The ANGUSTIFOLIA (AN) gene is required for leaf hair (trichome) branching and is also involved in polarized expansion underlying organ shape. Here we show that the AN gene encodes a C‐terminal binding proteins/brefeldin A ADP‐ribosylated substrates (CtBP/BARS) related protein. AN is expressed at low levels in all organs and the AN protein is localized in the cytoplasm. In an mutant trichomes, the organization of the actin cytoskeleton is normal but the distribution of microtubules is aberrant. A role of AN in the control of the microtubule cytoskeleton is further supported by the finding that AN genetically and physically interacts with ZWICHEL, a kinesin motor molecule involved in trichome branching. Our data suggest that CtBP/BARS‐like protein function in plants is directly associated with the microtubule cytoskeleton.
The particular shape that plant cells adopt not only relates to their function but also affects the overall shape of plant organs. Because of this inter‐relationship between plant cell shape and organ shape, it is important to understand how cell shape is regulated. Arabidopsis thaliana is an excellent model to study this problem. Mutations in the ANGUSTIFOLIA (AN) gene affect the morphogenesis of some cell types specifically, such as leaf hairs (trichomes), as well as the shape of various organs, such that cotyledons and the rosette leaves are narrow, and the seed pods (siliques) are twisted (Redei, 1962; Hülskamp et al., 1994; Tsukaya et al., 1994; Tsuge et al., 1996).
The control of organ shape is best studied in leaves. Several mutants affect leaf morphology. Whereas one class of mutants shows general defects in cell expansion, e.g. dwarf mutants, a different class of mutants is defective in polarized cell expansion, resulting in leaves that are narrower or wider than the wild type. In particular, the latter class is instructive for an understanding of the spatial regulation of cell form. Three mutants, rotundifolia 1, (rot1), rot2 and rot3, have cells that are widened at the expense of cell length, such that leaves are short and wide without changes in cell number (Tsukaya, 1995; Tsuge et al., 1996). Mutations in the AN gene result in the opposite phenotype: leaves that are narrower and thicker than normal, but longer (Tsukaya, 1995; Tsuge et al., 1996). A detailed morphological study of both cotyledons and rosette leaves on an mutants has shown that the narrow organ phenotype is due to a defect in polarized cell expansion. Cells are generally smaller in the leaf‐width direction and larger in the leaf‐thickness direction. The an rot double mutant showed an additive phenotype, which indicated that the two processes are regulated by independent pathways (Tsukaya, 1995; Tsuge et al., 1996).
Trichomes represent a well‐studied model system for the spatial regulation of morphogenesis at the single‐cell level (Marks, 1997; Oppenheimer, 1998; Hülskamp et al., 1999). One major advantage is that trichomes have a distinct structure and polarity. Trichomes originate from single epidermal cells that stop dividing and start to endoreduplicate. After three or four endoreduplication cycles, trichome cells undergo two successive branching events. The mature trichome is a three‐branched, 500‐μm‐tall, single cell. The branching pattern provides excellent criteria by which to identify specific mutations that affect cell morphogenesis. More than 15 branching mutants have been isolated to date in which branch number is altered. Two classes of trichome branching mutants can be distinguished. The first class comprises trichome branch number mutants that also have an altered DNA content. An increased DNA content has been correlated with an increase in branch number, and trichomes with a reduced DNA content have fewer branches than the wild type (Koornneef et al., 1982; Hülskamp et al., 1994; Perazza et al., 1999). Because cellular DNA content is also correlated with cell size, it has been hypothesized that trichome branch number is controlled by cell size or cell growth. The second class consists of branch number mutants that have a normal DNA content. This class includes eight mutants that have a reduced branch number (Hülskamp et al., 1994; Folkers et al., 1997; Krishnakumar and Oppenheimer, 1999; Luo and Oppenheimer, 1999) and one mutant that has an increased branch number (Folkers et al., 1997). A detailed genetic analysis of these mutants has revealed that most double mutant combinations show an additive phenotype, suggesting that the genes act in independent pathways (Oppenheimer, 1998; Hülskamp, 2000). Double mutant combinations of underbranched mutants and the overbranched noeck (nok) mutant yielded intermediate phenotypes in most cases. Only the two‐branched mutants an and furca 4 (frc4) were epistatic to nok, suggesting that only AN and FRC4 are controlled by NOK (Folkers et al., 1997; Luo and Oppenheimer, 1999).
