’s stain without fixation according to Cole et al. (2005) and Lalanne et al. (2004). Germination of pollen on the stigma was recorded under an inverted TE2000 microscope (Nikon Instruments). Image acquisition was performed with the use of a colour camera and NIS-Elements software (Nikon Instruments). At least 10 experiments were carried out for each line with pollen donors obtained from three independent plant cultivations.

Staining of pollen anthers with Alexander stain

Mature anthers just before dehiscence were fixed in Carnoy fixative (60% ethanol, 30% chloroform, 10% glacial acetic acid) for 2h and stained with Alexander stain according to Lalanne et al. (2004). Anthers were observed under an inverted TE2000 microscope (Nikon Instruments). Image acquisition was performed with the use of a colour camera and NIS-Elements software (Nikon Instruments). Anthers obtained from at least five plants from two independent cultivations were observed.

Confocal microscopy

Incorporation of FM 1–43 dye into growing root hairs was observed under a C1 confocal microscope (Nikon Instruments) with 488nm excitation from an argon ion laser and fluorescence detection with a 610LP emission filter. Roots of 9-day-old seedlings were transferred to 10 μM FM 1–43 solutions for 15min on ice and washed in a drop of water on a microscope slide. Observations of a single root hair were performed at the indicated time points. Images were recorded as z-stacks of ~20 optical sections with the EZ C1 image acquisition software (Nikon Instruments) and processed with EZ-C1 Viewer v.3.6 (Nikon Instruments). Experiments were performed on at least 10 roots from each mutant with at least three independent plant cultivations. Representative results are shown.

Scanning electron microscopy (SEM) and transmission electron microscopy (TEM)

For TEM observations, flowers (green buds) were fixed in 2.5% glutaraldehyde in 100mM cacodylate buffer (pH 7.2) overnight, rinsed once in the buffer, and post-fixed in 1% osmium tetroxide overnight. Samples were rinsed, dehydrated in a graded ethanol series, and finally embedded in epoxy resin. Ultrathin sections were cut with a diamond knife on an MTX ultramicrotome (RMC Boeckeler Instruments). Specimens were examined using a LEO 912AB transmission electron microscope (Carl Zeiss). For SEM observations, pollen was spilled directly on microscope tables, coated with a thin layer of gold, and examined using a LEO 1430VP scanning electron microscope (Carl Zeiss).

Statistical analysis

Statistical analysis was performed with the Graph Pad Prism program (Graphpad software). For analysis of trait inheritance, χ² test against the appropriate H₀ hypothesis, as described in Tables 1 and 2, was performed. In the case of features distributed bimodally, the exact binomial test was performed.

Table 1.

Segregation of mutant alleles in the F₁ generation of a self-cross of the Atrgtb1+/–Atrgtb2–/– mutant Atrgtb1+/–Atrgtb2–/– plants were self-crossed. Analysis of the genotypes in the F₁ generation was performed by binomial exact test against the H₀ hypothesis that one in four of the progeny carries a double mutation in RGTB genes.

Cross	n	Expected fraction of rgtb1–/–rgtb2-/-	Expected number of rgtb1–/– rgtb2-/-	Observed number of rgtb1–/–rgtb2–/–	P-value
rgtb1-1+/–rgtb2-2-/–×rgtb1-1+/–rgtb2-2–/–	82	1/4	20.5	0	5ʹ68884e-11***
rgtb1-2+/–rgtb2-1–/–×rgtb1-2+/–rgtb2-1–/–	128	1/4	32	0	1.01822e-16***

n, number of plants analysed.

***P-value <0.001.

Table 2.

Segregation of mutant alleles in the F₁ generation of the cross of pollen derived from Atrgtb1+/–Atrgtb2–/– on wt stigmaPollen derived from Atrgtb1+/–Atrgtb2–/– was crossed to wt stigma. Analysis of the genotypes in the F₁ generation was performed by binomial exact test against the H₀ hypothesis that segregation is Mendelian.

Cross	n	Expected fraction of rgtb1+/–rgtb2+/–	Expected number of rgtb1+/–rgtb2+/–	Observed number of rgtb1+/–rgtb2+/–	P-value
rgtb1-1+/–rgtb2-2–/–×wt stigma	21	1/2	11.5	0	4.76837e-07***
rgtb1-2+/–rgtb2-1–/–×wt stigma	21	1/2	11.5	0	4,76837e-07***

n, number of plants analysed.

