Identification of Two Maize Mutants with Impaired Stalk and Leaf Development

Two independent semi-dwarf mutants, dil474 and dil338 with similar phenotypes were isolated from an EMS mutagenized PHN4611 population. Homozygous mutant plants have reduced plant heights due to shorter internodes (Figure 1A, 1B). Both dil1 mutants also have more erect, shorter but wider, crinkled leaves (Figure 1A, 1D, 1E and 1F). Leaf angles, leaf length and width, internode length and plant height were measured in 12 mature plants from each genotype (homozygous wild type, dil338 and dil474) to better quantify the variations. The mutant plants are significantly different from the wild type in all the parameters measured (Table 1). In addition, the root and seedling lengths of one-week-old mutant seedlings seem to be shorter than that of wild type seedlings (Figure 1C). In summary, the dil1 mutations result in reduced plant height and changes in leaf shape.

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Figure 1. Characterization of dil1 mutant phenotype.

A. dil1 mutant plants (9-weeks-old) are characterized by their reduced plant height and smaller leaf angles as compared to the wild type plants. B. Stalks of wild type and dil1 mutant plants (9-weeks-old) with leaves and ears removed. C. Wild type (upper) and dil338 mutant (lower panel) seedlings six days after germination in dark. D. Abaxial surface of the first leaf below the ear in 9-weeks-old wild type and dil1 mutant plants. E and F. Close look of abaxial (E) and adaxial (F) surfaces of the first leaf below the ear in 9-weeks-old wild type and dil1 mutant plants.

https://doi.org/10.1371/journal.pone.0037040.g001

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Table 1. Comparison of leaf angle, leaf length and width, internode length and plant height between wild-type and dil1 mutant plants.

https://doi.org/10.1371/journal.pone.0037040.t001

Abnormal Leaf Epidermal and Stalk Parenchyma Cells in dil1 Mutant Plants

Leaf (V3 and post-flowering stages) and stalk (post-flowering stage) sections were examined with a multiphoton laser scanning microscope (LSM) to determine the cytological variations in dil1 mutants. The leaf epidermal cells of dil1 mutant plants are irregular in size and shape, and are arranged more randomly when compared to those of the wild type at V3 (Figure 2A and 2B) and post-flowering stages (Figure 2C and 2D). The reduced length/width ratio in leaf epidermal cells may result in shorter and wider leaves in mutant plants. The reduced cell expansion along the longitudinal dimension may cause the cells to expand towards the adaxial or abaxial surfaces of the leaves, which results in bulging cells and wrinkled leaf surfaces. Stalk parenchyma cells in dil1 mutants at the post-flowering stage are irregular in shape and distribution, and are significantly smaller than those of the wild-type plants (Figure 2E, 2F, 2G and 2H). The smaller cell size at least partially explains the shorter internodes in mutant plants.

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Figure 2. Cytological observations of dil1 mutant.

A and B: Multiphoton laser scanning micrograph (LSM) images of the adaxial surface of leaf epidermis from the 2^nd leaf of V3 stage wild type (WT) (A) and dil338 (B) seedlings. C and D: Multiphoton LSM images of the adaxial surface of leaf epidermis at post-flowering stage in WT (C) and dil338 (D) plants. E and F: Multiphoton LSM images of stalk parenchyma cells from third internode (from base) at post-flowering stage in WT (E) and dil338 (F) plants. G and H: Multiphoton LSM images of stalk parenchyma cells from ninth internode (from base) at post-flowering stage in WT (G) and dil338 (H) plant. I and J: The adaxial surface of WT leaf with flat blade and regularly spaced macrohairs (I), and dil338 with an undulating leaf surface and clustered macrohairs (J, arrows), from fully expanded leaves. K and L: Stomata in the adaxial surface of WT leaves with paired subsidiary cells (K), whereas in dil338 the stomata sometimes had single subsidiary cells (arrows) (L).

https://doi.org/10.1371/journal.pone.0037040.g002

In addition to the observed cell size and shape defects, defects in patterning of specific cell types on the adaxial surface of leaves were observed using a scanning electron microscope (SEM). In particular, the spacing of macrohairs was irregular, with about half of the macrohairs being clustered (Figure 2I and 2J). In addition, stomatal defects, where approximately 10% of stomata had only a single subsidiary cell, compared to the normal paired subsidiary cells seen in wild type, were observed (Figure 2K and 2L).