Little is known about the cellular and biochemical processes underlying cell morphogenesis. However, the microtubule cytoskeleton appears to be important for establishing and maintaining cell polarity. One line of evidence comes from the analysis of two mutants displaying a reduced branching phenotype. The ZWICHEL (ZWI) gene encodes a kinesin motor protein with a calmodulin‐binding domain. This strongly suggests that microtubule‐based transport is important for branch formation (Reddy et al., 1996b; Oppenheimer et al., 1997). In fass (fs) mutants, cell shape changes are correlated with an aberrant microtubule cytoskeleton, and it is therefore conceivable that the unbranched trichome phenotype in fs mutants is also caused by defects in microtubule organization (Torres‐Ruiz and Jürgens, 1994; Traas et al., 1995). Recent drug inhibitor studies support this interpretation. The application of drugs that disrupt the microtubule cytoskeleton results in a loss of trichome polarity, leading to bloated trichome cells with a reduced branch number (Szymanski et al., 1999; Mathur and Chua, 2000).
To analyze the molecular mechanisms underlying cell morphogenesis, we have isolated the AN gene. We show that AN encodes a C‐terminal binding proteins/brefeldin A ADP‐ribosylated substrates (CtBP/BARS)‐like protein and provide evidence that AN is involved in the regulation of the microtubule cytoskeleton.
Positional cloning of the AN gene
We isolated the AN gene by a positional cloning approach. Initially, the AN gene was mapped between the molecular marker nga59 and the ECERIFERUM 1 (CER1) gene on chromosome I. For further fine mapping, recombination breakpoints between AN and CER1 were mapped in ∼10 000 meiotic events from a cross between the an–cer1 double mutant (Landsberg erecta; Ler) and a wild‐type (Niederzenz; Nd) plant. Recombinants were identified in the F2 generation as an mutant plants not displaying the cer1 phenotype. In ∼2000 F1 events from the same cross, recombinant breakpoints between AN and nga59 were mapped using molecular markers (Figure 1A). A YAC and BAC/P1 contig was established between CER1 and nga59. Several new CAPS markers were developed, and the AN gene was localized to a 20 kb interval that comprises seven potential genes (for details see Figure 1A). To identify the AN gene, we sequenced genomic DNA from wild‐type and an alleles for several of the candidate genes. Allele‐specific polymorphisms were found in a gene annotated as a dehydrogenase (Figure 1B; Table I). All ethylmethane‐sulfonate (EMS) induced alleles, except an‐EM1, displayed a G to A transition leading to a stop codon or defects in splice acceptor sites. The two X‐ray‐induced mutants, an‐X1 and an‐X2, have a single base deletion and an inversion, respectively (Table I).
To determine the genomic structure of the AN gene, cDNA fragments were amplified from total RNA of young rosette leaves by RT–PCR. Sequencing of the amplified cDNA fragments revealed a 1908 bp open reading frame (ORF). Our sequences matched the cDNA clone deposited in DDBJ/EMBL/GenBank with accession No. AB032060. The comparison with the genomic sequence revealed seven exons and six introns. The transcription start site is predicted to be 37 bp downstream of the TATA box. Upstream of the AN coding sequence, a short ORF was found. The stop codon of the short ORF overlaps with the predicted start codon of the AN gene.
A 4 kb genomic fragment containing the AN coding region and the complete non‐coding region between the two flanking genes was used to complement the an mutant. The majority of the 24 transformants showed only partial rescue of the an trichome phenotype, suggesting that additional regulatory sequences are needed for full expression of the AN gene.