***P-value <0.001.

The number of seeds per silique in mutant lines was compared with an appropriate experimental control. At least 20 siliques per plant line (wt or mutant) were used (4–5 plants obtained from at least two cultivations). Gaussian distribution of the obtained values was assumed. Statistical significance of the data was analysed by unpaired two-tailed Student t-test with Welch correction for inequality of variances.

The fraction (%) of abnormal pollen tubes/root hairs in mutant lines was compared with the wt. Statistical significance of the data was analysed by unpaired two-tailed Mann–Whitney test (due to the fact that the number of pollen tubes/root hairs analysed cannot be defined a priori and thus the fraction of abnormal pollen tubes/root hairs cannot be assumed to have a Gaussian distribution, the non-parametric test was chosen for analysis).

Amino acid and nucleotide sequence analysis and insert positioning

AtRGTB1 and AtRGTB2 nucleotide sequences, NM_121259 and NM_180236, respectively, were derived from the EMBL server. Corresponding amino acid sequences, NP_568259 and NP_850567, respectively, were derived from the PDB server. Alignments were performed with the T-coffee (http://www.ebi.ac.uk/Tools/msa/tcoffee) and visualized with Jalview. DNA obtained from genotyping PCR reaction of each mutant line was sequenced from the Lbb1.3 primer (http://oligo.ibb.waw.pl/). Results of the sequencing were aligned with genomic sequence of the AtRGTB1 and AtRGTB2 genes with the EMBOSS program (http://emboss.bioinformatics.nl).

Results

Characterization of AtRGTB2

The AtRGTB2 gene is located on the third chromosome, comprises nine exons, and its structure is very similar to that of its paralogue, AtRGTB1, except that the sequence corresponding to the first exon of AtRGTB2 is split into two shorter exons in the AtRGTB1 gene (Supplementary Fig. S1 available at JXB online). The nucleotide and protein sequences of AtRGTB1 and AtRGTB2 are very similar to each other, showing ~87% nucleotide identity and 94% amino acid similarity (Supplementary Fig. S1). To study the effects of single-gene disruptions of AtRGTB1 or AtRGTB2 on plant development, two different insertion mutant lines for each gene were chosen. The location of the insert was confirmed for the former (Hala et al., 2010) and determined for the latter pair of mutants (Supplementary Fig. S1).

The level of expression of both genes in different organs of plants grown in a hydroponic culture was analysed using semi-quantitative RT–PCR. In both Atrgtb1 homozygotes, the AtRGTB1 mRNA was undetectable, while it was present at a high level and ubiquitous in the wt and the two Atrgtb2 lines (Fig. 1). Consistently, the expression of the AtRGTB2 gene was down-regulated in the Atrgtb2-1 line, on contrast to the expression of the possibly truncated AtRGTB2 mRNA detectable in the Atrgtb2-2 line (this truncation may lead to partially active protein, since it probably does not destroy the overall structure of the α-barrel). The expression of AtRGTB2 in wt and Atrgtb1 homozygotes was low, but ubiquitous. Up-regulation of AtRGTB2 in Atrgtb1 homozygotes could not be observed by this experimental method.

Fig. 1.

Expression of AtRGTB1 and AtRGTB2 in Atrgtb homozygous lines. Semi-quantitative RT–PCR in different organs of plants. L, leaf; F, flower; S, stem; R, root. Actin mRNA was used as normalization control. Results representative of three independent plant cultures are shown.

To summarize, the results regarding AtRGTB expression confirmed the data from the Genvestigator database referred to by Hala et al. (2010) and those from the Bio-Array Resource website (BAR, http://bar.utoronto.ca; Toufighi et al., 2005) and were in line with the severity of the phenotypes observed in the Atrgtb1 and Atrgtb2 homozygotes (see below). Atrgtb1 plants were strongly affected, forming small rosettes and a low, branched stem with malformed flowers, and they were delayed in flowering time (Hala et al., 2010). In contrast, Atrgtb2 plants were indistinguishable from the wt plants in their morphology and the time of flowering (Supplementary Fig. S2 at JXB online).