Fine Mapping of dil1

A positional cloning approach was used to clone dil1. Two F₂ populations (F₂-dil338 and F₂-dil474) were generated by crossing homozygous mutant plants with the maize inbred line A632. The segregation patterns in the F₂ populations indicate that the mutant phenotypes were caused by recessive mutations at a single locus (Table S2). With 81 polymorphic SNP markers across the maize genome and 45 F₂-dil338 and 53 F₂-dil474 mutant plants, both mutants were mapped to the same interval on chromosome 6, between PHM788 (278 cM of IBM2 Neighbors map) and PHM1147 (394 cM of IBM2 Neighbors map).

IDP and CAPS markers polymorphic between PHM788 and PHM1147 were used on 259 individuals from F₂-dil474 and 275 individuals from F₂-dil338 to further define the DIL1 locus. Both dil338 and dil474 mutants were mapped in the same interval between IDP7703 (285.9 cM) and IDP608 (316.8 cM) (Figure 3A), implying that dil474 and dil338 are allelic. To test whether dil338 and dil474 are allelic, individual F₂-dil474 and F₂-dil338 plants that were heterozygous at the DIL1 locus (as determined by two flanking markers) were reciprocally crossed and five F₁ ears were generated. Mutant phenotypes were observed in F₂ progenies from all five ears and the ratio between wild type and mutant plants was approximately 3∶1 (data not shown). It was therefore concluded that dil474 and dil338 are two alleles of the same gene and that mutations in this gene are responsible for the observed mutant phenotypes.

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Figure 3. Fine mapping and cloning of dil1.

A. DIL1 was mapped on the long arm of chromosome 6, between Brugi030 and IDP8945. B. B73 BAC contig covering the DIL1 locus. C. Recombination events near DIL1 delimited DIL1 between c0137A18-A2 and c0427D16-D1. A: wild type (A632) genotype. B: mutant (PHN4611) genotype. H: heterozygous genotype.

https://doi.org/10.1371/journal.pone.0037040.g003

To further fine map and clone DIL1, 2484 F₂ plants from dil338 were screened with flanking markers PHM788 and PHM1147 (Figure 3A), and 1240 recombinants were identified. DIL1 was further delimited to the interval between Brugi030 and IDP8945, spanning nine overlapping sequenced BACs (Figure 3B). Additional markers were developed from the BAC sequences (Table S1), and DIL1 was finally mapped between c0137A18-A2 and c0427D16-D1, spanning 214 kb (Figure 3C).

Identification and Validation of Candidate Gene for dil1

The closest flanking markers that define the DIL1 interval consist of two overlapping B73 BAC clones: c0137A18 and c0427D16. Only one low copy annotated gene with corresponding EST, an AP2 transcription factor-like gene, was identified within this interval (GeneBank EU966890.1). Three markers (c0427D16-A1, PCO589962-3 and PCO589962-4) developed from the AP2-like gene co-segregated with the phenotypes (Figure 3C). 5′ and 3′ RACE as well as RT-PCR were performed to generate the full length cDNA for the AP2-like gene and to determine its structure. The gene consists of nine exons and eight introns (Figure 4A, Figure S1), encoding a putative polypeptide of 412 amino acids. Sequence comparison of the AP2-like gene between PHN4611 and dil338 mutant revealed a point mutation (G to A) in the 4^th intron, near an exon-intron junction (Figure 4A). Interestingly, a point mutation (G to A) in the 2^nd intron, near another exon-intron junction, was detected in dil474 (Figure 4A). Identification of mutations within the same candidate gene in two independent mutant alleles confirms that DIL1 encodes the AP2 transcription factor-like gene.

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Figure 4. Single base pair mutations in dil1 mutants cause alternative splicing.

A. Structure of DIL1 gene and positions of single base pair mutations in dil338 and dil474 (in red and labeled with asterisk). B. Proportion of transcript variants in wild type and dil1 mutants.