Sequence comparisons of the AN protein
The AN gene is predicted to encode a protein of 636 amino acids. The AN protein sequence shows similarity to proteins and motifs in DDBJ/EMBL/GenBank (Figure 1B). The presence of the nuclear targeting sequence KKRH at position 424–427 suggests that the AN protein is nuclear localized. At position 328–361, a PEST motive was found in close proximity to a cell cycle‐specific phosphorylation site (position 453–456). This suggests that AN protein is subject to cell cycle‐dependent protein degradation.
The N‐terminus of the AN protein shares sequence similarity with three protein classes, which also show similarities with each other in this region: dehydrogenases, CtBPs and BARS (Figure 2).
Sequence similarities were found to bacterial d‐2‐ hydroxy acid dehydrogenases that catalyze the NADH‐dependent reduction of 2‐oxocarboxyl acids to their corresponding 2‐hydroxycarboxyl acids. However, several amino acids, H296, D259 and E264, known to be important for the catalytic function in d‐lactate‐dehydrogenase (Asryants et al., 1989; Stoll et al., 1996; Bernard et al., 1997), are not present in AN, rendering it unlikely that AN functions as a dehydrogenase.
Sequence similarity of AN to CtBPs and BARS is less pronounced than between CtBPs and BARS themselves. Although CtBPs and BARS were initially identified by their different functions as transcriptional co‐repressors (Nibu et al., 1998; Schaeper et al., 1998) and proteins involved in the regulation of Golgi dynamics, respectively (Matteis et al., 1994; Spanfo et al., 1999), the recent findings that CtBPs can function as BARS, and vice versa (Spanfo et al., 1999), suggests that they are homologs with a dual function.
The AN gene is evolutionarily conserved in plants
Database searches revealed putative AN homologs in various plant species (Figure 3). Expressed sequence tag (EST)‐derived amino acid sequences with high sequence identity to the N‐terminal region of the AN protein were found in Glycine max, Lotus japonicus, Solanum tuberosum and Medicago truncatula, and for the middle region, in G.max, Triticum monococcum and M.truncatula. Although the EST sequence comparisons were limited to small regions, the high percentage of amino acid sequence identities found in plants, but not in other species, suggests that these genes represent true AN orthologs.
Expression analysis of AN
The pleiotropic phenotype of an mutants, affecting virtually all organs, suggests that AN is ubiquitously expressed. Attempts to study AN expression by northern blot hybridization revealed no signal, suggesting that AN is expressed either at very low levels or only in few cells. Using RT–PCR, we found AN expression in all tissues analyzed, including roots, leaves, stems and flowers (Figure 4).
In order to test whether AN regulates morphogenesis in a concentration‐dependent manner, we created plants expressing the cDNA under the control of the cauliflower 35S promotor. This construct rescues the an mutant phenotype; however, it does not result in a new phenotype in a wild‐type background. Leaf form and trichome branching were indistinguishable from the wild type (data not shown).
Intracellular localization of AN
The sequence similarity to the transcriptional co‐repressor CtBP and the presence of a nuclear localization sequence motif suggest that the AN protein might be targeted to the nucleus. In order to test this, we constructed a fusion construct with green fluorescent protein (GFP) under the control of the 35S promotor from the cauliflower mosaic virus. The intracellular localization of this fusion construct was studied in onion cells in a transient assay. The AN–GFP fusion protein was found ubiquitously in the cytoplasm and the nucleus (Figure 5A). No enrichment in specific subcellular compartments was found.
Analysis of the cytoskeleton in an mutants
As the sequence similarities of AN to other proteins do not immediately suggest in what cellular processes it might be involved, we assessed its role in the organization of the cytoskeleton, one of the major components controlling cell architecture.
The actin cytoskeleton was studied in an mutant plants expressing GFP–talin under the control of the 35S promotor (Mathur et al., 1999). The organization of the actin cytoskeleton, as visualized by the talin‐mediated localization of GFP, was indistinguishable from the wild type (data not shown).