Morphology of generative organs in Atrgtb mutants

Hala et al. (2010) described that Atrgtb1 mutants have malformed flowers with small stamens developing much later than pistils. In contrast, this kind of deformation was not found in any of the homozygous Atrgtb2 lines investigated (Fig. 2A). A closer inspection of the generative organs of both Atrgtb1 and Atrgtb2 mutants drew attention to the possibility that the self-infertility of the Atrgtb1 mutants was not due solely to disturbed flower development. Siliques of homozygous Atrgtb1 mutants were smaller and rarely contained any seeds, while both homozygous Atrgtb2 mutants produced normal siliques (Fig. 2B, C). This observation was interesting, since the pollen of Atrgtb1 mutants was able to pollinate wt stigma, and wt pollen could pollinate Atrgtb1 stigma (reciprocal crosses were succesful; see below). The Atrgtb1 pistils protruded from petals in a mature flower ready for pollination (Fig. 2; Hala et al., 2010). Thus, such flowers could not be fertilized by pollen from the same flower due to the reduced height of the stamens but could easily be pollinated by pollen from adjacent flowers from the same plant. Such pollination, however, happened only occasionally and led to the formation of very few seeds per silique (Fig. 2C). Plants grown from such seeds morphologically resembled the parent and were genotyped to be Atrgtb1. This observation suggested that, apart from the flower deformation, other reasons, related to gametophyte development, pollen tube growth, or fertilization ability, may contribute to the very low Atrgtb1 self-fertility.

Fig. 2.

Morphology of generative organs in Atrgtb mutants. (A) Flowers, scale bar=1mm. (B) Siliques, scale bar=5mm; the arrowheads indicate the unfertilized ovules. (C) Number of seeds per silique after self-pollination, n>20. Bars represent the mean ±SE. Statistical significance analysed by Student t-test, *P<0.05, **P<0.01, ***P<0.001.

The number of Atrgtb1–/– progeny in the F₁ generation after self-pollination of an Atrgtb1+/– heterozygote was not considerably lower (P =0.065 for Atrgtb1-2+/– and P=0.2459 for Atrgtb1-1+/– by the χ² test) than the fraction expected from Mendelian segregation, and for the Atrgtb2+/– mutant the corresponding fraction was exactly as expected from Mendelian segregation.

Pollen germination and tube growth are impaired in Atrgtb mutants

Pollen germination and pollen tube growth in vitro were studied on solid germination medium. After 4h or 16h, growing pollen tubes were observed under a light microscope. Pollen derived from Atrgtb1-1–/– or Atrgtb1-2–/– plants hardly germinated in these conditions. For this reason, the germination of pollen derived from heterozygous plants was studied, always in parallel to wt-derived pollen. After 4h, the emerging pollen tubes were very short and in many cases germination had not started at all; therefore, the quantitative observations were performed after 16h. Pollen derived from Atrgtb1+/– plants germinated well, but the ratio of abnormally developing pollen tubes (tip swelling or branching) was significantly higher than in wt pollen (Fig. 3A, B). Similarly, pollen derived from Atrgtb2+/– plants (also heterozygous to enable easier comparison) showed swelling and shortening of pollen tubes. Branched pollen tubes were more frequently found in the pollen derived from Atrgtb1+/– than in that derived from Atrgtb2+/–, but the difference was not statistically significant.

Fig. 3.

Male gametophyte morphology in Atrgtb mutants. (A) Morphological aberrations in pollen tubes germinated in vitro; scale bar=100 μm. (B) Frequency of pollen tube abnormalities; bars represent the mean ±SE. Statistical significance was analysed by Mann–Whitney test, ***P<0.001. (C) In vivo germination of mutant pollen on wt stigma. Alexander stain 16h after pollination; grey and pale pink pollen grains are germinated (arrows), dark purple grains are non-germinated (white arrowhead). Scale bar=100 μm. Note shrunken pollen grains deposited on stigma for Atrgtb1+/– mutant pollen (black arrowhead) and low frequency of germination for Atrgtb1–/– pollen. Representative images are shown.