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Since both mutations occur near exon-intron junctions, RT-PCR with primers amplifying the full-length coding sequence was performed to determine the presence of splicing variants in dil1 mutants. The cDNA products were cloned and sequenced. Sequences from 125 cDNA clones from dil338 and 95 cDNA clones from dil474 showed that mis-spliced variants represent the predominant form in both mutants (98.4% and 90.8% in dil338 and dil474, respectively) (Figure 4B). The predominant splicing variant in dil474 (deletion of exon 3) results in a 3-amino acid deletion, while the major splicing variant in dil338 (deletion of both exons 3 and 4) causes amino acid deletions and introduces a premature stop codon. Since both exons 3 and 4 are within the AP2 domain, deletions of exons 3 and/or 4 would presumably affect the function of the AP2 protein. It is interesting to notice that a small percentage (∼8%) of the AP2 transcripts in wild type plants also misses one or two of the exons, whereas a small percentage (∼2–6%) of the transcript is full length in dil1 mutant plants. This indicates that the control of alternative splicing for this AP2 gene is not tight. Moreover, the mutations may not cause the complete loss of function for the AP2 gene, as a small number of functional transcripts are present in mutant plants.

Expression of DIL1

Besides the allelic variations at the amino acid level, the mutations may also affect transcript levels. Since the major splicing variant in dil338 contains a premature termination stop codon (PTC), it is likely to be targeted by the nonsense mediated mRNA decay (NMD) surveillance pathway. NMD is a quality-control mechanism that selectively degrades mRNAs harboring PTCs [14]. The expression levels of DIL1 in leaves between wild type and mutant plants were compared with semi-quantitative RT-PCR. The expression level of DIL1 gene in dil474 is similar to that of wild type plants, whereas the expression level in dil338 is significantly lower (Figure 5A). In comparison with dil474 transcript (with a nine nucleotide deletion), the larger deletion and in particularly the premature stop codon in dil338 transcripts may reduce the transcript stability by NMD, which results in the reduced steady-state level of the transcript.

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Figure 5. Expression analysis of DIL1 gene.

A. DIL1 mRNA levels in V3 leaves in wild type and mutant plants, as determined by RT-PCR with 30 cycles for DIL1 (Upper), with the actin gene as the control (Lower). B-D. RNA in situ hybridization on tissue sections from A619 wild type vegetative apices, showing expression of DIL1 in the leaf primordia and the P₀ region of the meristem (B and C). Hybridization signal was not observed with control, sense probes (D).

https://doi.org/10.1371/journal.pone.0037040.g005

A search of the DuPont/Pioneer MPSS database, which consists of libraries of 17-bp sequence tags from 2×10⁵ to 2×10⁶ cDNAs isolated from over 240 diverse maize tissues and developmental stages [15], with DIL1 indicates this gene is constitutively expressed in multiple tissues and developmental stages at a low level (data not shown). To further elucidate the expression patterns of DIL1, in situ hybridization was performed on tissue sections from A619 wild type vegetative apices (Figure 5B-D). Several independent hybridizations reveal that DIL1 transcripts accumulate in the leaf primordia and also the P₀ region of the meristem, suggesting that DIL1 might control leaf shape from the early leaf initiation stage. Interestingly, the expression of DIL1 was not observed in all cells, but was in a subset of cells in a speckled pattern, suggesting that it might cell cycle regulated (arrowed, Fig. 5C). Hybridization signal was not observed with control, sense probes (Fig. 5D).

Mutations in an AP2 Transcription Factor-like Gene Affect Stalk and Leaf Development in Maize