The microtubules were visualized by a GFP–MAP4 fusion protein that was expressed under the control of the trichome‐specific GL2 promotor (Figure 5B–E). In a wild‐type background, microtubules exhibited rapid changes during development. In incipient trichomes and all stages until branch initiation is completed, cortical microtubules are organized barrel like. During these stages, microtubule density is much higher in the tip region than at the base of the trichome. After branch formation, the cortical microtubules reorientate and become orientated longitudinally (Mathur and Chua, 2000). In an mutants, the orientation of microtubules was similar to that in the wild type. A striking difference, however, was found for the relative microtubule densities within the cell. While wild‐type trichomes showed an increased microtubule density in the tip regions during all stages before and at branch formation, microtubule density in an mutants was not changed along the basal–apical axis. This visual impression was confirmed by determining the apical–basal ratios of microtubule density in wild‐type and an mutant trichomes. In the wild type, the ratio was 4/1 (n = 18) and in an mutants it was 1.2/1 (n = 26). Thus, in the wild type, microtubule density is ∼4 times higher in the tip region as compared with the basal region, whereas in an mutants no significant accumulation was found.
Genetic and molecular interaction of AN and ZWI
To assess further the potential role of AN in the regulation of the microtubule cytoskeleton, we concentrated on its relationship with the ZWI gene, which encodes a kinesin‐like motor molecule and provides a natural link to the involvement of AN in the control of microtubule organization or function (Reddy et al., 1996a,b; Oppenheimer et al., 1997; Song et al., 1997).
A genetic interaction between AN and ZWI was shown by the finding that double‐heterozygous plants of certain zwi and an allele combinations exhibit more branches than the corresponding wild types. In F1 plants from a cross between zwi‐w2 and an‐EM6, up to four branch points were observed. This effect was allele specific because combinations of these two alleles with other an or zwi alleles did not show extra branch formation (Table II). In an‐EM6 mutants, a G to A transition in the splice/acceptor site of the third intron is likely to reduce the efficiency of correct splicing. Sequence analysis of the zwi‐w2 allele revealed a C to T transition that results in a stop codon at amino acid position 72. However, there is an in‐frame AUG ∼20 bp downstream from this stop codon, so we hypothesize that re‐initiation of translation may occur.
Because this type of genetic interaction often indicates that the products of the two genes physically interact, we tested the hypothesis that AN and ZWI/KCBP physically interact by using the yeast two‐hybrid system (Durfee et al., 1993). The N‐terminal portion of ZWI/KCBP (not including the motor or calmodulin‐binding domains) was cloned into pAS1CYH2 as a fusion to the GAL4 binding domain (NtKCBP/pAS1CYH2). The AN gene was cloned into pACT2 as a fusion to the activating domain. Yeast containing the NtKCBP/pAS1CYH2 plasmid were transformed with AN/pACT2. Transformants grew on media without leucine and tryptophan (−L/−W) but not on media without leucine, tryptophan and histidine (−L/−W/−H), and the colonies from the −L/−W plates showed no β‐galactosidase activity. However, when full‐length KCBP was cloned into the pAS1CYH2 plasmid, and yeast was double‐transformed with this plasmid and AN/pACT2, colonies grew on −L/−W/−H plates and showed β‐galactosidase activity (see Figure 6, top).
Two other proteins that are known to interact with kinesin‐like calmodulin‐binding protein (KCBP) in yeast two‐hybrid assays were also tested for their interaction with AN to determine whether they also interact with it. KCBP‐interacting protein kinase (KIPK) is a protein kinase that interacts with N‐terminal and full‐length KCBP (Day et al., 2000). KIPK was isolated as a pACT2 clone, and two subdomains, one containing the N‐terminal non‐catalytic domain (Sub 1) and one containing the C‐terminal protein kinase catalytic domain (Sub 2), were also cloned into pACT2. The AN gene was cloned into pAS1CYH2 plasmid. Yeast two‐hybrid assays were performed with the KIPK full‐length and Sub 1, Sub 2 pACT2 plasmids. In addition, the AN gene was also used in an assay with a putative calcium‐binding protein (M6), which was found in a screen with the motor domain of KCBP (T.R.Thomas, A.R.Reddy and I.Day, unpublished results) and with the motor domain of KCBP in pACT2. Colonies containing the AN gene together with each of these genes grew on −L/−W plates, indicating the presence of pACT and pAS plasmids. However, these colonies did not grow on −L/−W/−H plates. The colonies grown on −L/−W plates showed no β‐galactosidase activity (see Figure 6, bottom).
