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Genetics, Vol. 166, 113-124, January 2004, Copyright © 2004

REN1 Is Required for Development of Microconidia and Macroconidia, but Not of Chlamydospores, in the Plant Pathogenic Fungus Fusarium oxysporum

Toshiaki Oharaa, Iori Inouea, Fumio Namikib, Hitoshi Kunohc, and Takashi Tsugea
a Graduate School of Bioagricultural Sciences, Nagoya University, Chikusa, Nagoya 464-8601, Japan,
b National Agricultural Research Center for Kyushu-Okinawa Region, Nishigoshi-Machi, Kikuchi-Gun 861-1192, Japan
c Faculty of Bioresources, Mie University, Tsu 514-0008, Japan

Corresponding author: Takashi Tsuge, Graduate School of Bioagricultural Sciences, Nagoya University, Furo-Cho, Chikusa, Nagoya 464-8601, Japan., ttsuge{at}agr.nagoya-u.ac.jp (E-mail)

Communicating editor: P. PUKKILA


*  ABSTRACT
*TOP
 *ABSTRACT
*MATERIALS AND METHODS
 *RESULTS
 *DISCUSSION
 *LITERATURE CITED

The filamentous fungus Fusarium oxysporum is a soil-borne facultative parasite that causes economically important losses in a wide variety of crops. F. oxysporum exhibits filamentous growth on agar media and undergoes asexual development producing three kinds of spores: microconidia, macroconidia, and chlamydospores. Ellipsoidal microconidia and falcate macroconidia are formed from phialides by basipetal division; globose chlamydospores with thick walls are formed acrogenously from hyphae or by the modification of hyphal cells. Here we describe rensa, a conidiation mutant of F. oxysporum, obtained by restriction-enzyme-mediated integration mutagenesis. Molecular analysis of rensa identified the affected gene, REN1, which encodes a protein with similarity to MedA of Aspergillus nidulans and Acr1 of Magnaporthe grisea. MedA and Acr1 are presumed transcription regulators involved in conidiogenesis in these fungi. The rensa mutant and REN1-targeted strains lack normal conidiophores and phialides and form rod-shaped, conidium-like cells directly from hyphae by acropetal division. These mutants, however, exhibit normal vegetative growth and chlamydospore formation. Nuclear localization of Ren1 was verified using strains expressing the Ren1-green fluorescent protein fusions. These data strongly suggest that REN1 encodes a transcription regulator required for the correct differentiation of conidiogenesis cells for development of microconidia and macroconidia in F. oxysporum.

ASEXUAL sporulation is a common reproductive mode for a diverse group of agriculturally, industrially, and medically important fungi. Asexual spores of higher fungi are called conidia (COLE 1986 Down). In many plant pathogenic fungi, conidia are the infectious propagules responsible for initiating infection as well as disease dissemination (DAHLBERG and VAN ETTEN 1982 Down). Knowledge of the molecular mechanisms controlling conidiation in plant pathogenic fungi will contribute to the search for a target for disease control through reducing primary inocula and spread of the disease. The genetic and molecular mechanisms controlling conidiation have been addressed in detail for two experimental fungi, Aspergillus nidulans (TIMBERLAKE 1990 Down; ADAMS et al. 1998 Down) and Neurospora crassa (SPRINGER 1993 Down). However, the conidiation mechanisms remain largely undefined in plant pathogenic fungi.

Fusarium oxysporum is an economically important soil-borne pathogen with worldwide distribution (ARMSTRONG and ARMSTRONG 1981 Down; BECKMAN 1987 Down). This fungus causes vascular wilts in ~80 botanical species (ARMSTRONG and ARMSTRONG 1981 Down; BECKMAN 1987 Down). Individual pathogenic strains within the species have a limited host range, and strains with similar or identical host ranges are assigned to intraspecific groups, called formae speciales (ARMSTRONG and ARMSTRONG 1981 Down; BECKMAN 1987 Down).