A candidate gene for dil1 was identified via positional cloning. It encodes an AP2 transcription factor-like gene. The presence of mutations within the same gene in two independently isolated mutant alleles confirmed the identification of the causal gene. AP2 genes belong to a large gene family of plant transcription factors, which contain the highly conserved AP2/ERF DNA binding domain and play important roles in developmental regulation as well as in response to abiotic and biotic stresses [16], [17]. Based on the number of AP2/ERF domains and the gene structure, the AP2/EREBP gene family has been divided into four subfamilies: AP2, RAV (related to ABI3/VP1), dehydration-responsive element-binding protein (DREB) and ERF [17], [18], [19]. A comprehensive phylogenetic analysis of 167 AP2-like genes in maize has been conducted recently ([17]), and DIL1 belongs to the AP2 subfamily (identical to ZmAP2-5 or Unigene ZM.83210 in [17]). While many genes of the RAV, DREB, and ERF subfamilies are involved in plant response to stresses, members of the AP2 subfamily have been implicated in developmental regulation. Genes from the AP2 subfamilies in Arabidopsis include AINTEGUMENTA (ANT), PLETHORA1 (PLT1) and WRINKLED1 (WRI1), all of which are involved in developmental regulation [20], [21], [22]. Wri1 mutants have wrinkled seeds due to altered fatty acid metabolism, but do not affect plant height or leaf development. The WRI1 protein binds to the AW-box sequence conserved among proximal upstream regions of genes involved in fatty acid biosynthesis [23]. AP2 transcription factors controlling meristem fates and inflorescence architecture in maize have been identified. Spikelet meristem (SM) identity is controlled by BD1 (branched silkless1), a putative AP2 transcription factor in the ERF subfamily, in maize [24]. bd1 mutants initiate extra spikelets in the tassel, and in the ear, SMs are replaced with branch meristems. Two related AP2 transcription factors in the AP2 subfamily, indeterminate spikelet1 (ids1) and sister of ids1 (sid1), regulate the SM determinacy [25]. Double mutants of ids1 and sid1 do not make floral meristems (FMs). Instead, they initiate many bract-like organs. Expression patterns of meristem markers suggest that the SM never transitions to FM fate in the double mutants. It is of interest that a MIR172 family member (TS4) can negatively regulate both IDS1 and SID1 [25], [26]. Up-regulation of IDS1 results in extra florets, and sexual identity in maize is acquired by limiting floral growth through negative regulation of the floral homeotic pathway [26]. This observation indicates that the sex determination and SM determinacy pathways intersect, and AP2 transcription factors are involved in the regulation. Although the expression of certain AP2-like genes is regulated by microRNA, we failed to identify any putative microRNA binding sites in DIL1 (data not shown).

Although virtually all the genes cloned thus far from maize dwarf mutants are hormone-related, over-expression of several AP2 transcription factors produces dwarf phenotypes in Arabidopsis [27], [28], [29]. Also, several genes affecting cell shape have been isolated in maize and Arabidopsis, all of them are involved in cytoskeleton organization [30], [31], [32]. These observations indicate that DIL1 provides a new insight into regulation of plant architecture and cell specification. The phenotypic similarity between dil1 mutants and mutants in the cytoskeleton may suggest that the genes identified in the cytoskeleton mutants are putative targets for DIL1.

The molecular mechanism of DIL1 regulation in stalk and leaf development is unknown. It could affect the expression of genes related to hormonal pathways (plant height) or cytoskeleton organization (leaf development). Thousands of differentially expressed genes in leaves and stalks between dil1 mutant and wild type plants were identified in a microarray experiment (data not shown). Although many of the differentially expressed genes are involved in hormone metabolism or are hormone-responsive, it is virtually impossible to identify the genes that are directly regulated by DIL1 using this approach. A CHIP-seq (chromatin immunoprecipitation sequencing, [33]) experiment would be an appropriate approach to identify directly regulated genes, and may shed light on the molecular mechanism of DIL1 regulation in plant development. Alternatively, genetic screening to identify suppressors or modifiers (mutagenized or native alleles) for dil1 would be a powerful way to identify genes that interact directly or indirectly with DIL1 [34], [35].

Both dil1 Alleles Result in Alternative Splicing Variants of the DIL1 Gene

Mutations in both dil1 alleles occur in introns, near the exon-intron junctions. Since changes in introns would not directly affect amino acid sequences, one obvious possibility is their effect on intron splicing. Indeed, the mutations cause skipping of one or two exons, which results in the deletion of amino acids and introduction of premature stop codon. It is interesting to note that the aberrant splicing variants are present in wild-type plants and the full-length mRNA present in mutant plants, although at low frequencies. Mutations in introns cause a major shift in the ratio of full-length mRNA to the exon-skipping variants. Because the two exons skipped are located in the AP2 domain, the predominant splicing variants in dil1 mutants presumably would not function properly. In addition, the dominant splicing variant in dil338 contains a premature termination stop codon (PTC), which could be targeted by the nonsense mediated mRNA decay (NMD) surveillance pathway [36], [37]. Indeed, the expression level of DIL1 is significantly lower in dil338 than that in dil474 or wild type plants.

Alternative splicing (AS) of pre-mRNA was first described more than 30 years ago [38]. Although it was once considered unusual, recent studies with high throughput sequencing indicate that most intron-containing human pre-mRNAs are processed to yield multiple mRNAs [39]. Alternative splicing is considered one of the main sources of proteomic diversity in multicellular eukaryotes [39]. In Arabidopsis and rice, a significant proportion of intron-containing genes are also alternatively spliced [36], [37]. Alternative splicing could be regulated developmentally and by environmental stimuli, resulting in functional consequences [40]. While exon skipping is the most prevalent form of alternative splicing in human [41], intron retention seems to be more common in plants [36], [37]. Alternative splicing is primarily regulated by RNA-binding proteins, which bind pre-mRNA near splicing sites and modulate the efficiency of their recognition by the basal splicing machinery or splicesome [40]. It would be of interest to investigate in detail how the specific point mutations in dil1 mutants affect the splicing patterns.