To complement in vitro observations, in vivo pollen germination was studied. The method allows non-germinated grains to be distinguished from those with growing pollen tubes. Approximately 16h after pollination, most pollen grains derived from wt and Atrgtb2-1–/– plants had already emptied (grey grains in Fig. 3C, white arrow) or started germination (pink pollen grains in Fig. 3C, black arrow). Pollen derived from Atrgtb1-2–/– was scarce and always stained dark purple, which means it had not germinated, but after 24h growing pollen tubes or emptied pollen grains were occasionally observed (Fig. 3C, non-germinating pollen indicated by white arrowhead). Interestingly, many grains of pollen derived from Atrgtb1-2+/– also stained dark purple (Fig. 3C, white arrowhead). However, in the case of Atrgtb1-2+/– and, to a lesser extent, Atrgtb1-2–/–, a fraction of shrunken grains deposited on a stigma never formed pollen tubes (Fig. 3C, black arrowhead). These in vivo observations, although only qualitative, indicate that in the Atrgtb1 mutant both production and germination of pollen may be defective.

Root hair morphology is altered in Atrgtb mutants

Since tip growth is a developmental feature specific for pollen tubes and root hairs, the morphology of the latter cells in the Atrgtb1 and Atrgtb2 mutants was examined. The overall morphology of roots of the Atrgtb1 and Atrgtb2 mutants seemed normal (Supplementary Fig. S2 at JXB online; see also Hala et al., 2010). However, the frequency of abnormal, branched (sometimes even multiply) or swollen, root hairs was significantly higher for both homozygous mutants in comparison with wt plants (Fig. 4A, B). The branching was more frequent in Atrgtb1 plants than in Atrgtb2, but the difference was not statistically significant. The disturbed root hair development indicates that the functioning of these cells is compromised by disruption of either AtRGTB gene.

Fig. 4.

Root hair morphology and functioning in Atrgtb mutants. (A) Aberrations in root hair morphology; scale bar=30 μm. (B) Frequency of abnormal root hairs; bars represent the mean ±SE. Statistical significance was analysed by Mann–Whitney test, **P<0.01, ***P<0.001. (C) Time course of FM 1-43 styryl dye uptake and recycling in root hairs, confocal microscopy. Z-stacks of ~20 images from each root hair are shown. Scale bar=30 μm. Note large dye aggregates in mutant cells (arrowhead). Representative images are shown.

To test the root hair functionality, endocytosis and membrane recycling were studied in these cells by following the incorporation of a styryl dye (Ovecka et al., 2008). In wt plants the FM 1–43 dye was incorporated into the outer membrane of the cell within ~10min and later small vesicles in the cytoplasm became fluorescent (40min) (Fig. 4C), in agreement with earlier observations (Ovecka et al., 2008; Geldner et al., 2009). However, even in wt root hairs, the accumulation of vesicles in the so-called ‘inverted cone’ region in short time frames was rarely observed here, probably due to different experimental conditions compared with those of Ovecka et al. (2008). For both Atrgtb1 and Atrgtb2 mutants, the process of large vesicle formation was much faster and the staining more intense: large vesicles were visible in the cytoplasm within 10–20min (Fig. 4C). This result combined with the earlier findings regarding pollen tube growth showed that cells known to carry out intense vesicular transport (pollen tubes and root hairs) are affected by both AtRGTB2 and AtRGTB1 mutations. From the results presented it might be concluded that in the root hair these mutations have a stronger effect on exocytosis and vesicle recycling than on endocytosis.

Atrgtb1Atrgtb2 double mutation is pollen-lethal in Arabidopsis

Finally, an effort was made to construct a homozygous double mutant in both AtRGTB genes. To this end several independent crosses were set of selected Atrgtb1 mutants (homozygotes or heterozygotes) with Atrgtb2 homozygotes. In the F₂ generation, the expected Mendelian ratio of inheritance of the double mutation is 1/16. Two hundred Atrgtb1-1×Atrgtb2-2 and 202 Atrgtb1-2×Atrgtb2-1 F₂ progeny plants were analysed, but no double mutant homozygote was found, although 13 were expected assuming Mendelian inheritance.