F. oxysporum is classified in the subdivision Deuteromycotina (fungi imperfecti), because it lacks sexual reproduction. Fusarium species that have sexual stages are classified in Pyrenomycetes of the subdivision Ascomycotina. F. oxysporum is unique in its asexual reproduction (NELSON et al. 1983 Down); it produces three kinds of asexual spores: microconidia, macroconidia, and chlamydospores (Fig 1). Microconidia are ellipsoidal and have no or one septum (Fig 1A). Macroconidia are falcate and have three or four septa (Fig 1B). Globose chlamydospores have thick walls (Fig 1C). Conidiogenesis of microconidia and macroconidia are phialidic (NELSON et al. 1983 Down). Microconidia are formed from phialides in false heads by basipetal division, the developmental mode from the apex toward the base without catenation of cells (Fig 1A). Macroconidia with pronounced foot cells are generally produced from phialides on conidiophores by basipetal division (Fig 1B). Chlamydospores are formed acrogenously from hyphae or by the modification of hyphal cells (Fig 1C). These asexual spores play important roles in the disease cycle of F. oxysporum: microconidia and macroconidia are important as secondary inocula, and chlamydospores are endurance organs in soils and act as inocula (ROWE et al. 1977 Down; COUTEAUDIER and ALABOUVETTE 1990 Down; KATAN et al. 1997 Down; REKAH et al. 2000 Down).



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  		Figure 1. Conidiation of the rensa mutant. (A–F) The wild-type strain Mel02010 and the rensa mutant B50-19 were grown on CLA at 25° for 5 days (A–D and F) or 10 days (E). Bars, 10 µm. mi, microconidium; p, phialide; ma, macroconidium; cp, conidiophore; cs, chlamydospore; rc, rod-shaped, conidium-like cell. (G–J) Mel02010 and B50-19 were grown in CMC at 25° for 4 days on an orbital shaker (at 100 rpm). The resulting cells were observed with a differential phase contrast microscope (G and I). The cells were stained with fluostain I and Hoechst 33258 to visualize cell walls and nuclei, respectively, and observed with a fluorescence microscope (H and J). Bars, 10 µm.

We previously described a mutant screen of F. oxysporum f. sp. melonis using restriction-enzyme-mediated integration (REMI) mutagenesis (KUSPA and LOOMIS 1992 Down; LU et al. 1994 Down; INOUE et al. 2001 Down). This pathogen causes vascular wilt of melon (LEACH and CURRENCE 1938 Down). Strain Mel02010 was transformed with the plasmid pSH75, conferring resistance to hygromycin B (KIMURA and TSUGE 1993 Down) by the REMI method. We tested 2929 transformants for pathogenicity to melon and selected 43 mutants that showed reduction or complete loss of virulence on susceptible melon cultivars (INOUE et al. 2001 Down). Molecular analysis of these mutants allowed us to identify two genes so far, ARG1 and FOW1, essential for virulence of this pathogen (NAMIKI et al. 2001 Down; INOUE et al. 2002 Down).

Here we describe the isolation and characterization of rensa, a conidiation mutant of F. oxysporum. To isolate genes required for conidiation in this fungus, previously isolated REMI transformants (INOUE et al. 2001 Down) were tested for conidiation, and the rensa mutant was selected. The affected gene, REN1, encodes a protein with similarity to MedA of A. nidulans (CLUTTERBUCK 1969 Down; MILLER et al. 1993 Down; GEMS and CLUTTERBUCK 1994 Down; BUSBY et al. 1996 Down) and Acr1 of Magnaporthe grisea (LAU and HAMER 1998 Down; NISHIMURA et al. 2000 Down). MedA and Acr1 have been identified as developmental regulators of conidiation in these fungi (CLUTTERBUCK 1969 Down; MILLER et al. 1993 Down; GEMS and CLUTTERBUCK 1994 Down; BUSBY et al. 1996 Down; LAU and HAMER 1998 Down; NISHIMURA et al. 2000 Down). A mutation at REN1 results in a defect in development of microconidia and macroconidia and causes the production of rod-shaped, conidium-like cells in chains by head-to-tail arrays (acropetal division). The mutants, however, exhibit normal vegetative growth and form chlamydospores. Thus, it appears that REN1 specifically controls the developmental pathway of microconidia and macroconidia in F. oxysporum.