The an mutant is one of the few examples in which the altered morphogenesis of whole organs can be explained by specific polarity defects at the level of the single cells. This, in combination with the specific branching phenotype of trichomes, makes the AN gene a very valuable tool to study cell morphogenesis. What have we learned from the molecular characterization of the AN gene?
The AN gene encodes a CtBP/BARS‐like protein
We cloned the AN gene by a positional approach. The presence of allele‐specific polymorphisms in nine an alleles and the rescue of the an mutant phenotype with the genomic fragment prove the identity of the AN gene.
The deduced AN protein shows overall low‐level sequence similarity to the transcriptional co‐repressor CtBP and to BARS proteins (Nibu et al., 1998; Spanfo et al., 1999). The CtBPs were initially identified as co‐repressors of the zinc‐finger transcriptional repressors Krüppel, Knirps and Snail in Drosophila (Nibu et al., 1998). CtBPs bind to a seven amino acid‐long consensus sequence at the C‐terminus of these transcription factors. BARS were identified as proteins that become ADP ribosylated upon brefeldin A treatment in rats (Matteis et al., 1994). Brefeldin A is a fungal toxin that results in the transformation of Golgi stacks into a tubular–reticular network (Lippincott‐Schwartz et al., 1989). Among others, one important aspect of the regulation of Golgi dynamics affected is the ADP ribosylation status of BARS (Matteis et al., 1994; Girolamo et al., 1995). Brefeldin A treatment leads to a ribosylation of BARS and inactivates it. Recently, it has been shown that BARS catalyzes the acylation of lysophosphatidic acid to phosphatidic acid, and that this reaction is essential for membrane fission and thereby Golgi dynamics (Weigert et al., 1999). Although initially identified by their different biochemical properties, CtBPs and BARS share a high degree of sequence identity, and the findings that BARS can bind to the same transcription factors as CtBPS and that CtBPs are subject to the brefeldin A‐dependent ADP ribosylation indicate that CtBPs and BARS can be considered homolog proteins (Spanfo et al., 1999).
The AN gene is highly conserved in plants. In DDBJ/EMBL/GenBank searches, EST fragments were found from various plant species that show high sequence identity. Within the completed genome sequence of Arabidopsis, no additional genes encoding CtBP/BARS homologs were identified, suggesting that AN represents the plant ortholog of CtBP/BARS.
Does AN link vesicle transport to microtubule‐based directional transport processes?
A presumed role for AN in the control of Golgi dynamics and vesicle trafficking is in principle consistent with its role in cell morphogenesis. However, it remains unclear why mutations in the AN gene specifically affect cell polarity rather than general morphogenesis. A potential explanation is provided by the finding that AN is involved in the organization of the microtubule cytoskeleton. This is supported by two lines of evidence. First, microtubule density is altered in a region‐specific manner in an mutant trichomes. Secondly, genetic and molecular interactions of AN were found with ZWI/KCBP. ZWI is also involved in trichome branching and zwi mutants show a phenotype similar to an mutants (Hülskamp et al., 1994; Folkers et al., 1997; Oppenheimer et al., 1997). ZWI encodes a kinesin motor molecule and was shown to move as a minus end‐directed motor molecule on microtubules (Song et al., 1997).
It is therefore conceivable that AN is required to link Golgi‐derived vesicle trafficking with directional transport processes as controlled by the microtubule cytoskeleton or, more specifically, certain motor molecules.