The AS variants of DIL1 are from induced mutagenesis. Since AS is a ubiquitous phenomenon, it is possible that natural variations in AS are present in members of AP2 transcription factors. Indeed, the presence of AS variants of certain AP2-like genes have been reported in barley[42], wheat [43], maize [44] and kiwifruit [45]. The AS patterns in the homologous barley and wheat AP2 gene are conserved and differentially regulated by various abiotic stresses, implying a regulatory role at the level of AS in response to abiotic stresses. ZmDREB2A, a DREB2 homolog in maize, produces two forms of transcripts and only one of them is functional [44]. Under normal conditions the “defect” isoform is present but the functional isoform is undetectable. However, the functional variant is much more responsive to stress treatments. The data indicate that AS plays an important role in regulating ZmDREB2A activity under stress conditions. Thus, AS variants are not only present in AP2 genes, but AS regulation may have important implications for stress responses. It is possible that AS regulation on the AP2 transcription factors is ubiquitous. With the advance of Next Gene Sequence technologies, it becomes increasingly feasible to identify and characterize AS variants for all the AP2 genes.

Regulation of Plant Stature and its Application

The genetic control of plant architecture is very complex [2]. Reduced plant height and leaf angles are desirable traits in maize breeding [1]. Such plants provide better tolerance to lodging and are more adaptable to high planting density. Mutations in DIL1 reduce internode length and leaf angle, but also cause undesirable pleiotropic effect (e.g. wrinkled leaves). Tightly controlled transgenic expression of DIL1 with tissue-specific promoters may be a way to generate the desirable phenotypes without the negative pleiotropic effect (e.g. [46]). An alternative approach would involve searching for naturally occurring alleles of DIL1 with preferred phenotypes. A third approach is to identify genes which act downstream of DIL1 through genetic screening [34], [35]. Such genes may give more specific phenotypes that can be used for crop plant improvement.

EMS Mutagenesis for Dwarf Mutant Screening

An ethyl methanesulfonate (EMS) mutagenized population was generated in PHN4611, an elite, Non-Stiff Stalk (NSS) inbred lines from Pioneer Hi-bred International, Inc. Fresh PHN4611 pollen was suspended in a 0.06% solution of EMS in paraffin oil (Fisher 0121-1) for 45 min with shaking at 5 min intervals. A ratio of ten parts EMS solution to one part pollen was used. The EMS treated pollen was then applied to silks of the PHN4611 with a camel hair brush. The M1 individuals were self-pollinated to generate the F₂s families, which were screened for alterations in plant and organ growth. Approximately 500 M2 families of the EMS mutagenized maize populations were grown in the greenhouse in 18-plant flats and screened. The number of plants per family grown varied and depended upon the seed availability. Seedling plant architecture characteristics such as, but not limited to, leaf initiation rate, leaf morphology, seedling size, leaf angle, leaf length, leaf width of mutant plants and wild type plants were observed at different stages during the germination and seedling growth.

Phenotypic changes were identified and monitored. At approximately the three leaf stage, mutant phenotypes became obvious and distinct from the wild type. Mutants that fit approximately the segregation ratio of 3∶1 were identified as recessive mutations and advanced for further characterization.

Cytological Analysis of Mutant Leaf Epidermal Cells and Stalk Parenchyma Cells

Leaf samples were collected by cutting a 2 cm wide strip from the mid-point of the 2^nd leaf of V3 seedlings (3–4 week old plants, when the collar of the 3^rd leaf is visible) and from the first leaf below the ear of mature plants. Samples were fixed in a solution of 25% acetic acid and 75% ethanol. Samples were further processed by taking 6 mm leaf punches from corresponding regions of fixed tissue and post-fixed in 2% glutaraldehyde to enhance host cell autofluorescence. These post-fixed leaf disks were rinsed, cleared in chloral hydrate, mounted in Hoyer’s medium, and examined with the 720 nm laser line of a Zeiss multiphoton laser scanning microscope (LSM), using a 20x Plan Apochromat (0.75 NA) objective lens. Multiple optical sections (0.8 µm section thickness) were collected and maximum intensity projections assembled as single images for evaluation.