*  MATERIALS AND METHODS
*TOP
 *ABSTRACT
 *MATERIALS AND METHODS
*RESULTS
 *DISCUSSION
 *LITERATURE CITED

Fungal strains, plasmids, and genomic libraries:
Strain Mel02010 (JCM9288) of F. oxysporum f. sp. melonis (NAMIKI et al. 1994 Down) was used for REMI transformation and identification of REN1. The rensa mutant (B50-19) was selected from the REMI transformants previously isolated (INOUE et al. 2001 Down).

The integrative transformation vector pSH75 (KIMURA and TSUGE 1993 Down) was used for transformation of F. oxysporum. This vector contains the hygromycin B phosphotransferase gene (hph), which is fused to the A. nidulans trpC promoter and terminator (GRITZ and DAVIES 1983 Down; MULLANEY et al. 1985 Down; KIMURA and TSUGE 1993 Down).

The ß-tubulin gene fragment was amplified from total DNA of Mel02010 by polymerase chain reaction (PCR) with primers C (5'-GAGGAATTCCCAGACCGTATGATG-3') and D (5'-GCTGGATCCTATTCTTTGGGTCGAACAT-3'; KOENRAADT et al. 1992 Down). These primers were reported as degenerate primers for PCR amplification of the fungal ß-tubulin genes (KOENRAADT et al. 1992 Down). PCR amplification from total DNA (100 ng) was performed with Taq DNA polymerase (Takara, Ohtsu, Japan) according to the manufacturer's instructions. The PCR product of ~0.4 kb was cloned in pGEM-T Easy vector (Promega, Madison, WI) to make pFOTUB1 and sequenced to confirm that it encodes part of ß-tubulin. The pFOTUB1 insert was used as a probe for RNA gel blot analysis.

A genomic cosmid library of Mel02010 was constructed with a cosmid vector pMLF2 (AN et al. 1996 Down) using half-site fill-in reactions (SAMBROOK et al. 1989 Down). Total DNA of Mel02010 was partially digested with Sau3AI to generate fragments of ~40 kb and partially filled with dATP and dGTP. The cosmid vector pMLF2 was completely digested with XhoI and partially filled with dCTP and dTTP. Partially filled Sau3AI genomic DNA fragments were cloned at the partially filled XhoI site of pMLF2 to construct a genomic library. Screening of the library by colony hybridization was conducted by the standard method (SAMBROOK et al. 1989 Down).

Fungal transformation:
Protoplast preparation and transformation of F. oxysporum were performed by the methods previously described (INOUE et al. 2001 Down). Transformants carrying the hph gene were selected on regeneration media containing hygromycin B (Wako Pure Chemicals, Osaka, Japan) at 60 µg/ml (INOUE et al. 2001 Down). Colonies that appeared 5–10 days after plating on the media were transferred to potato dextrose agar (PDA; Difco, Detroit) containing hygromycin B at 60 µg/ml, and transformants were selected after incubation at 25° for 5 days.

Test for conidiation:
To induce conidiation of F. oxysporum strains, two media were used: carnation leaf agar (CLA; 1.5% agar with sterilized carnation leaf pieces; FISHER et al. 1982 Down; TOGAWA 1992 Down) and carboxymethyl cellulose liquid medium (CMC; 15 g carboxymethyl cellulose, 1 g yeast extract, 1 g NH4NO3, 1 g KH2PO4, and 0.5 g/liter MgSO4·7H2O; CAPPELLINI and PETERSON 1965 Down).

Strains were grown on PDA at 25° for 5 days. Agar blocks (3 mm in diameter) carrying mycelia were prepared from the resulting colonies and inoculated on CLA, 5 mm apart from carnation leaf pieces. After incubation at 25° for 5–10 days, under continuous BLB (black light blue) light (FL15BLB; Toshiba, Osaka, Japan) (NIRENBERG 1990 Down), conidiation was observed with a light microscope (BX50, Olympus, Tokyo). The number of chlamydospores formed in a 5-mm square between agar blocks and leaf pieces was counted with a microscope.