Materials and methods
Plant material and genetic analysis
Plants were grown at constant illumination at 23°C. The wild‐type strains used in this work were Ler, Nd and Columbia‐0 (Col). New an alleles were isolated from the F2 progeny of plants mutagenized with EMS. All alleles were induced in a Ler ecotype background, except for the an‐EM6 allele, which is in a RLD ecotype background. Agrobacterium‐mediated transformation of Arabidopsis plants was performed as described by Clough and Bent (1998).
Molecular analysis of the AN gene
The YAC, BAC and P1 libaries used to establish a chromosomal walk were obtained from the Arabidopsis Biological Resources Centre in Ohio.
For further fine mapping, new CAPS markers were generated by the following strategy: BACs were shotgun‐subcloned into pBluescriptKS+ (Stratagene), inserts of appropriate size were sequenced, and primers for genomic amplification were designed with the McVector 4.5 software (Kodak Scientific Imaging Systems, New Haven, CT). PCR products were tested for ecotype‐specific restriction enzyme polymorphisms. New molecular markers established the following differences between Ler and Nd: T2,5, GGTGCCAAATTAGAGTTTCAGGGG and TTGTGGAGCAGATATTGCGTGC shows a length polymorphism, 2.9 kb in Ler and 2.8 kb in Nd; postZat, TGCTGACTTCCCGCATCGTATG and CGTCAAAAAGCAAAAAACCGCC shows a NLAIII polymorphism, 600 bp in Ler and 580 bp in Nd; M‐left, AGCATCAACCTGTAAAGAAGGATAATC and TTCGTCAATGTAGTTTTGCTCC shows a Bsu1365I polymorphism, 210 bp in Ler and 195 bp in Nd; K8‐2, AATGAAATATAATGGTCGTGTGG and AACCACCATCCTCAAAGGCTC shows a TruI1 polymorphism, 240 bp in Ler and 230 bp in Nd; ATHACS, AGAAGTTTAGACAGGTAC and AAATGTGCAATTGCCTTC shows length polymorphism, 256 bp in Ler and 259 bp in Nd; and T2P5, TGGTAGACGATAGTGACAGGTGGA and GGATTGGCTTAAATCAATGGTGGG shows a Trul1 polymorphism, 160 bp in Ler and 145 bp in Nd.
For the genomic rescue of an mutants, a 4186 bp long genomic SpeI–HindIII fragment was cloned in pBluescriptKS and subcloned as a SacI–Cfr91 fragment into pBAR A. The 35S:AN construct was obtained by PCR amplification of a cDNA by RT–PCR using primers introducing a BamHI site on both ends and cloning it directly into pAR19. To construct the 35S:GFP4:AN fusion, the AN coding region was PCR amplified, introducing a Acc65I site and a BamHI site, and GFP4 was PCR amplified, introducing a Cfr9I and a BamHI site. The two fragments were cloned into the Cfr9I and BamHI sites of pBluescriptKS, and further subcloned into pBAR35S using Cfr9I and BamHI. The AN:GUS construct was obtained by PCR amplification of the complete non‐coding region between the AN gene and the neighboring gene, introducing a HindIII and a SalI site. This fragment was cloned into pGUS1 (Peleman, 1989). The GL2:GFP:MAP4 construct was created by cloning the NcoI–NotI GFP:MAP4‐fusion fragment into pBluescriptKS, introducing a PstI site by using the corresponding linker. Subsequently, the fragment was subcloned as a Cfr9I–SacI fragment into pBI101 containing the GL2 promoter (Szymanski et al., 1998).
For semi‐quantitative RT–PCR, we used different cycle numbers to ensure that amplifications were within the linear range for each primer pair. AN was amplified with 35 cycles using the following primers: DHMYBB, 5′‐TGCAGATTACAGTGAGGAAGTATGG; and DHF4, 5′‐CGACATTCGTCCAGAGAACC. As a control, we amplified the translation elongation factor EF1 with 25 cycles using the following primers (Liboz et al., 1990): EF1A4‐RP, 5′‐TTGGCGGCACCCTTAGCTGGATCA; and EF1A4‐UP, 5′‐ATGCCCCAGGACATCGTGATTTCAT.