To verify the assumption that the lack of RGT activity is lethal in plants and to investigate the stage on which lethality occurs, genotyping of plants from the F₃ generation of the initial crosses, namely the progeny of Atrgtb1+/–Atrgtb2–/– self-pollination, was performed. In F₃ progeny of both initial crosses no double mutant homozygotes were found, although 1:2:1 segregation was assumed (Table 1). To check whether the double Atrgtb1–/–Atrgtb2–/– mutation causes embryolethality, the siliques of the Atrgtb1+/–Atrgtb2–/– plants after self-pollination were opened. The number of seeds was only slightly diminished compared with the wt, with a surprisingly low number of unfertilized ovules or dead embryos (Fig. 5). Moreover, the ratio of seed germination and the lethality of young 1-week-old seedlings were the same as in the wt in both F₃ progeny lines (Fig. 5A, B).

Fig. 5.

Male gametophyte defect in the Atrgtb1Atrgtb2 double mutant. (A) Number of seeds per silique, n>20; bars represent mean ±SE. (B) Frequency of germination of seeds from self-pollination of Atrgtb1+/–Atrgtb2–/– plants, n>250. Statistical significance analysed by Student t-test, *P<0.05, ***P<0.001. (C) Siliques of an Atrgtb1+/–Atrgtb2–/– plant after self-pollination; scale bar=1mm. (This figure is available in colour at JXB online.)

This observation indicated that the double Atrgtb1–Atrgtb2– mutation causes lethality already at the stage of the male gametophyte. To verify that assumption further, wt stigmas were pollinated with pollen derived from Atrgtb1+/–Atrgtb2–/–; again no Atrgtb1+/–Atrgtb2+/– progeny was found. This observation confirmed that Atrgtb1–Atrgtb2– is pollen-lethal (Table 2).

Atrgtb mutants pollen development and ultrastructure

To check whether Atrgtb1–Atrgtb2– pollen is produced, the mature anthers of the wt and both lines of Atrgtb1-1+/–Atrgtb2-2–/– and Atrgtb1-2+/–Atrgtb2-1–/–- plants were stained with Alexander stain to visualize viable pollen grains. Wt and Atrgtb2 anthers were full of pollen grains. In other cases, empty spaces between pollen grains were visible, meaning, that not all pollen grains developed correctly (Fig. 6A). Direct visualization of pollen grains was performed with SEM (Fig. 6B). Again, all pollen grains from wt and Atrgtb2–/– plants were of normal size, showing characteristic regular exine structure. Pollen grains from Atrgtb1+/– plants were of normal length, but a few of them were hollow; however, exine structure was regular. About half of the pollen grains derived from Atrgtb1+/–Atrgtb2–/– were shrunken, many of them showing irregular exine structure.

Fig. 6.

Pollen grain development in single mutants in AtRGTB and in the Atrgtb1Atrgtb2 double mutant. (A) Alexander stain of mature anthers; scale bar=100 μm. (B) SEM images of mature pollen grains. Note that in pollen derived from Atrgtb1+/– some grains are hollow, but of normal length, but in pollen derived from Atrgtb1+/–Atrgtb2–/–, half of the grains are shrunken and many of them show abnormal exine structure; scale bar=10 μm for higher magnification and 20 μm for lower magnification. Representative images are shown. (This figure is available in colour at JXB online.)

To characterize Atrgtb1–Atrgtb2– pollen further, TEM analysis was conducted on selected lines, namely the wt and Atrgtb1-2+/– treated as the control, and the Atrgtb1-2+/–Atrgtb2-1–/– double mutant. Pollen from the Atrgtb2-1–/– line was indistinguishable from that of the wt and was therefore not included in the analysis. In contrast pollen derived from the Atrgtb1-2–/– line showed additional effects, probably of maternal (tapetum) origin, that were not visible in pollen derived from Atrgtb1-1+/– (data not shown) and therefore could not serve as an appropriate control. Immature pollen derived from closed green buds was studied (Fig. 7A, B). A high number of small vacuoles in the cytoplasm of pollen grains, the presence of two nuclei, and lack of degradation of tapetum cells surrounding the loculus in all observed specimens indicated the bicellular stage of pollen development (Quilichini et al., 2014). At this stage, wt pollen showed a uniformly structured cell wall with clearly visible exine structures (T-shaped baculae and tecta). Undisturbed membrane structures were seen inside the cell, such as rough and smooth ER, the nuclear envelope, the plasma membrane, and the tonoplast. The structure of mitochondria and plastids was also unchanged. The ultrastructure of Atrgtb1-2- pollen derived from heterozygous Atrgtb1-2+/– plants was not noticeably changed. The only difference was that the cell wall was not so uniform, showing thinner and thicker sections, as well as intrusions into the cytoplasm. Some of the grains had underdeveloped exine structures and a few were hollow, with cytoplasm remnants in the middle of the grain (data not shown). Atrgtb1–Atrgtb2– pollen grains showed looser cytoplasmic structure, occasionally leading to pollen shrinkage. The vacuoles were larger and were not round shaped as in the wt; no rough or smooth ER was visible. Many of the more strongly affected grains imploded during the preparation procedures, and remnants of cytoplasm and nuclei were visible in them. It must be emphasized here that in each studied anther derived from Atrgtb1+/–Atrgtb2–/– plants, two kinds of pollen grains were visible at a time, some of them normal, some shrunken, so the changes in the cytoplasm are most probably not an artefact of the preparation methods.