For cryo-scanning electron microscopic observation, strains were grown on CLA at 25° for 5 days, and agar blocks (~2 x 2 mm) containing fungal propagules were cut out from the media. They were attached onto specimen stubs, frozen in liquid nitrogen, and observed with a scanning electron microscope (S-4000, Hitachi, Ibaraki, Japan) after gold coating.

A PDA block (3 mm in diameter) carrying mycelia was inoculated in 50 ml of CMC in a 100-ml Erlenmeyer flask and incubated at 25° for 4 days on an orbital shaker (100 rpm) under continuous fluorescent light (CAPPELLINI and PETERSON 1965 Down). The number of conidia was counted with a microscope. The resulting culture was passed through four layers of cheesecloth, and the filtrate was centrifuged at 1600 x g for 10 min to collect conidial cells. Cells were fixed in 0.4% p-formaldehyde in PME (50 mM PIPES, pH 6.7, 1 mM MgSO4, 20 mM EGTA) for 45 min at room temperature (BORNEMAN et al. 2000 Down), washed three times, and mounted in PME containing fluostain I (25 µg/ml; Dojin, Kumamoto, Japan) and Hoechst 33258 (250 µg/ml; Wako Pure Chemicals) to visualize cell walls and nuclei, respectively. Stained cells were observed with a fluorescence microscope (BX50) using a U-MWU filter (Olympus).

For the time course study of conidial development, a PDA block (3 mm in diameter) carrying mycelia was inoculated in 25 ml of complete medium (CM; 10 g KNO3, 5 g KH2PO4, 2.5 g MgSO4·7H2O, 0.02 g FeCl3, 10 g glucose, 1 g yeast extract, and 1 g/liter peptone; SANDERSON and SRB 1965 Down) in a 50-ml Erlenmeyer flask and incubated at 25° for 18 hr on an orbital shaker (100 rpm). The resulting mycelia were collected by centrifugation at 1600 x g for 10 min, inoculated in 50 ml of CMC in a 100-ml Erlenmeyer flask, and incubated at 25° for 132 hr on an orbital shaker (100 rpm) under continuous fluorescent light. During incubation, the number of conidia was counted with a microscope at 12-hr intervals. At 0, 12, 24, 36, 48, 60, 72, 96, and 120 hr after inoculation in CMC, fungal tissues were collected from five flasks by centrifugation at 1600 x g for 10 min and subjected to RNA isolation as described below.

Test for vegetative growth and pathogenicity:
To test for vegetative growth of F. oxysporum strains, strains were grown on three agar media: PDA, complete medium agar (CMA; CM supplemented with 20 g/liter agar; SANDERSON and SRB 1965 Down), and minimal medium agar (MMA; CMA without yeast extract and peptone; SANDERSON and SRB 1965 Down). Strains were grown on PDA at 25° for 5 days. PDA blocks (3 mm in diameter) carrying mycelia were inoculated on PDA, MMA, and CMA. After incubation at 25° for 5 days, colony growth and morphology were observed.

Pathogenicity was tested by a root-dip method using the susceptible melon (Cucumis melo L.) cultivar Amus as previously described (INOUE et al. 2001 Down). Strains were grown in CMC at 25° for 5 days on an orbital shaker (100 rpm) under continuous fluorescent light, and conidial cells were collected as described above. The cell pellet was suspended in sterilized water at ~1 x 107 conidia/ml, and plant roots were dipped in the suspension for 15 sec. Plants were grown in pots filled with sterilized soil. Ten seedlings, which had a single true leaf, were used for inoculation of each strain, and disease symptoms were assessed 3 weeks after inoculation.