Maize stalk samples were collected by cutting 2 cm wide cross-sections of stalk from the center of internode #3 (base) and #9 (apex) and were fixed in acetic acid-ethanol. Cross-sections were post-fixed in glutaraldehyde to enhance cell wall autofluorescence, cleared in chloral hydrate, mounted and examined with multiphoton LSM.

dil1 mutants and wild type sibs were grown for ∼5 weeks in the growth chamber, and leaf tissue from the base of the blade was dissected from leaves that were emerging from the whorl or from leaves that were almost fully expanded. Leaf pieces were mounted on aluminum stubs using silver paint (Electron Microscopy Sciences, Hatfield, PA, USA), then imaged in a Hitachi S3500N scanning electron microscope under high vacuum mode, and 5keV accelerating voltage, as described in Jackson (2002)[47].

Fine-mapping and Cloning of DIL1

Two large F₂ populations (F₂-dil338 and F₂-dil474) were generated from homozygous dil mutant plants and A632. For initial chromosomal localization of the mutants, 45 F₂-dil338 and 53 F₂-dil474 mutant plants were genotyped with 81 SNPs distributed across the maize genome. Additional IDP and SNP markers around the DIL1 locus were developed with publicly available IDP and BAC sequences. In the end, the DIL1 interval was delimited into a two overlapping BAC interval and a single candidate gene was identified.

RT-PCR and RACE

Total RNA was extracted from the leaves of wild type and homozygous mutant plants using a Qiagen RNeasy kit (Qiagen Inc., Valencia, CA, USA) and cDNA obtained with oligo DT and Superscript® reverse transcriptase (Invitrogen, Carsbad, CA, USA). PCR was performed using GoGreen mixture (Promega, Madison, WI, USA). Primers for DIL1 are 5′-CTCGTCCTCGTCGCTCAG-3′ and 5′-AACCGTTGTTGTTGTTATTGTCG-3′, and primers for Actin are 5′-CACTGTGCCAATCTACGAGGGT-3′ and 5′-CACAAACGAGGGCTGGAACAAG-3′. RT-PCR products were fractionated in a 1.5% agarose gel and visualized by ethidium bromide staining.

5′ and 3′ RACE were carried out with the GeneRacer™ kit (Invitrogen). Total RNA was extracted from maize tissue using Trizol reagent (Invitrogen) and treated with RNase-free DNase I (Promega). Additional steps include dephosphorylation and decamping of mRNA, ligating the GeneRacerTM RNA oligo to full-length mRNA, reverse transcription with RT and GeneRacerTM oligo dT primers, performing PCR with the GeneRacerTM primer and gene specific primers, gel imaging, cloning and sequencing PCR products, and analyzing sequencing results. The primers used include 5′-GCTGTCAACGATACGCTACGTAACGGCATGACAGTG (T) -3′ for reverse transcription, 5′-CGACTGGAGCACGAGGACACTGA-3′ and 5′-CGACCTGTCCACCTATGCCGGGTGAC-3′ for 5′RACE first round amplification, 5′-GGACACTGACATGGACTGAAGGAGTA-3′ and 5′-AACGCCCTCCTGGGCACCAGCTC-3′ for 5′RACE nested PCR amplification, 5′-GCTGTCAACGATACGCTACGTAACC-3′ and 5′-TGGCTTCAGTTCTCCATCAAAGCCCTCT-3′ for 3′RACE first round amplification, 5′-CGCTACGTAACGGCATGACAGTG-3′ and 5′-GAGTACCTGGAGCCCTGCTGATCCTTCC-3′ for 3′RACE nested PCR amplification.

RNA in Situ Hybridization

Sample preparations and in situ hybridizations were performed as described previously [48], except that 8% polyvinyl alcohol (MW 70.000 – 100.000, SigmaP1763) was included in the staining buffer. The DIL1 probe contained the nucleotide sequences for about 600 bp coding region and 130 bp 5′UTR. The sequences were cloned into pCR-Blunt II-TOPO vector in sense and antisense orientation, relative to the T7 promoter. Linearized plasmids were used as templates for probe synthesis using T7 RNA polymerase. Probes were not hydrolyzed. After the color reaction, slides were mounted in 30% glycerol and photographed using DIC microscopy.