Fig. 7.

Bicellular pollen grain ultrastructure; ultrathin section TEM images of wt, Atrgtb1– and Atrgtb1–Atrgtb2– pollen. (A) Cell wall and exine ultrastructure; scale bar=500nm. (B) General view of a pollen grain; scale bar=1 μm. Representative images are shown.

To summarize, double mutation in AtRGTB genes most probably leads to a pollen development defect and this explains the lack of functional pollen in genetic crosses and lack of a double mutant in sporophytic generation of Arabidopsis.

Discussion

The aim of this study was to elucidate the effects of disruption of Rab function in plants. To this end, the morphology and development of mutant Arabidopsis lines with disruption of AtRGTB1 and/or AtRGTB2 genes were analysed. Disturbed tip growth was the major effect of partial RGTB deficiency, while total RGTB deficiency led to absolute male sterility owing to a compromised pollen grain development.

The tip growth of cells is an evolutionarily ancient process. Exocytosis is required near the growing tip to provide new portions of plasma membrane components and the material for the new cell wall. Endocytosis and membrane cycling must be coupled with exocytosis to remove an excess of the plasma membrane from the tip (Cole and Fowler, 2006; Samaj et al., 2006; Cheung and Wu, 2008; Lycett, 2008; Zhang and McCormick, 2010; Pei et al., 2012). Functional, membrane-anchored Rabs are engaged in all these processes (Pfeffer, 2013). It is not surprising, therefore, that disturbing the enzymatic activity of AtRGT, the enzyme modifying all but one (AtRabF1) of the Arabidopsis Rabs (Ueda et al., 2001), is disastrous for the plant.

Experiments presented in this work focus on the function of AtRGTB in the polar growth of plant cells. The best studied cells that show tip growth are root hairs and pollen tubes. The initiation, emergence, and growth of the root hair are strongly dependent on intracellular transport. Mutations affecting the transport and polarity-related proteins have been shown to disturb the process. In particular, a lack of an AtRabA4b effector, phosphatidylinositol-4 kinase (AtPI4Kβ; Preuss et al., 2004, 2006; Thole et al., 2008; Stenzel et al., 2008; Camacho et al., 2009) causes an abnormal growth and branching of root hairs. The types and distribution of the phenotypes described (Preuss et al., 2006) correspond well to the fraction of aberrant root hairs observed in this study in Atrgtb1 and Atrgtb2 mutants. Mutants in the Rab-interacting exocyst complex (Atexo70A1), responsible for correct docking of the exocytosis vesicles to the plasma membrane, show root hair branching as well (Synek et al., 2006). Studies on mutants lacking single Rab activity have not revealed such phenotypes, probably due to a high level of redundancy among various Rabs in plants.