Sequence comparisons were made by BLAST (Altschul et al., 1990) and BEAUTY searches (Whorley et al., 1995). Sequence alignment was performed with the multiple sequence alignment program at the BCM Search Launcher (http://dot.imgen.bcm.tmc.edu:9331/multi‐align/) and BOXSHADE version 3.21 by K.Hoffmann and M.Baron at EmbNet (http://www.ch.embnet.org/software/).
Yeast two‐hybrid analysis
AN cDNA was cloned as a BamHI fragment into pACT2 and pAS1CYH2. The N‐terminal KCBP plasmid was constructed by cloning a SacI–NotI fragment (amino acids 12–1261) of Arabidopsis KCBP into pET32b. This plasmid was then cut with NcoI, releasing a 2.8 kb fragment (amino acids 12–924), which was ligated into pAS1CYH2 digested with NcoI. KIPK/pACT2 was isolated in a two‐hybrid screen with Nt‐KCBP (Day et al., 2000). Subclones of KIPK were made using PCR‐generated fragments. Primers were designed to amplify an N‐terminal fragment from amino acids 1–347 and a C‐terminal fragment from amino acids 323–744. A BamHI site was included in the 5′ primers and a XhoI site in the 3′ primers. Primers used were: KIPK1S, 5′‐CGGGATCCGATGCCTGTAAACGATAAACC‐3′; KIPK1A, 5′‐CCGCTCGAGAGTGTCGTAAACCCAAAGAGCC‐3′; KIPK2S, 5′‐CGGGATCCCATGTCGATGGATGTA GATGGG‐3′; and KIPK2A, 5′‐CCGCTCGAGACTCAAGATGATCGCCTATGGC‐3′. pET32b and the PCR‐generated fragments were cut with BamHI and XhoI, ligated and used to transform Escherichia coli (BL21). Subclones were cut from pET32b using NcoI and XhoI, and ligated into NcoI–XhoI‐cut pACT2. All clones were sequenced to confirm the accuracy of the PCR product and in‐frame ligation. M6 is a putative calcium‐binding protein that interacts with the motor domain of KCBP (T.R.Thomas, I.Day and A.R.Reddy, manuscript in preparation). A motor domain subclone of KCBP was constructed by PCR amplification of a C‐terminal fragment coding for amino acids 860–1261, including the motor domain, calmodulin‐binding domain and a small portion of the coiled‐coil region. The primers included a site for BspHI, which, when cut, has ends compatible with NcoI. pAS1CYH2 was digested with NcoI and the fragment with BspHI; they were ligated and used to transform E.coli (DH5a).
Two‐hybrid interactions were analyzed as described previously (Day et al., 2000).
Cytological methods and images
For particle bombardment, gold particles (1 μm; Bio‐Rad, Hercules, CA) were coated with AN–GFP DNA following the manufacturer's directions. Particles were delivered into onion epidermal cells using a Biolistic PDS‐1000/He system (Bio‐Rad) with 1100 p.s.i. rupture discs under a vacuum of 62.5 mm Hg. After bombardment, the onion slices were maintained on moist filter paper in parafilm‐sealed plastic Petri dishes. Epidermal peels were mounted in tap water and observed from 24 to 72 h after bombardment.
Confocal laser‐scanning microscopy was carried out using the TCS‐NT program (Leica, Bensheim, Germany). To determine the relative density of microtubules between the tip region and the basal region of trichomes, the ratio of pixel densities of equally sized areas was determined for each trichome using the program Metamorph 4.5r4 (Adobe, Mountain View, CA). Whole‐mount GUS stainings were performed as described previously (Sessions, 1999). Images were processed with Aldus Freehand 7.0 (Aldus Corp., Seattle, WA) and Adobe Photoshop 3.0 software.
We thank members of the authors' laboratory for critically reading the manuscript. We would like to thank M.Koornneef for making available the an–cer1 double mutant. This work was supported by the Volkswagen Stiftung to M.H., a DFG grant to M.H. and a Boehringer‐Ingelheim‐Fonds fellowship to U.F.
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