Analyses of the incorporation of widely used fluorescent styryl dyes, FM1-43 and FM4-64, have proved that endocytosis is tightly coupled with secretion in root hair cells and that vesicles undergo fusion with each other as well as with the plasma membrane (Ovecka et al., 2008). The staining pattern observed for Atrgtb1 and Atrgtb2 mutants might be interpreted as slowing down of membrane recycling and exocytosis due to a lower amount of prenylated Rabs (Ovecka et al., 2008). It is not clear which particular Rabs are responsible for this effect; however, it seems reasonable to assume that it is the hypoprenylated Rabs from the RabA family known to be engaged in endosome/trans-Golgi network recycling which are resposible. Hala et al. (2010) observed a decreased tempo of both exo- and endocytosis in hypocotyls of an Atrgtb1 mutant; however, in contrast to observations presented in this study, they did not notice any changes in these processes in the root. This discrepancy could be due to this study focusing on one particular type of specialized cells, the root hairs. They are known to be highly active in transport and their membrane trafficking activity could therefore be much higher than the overall activity of other root cells and therefore more sensitive to any disturbances.

Similarly to root hairs, mutations in Rab-encoding genes have been reported to cause cell deformations in pollen tubes. AtrabA4d causes cell tip swelling and meandering (Szumlanski and Nielsen, 2009), and the double mutant AtrabD2b/c also produces abnormal pollen with swollen and occasionally branched tips (Peng et al., 2011). Similar observations were made for tobacco pollen tubes (Cheung et al., 2002; de Graaf et al., 2005). The data presented here corroborate the earlier observations on single Atrab mutants. The Atrgtb1–Atrgtb2– double mutant pollen was non-viable, as was shown by studying genotype segregation in the F₂ and F₃ generations of the Atrgtb1×Atrgtb2 cross and the reciprocal cross to wt stigma. Observations of siliques and seed germination excluded the possibility of embryolethality or seedling lethality of the double mutant. The pollen lethality of the double RGTB mutant turned out to be caused by disorganization of internal membrane structures, in particular the ER.

Accordingly, mutations in other genes coding for Rab effectors engaged in exocytosis cause similar pollen defects. Insertion mutants in Arabidopsis phosphatidylinositol-4-phosphate 5-kinases 4 and 5 cause reduced pollen germination and defects in pollen tube elongation. Overexpression of either of these kinases in Arabidopsis leads to a zigzag growth pattern or multiple branching of the pollen tubes, similar to that observed for Atrgtb mutants (Ischebeck et al., 2008). Another good example is the effect of mutations in the exocyst complex subunits Atexo70A1 and Atsec5, 6, 8, 15 (Cole et al., 2005; Hala et al., 2008). In these cases, mutant pollen causes a male-transmitted defect. Further, knock-out mutations in SNARE proteins (responsible for vesicle fusion) are lethal at the male gametophyte stage (Shirakawa et al., 2010; Uemura et al., 2012). Also, in this work, the single Atrgtb mutants showed abnormal tip growth and the double-mutated pollen was sterile.

A complete lack of Rab prenylation is lethal for a multicellular organism. as was shown here for an angiosperm plant and recently for the moss Physcomitrella patens (Thole et al., 2014), where, similarly to Arabidopsis, two copies of the RGTB gene exist. Single mutants in its haploid sporophyte do not show a phenotypic defect, but the double mutant is lethal. Similarly, knock-outs in RGTA and REP, single-copy genes in P. patens, are lethal (Thole et al., 2014). Accumulated RGT, Rabs, or their encoding mRNAs could be sufficient for the development of the Atrgtb1–Atrgtb2– female gametophyte in heterozygous Arabidopsis plants. The male gametophyte is, however, much more dependent on vesicular transport than is the mobile animal sperm, animal egg (Moosajee et al., 2009), or the non-expanding female gametophyte, and is less dependent on nutrients and hormones secreted by surrounding sporophytic tissues.

In line with the observations from P. patens, the functions of RGTB1 and RGTB2 in Arabidopsis male haploid generation seem redundant due to a similar level of expression of these two genes in pollen (Genvestigator data referred to in Hala et al., 2010). In contrast, in sporophytic tissues, the severe growth defects may be caused by insufficient dosage of RGTB rather than by distinct functions of RGTB1 and RGTB2 in the cells. This hypothesis awaits confirmation.

Supplementary data

Supplementary data are available at JXB online.

Figure S1. RGTB gene structure, chromosome location, and nucleotide and amino acid alignment.

Figure S2. General morphology of seedlings, rosettes, shoots, and roots of Atrgtb1 and Atrgtb2 mutant homozygotes in comparison with wt Col-0 plants.