Nucleic acid isolation and manipulations:
Isolation of total DNA from F. oxysporum and DNA gel blot hybridization were performed as previously described (NAMIKI et al. 1994 Down). To isolate total RNA from F. oxysporum, strains were grown in 50 ml of CMC, minimal medium (MM; MMA without agar; SANDERSON and SRB 1965 Down), and CM (SANDERSON and SRB 1965 Down) in 100-ml Erlenmeyer flasks at 25° on an orbital shaker (100 rpm). Fungal tissues were collected by centrifugation at 1600 x g for 10 min and ground in liquid nitrogen in a mortar with a pestle. Total RNA was extracted from the powdered mycelia as previously described (OKUDA et al. 1998 Down). Poly(A)+ RNA was isolated from total RNA with the PolyATtract mRNA isolation systems (Promega) according to the manufacturer's instructions. RNA gel blot hybridization was performed as previously described (OKUDA et al. 1998 Down).

For analysis of nucleotide sequences, DNA was cloned in pBluescript KS+ (Stratagene, La Jolla, CA) or pGEM-T Easy vector. DNA sequences were determined with the BigDye terminator cycle sequencing ready reaction kit (Applied Biosystems, Warrington, UK) and an automated fluorescent DNA sequencer (Model 373A, Applied Biosystems) according to the manufacturer's instructions. DNA sequences were analyzed with BLAST (ALTSCHUL et al. 1997 Down). Alignment of nucleotide and amino acid sequences was made with the CLUSTAL W program (THOMPSON et al. 1994 Down).

Isolation of REN1:
Restriction mapping of the pSH75 insertion site in the rensa mutant B50-19 revealed the presence of a 7.8-kb HindIII fragment that contains pSH75 and the flanking genomic DNA (Fig 2). Total DNA of B50-19 was digested with HindIII, religated, and transformed to Escherichia coli DH5{alpha}. Ampicillin-resistant transformants were selected, and the rescued plasmid, pRB5019H, was isolated (Fig 2). A 0.4-kb BamHI fragment from pRB5019H was cloned into the BamHI site of pBluescript KS+ to make pBB50-19 (Fig 2). The pBB50-19 insert was used as a probe for screening a genomic library of Mel02010, and a positive clone pcB5019-1 was isolated (Fig 2). A 5.5-kb region containing REN1 was sequenced as described above. The 1.2-kb EcoRV-PvuII fragment internal to REN1 was cloned into the EcoRV site of pBluescript KS+ to make pR1EP (Fig 2) and used as a probe for RNA gel blot analysis.



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  		Figure 2. The tagged locus in the rensa mutant B50-19. The 7.8-kb HindIII fragment was recovered from total DNA of B50-19 by plasmid rescue as pRB5019H. Restriction sites of the tagged locus in B50-19 were deduced by restriction mapping of pRB5019H and DNA gel blot analysis of B50-19 with the pSH75 probe. The pBB50-19 insert was used as a probe for screening a genomic cosmid library of the wild-type strain Mel02010, and the clone pcB5019-1 was isolated. The arrowed bar indicates ORF1 (REN1) with introns (open segments). The sequence analysis of pRB5019H and pcB5019-1 showed that the insertion of the transformation vector pSH75 in B50-19 had occurred at the BamHI site in the first intron accompanied by deletion of the upstream region (>5.0 kb). The pR1EP insert was used as a probe for RNA gel blot analysis. Arrowheads above ORF1 denote orientation and location of oligonucleotide primers (Rf1 and Rr1) used in RT-PCR experiments. B, BamHI; E, EcoRV; H, HindIII; P, PvuII; Ps, PstI.

The REN1 cDNA was isolated by reverse transcription-PCR (RT-PCR) using the RNA PCR kit Ver. 2.1 (Takara). The cDNA was amplified from total RNA (1 µg) of Mel02010 with primers Rf1 (5'-ATGTCTACTGTCAAGTTCCAGT-3') and Rr1 (5'-TCATGCTCTTGGTGCAGGTTCTGC-3') according to the manufacturer's instructions (Fig 2). Rf1 and Rr1 contain the REN1 initiation and termination codons (italics), respectively (Fig 2). RT-PCR products were cloned in pGEM-T Easy vector to determine the sequences.

Construction of the REN1-EGFP fusion vectors:
The green fluorescent protein (GFP)-expression vectors pYTGFP-N and pYTGFP-C were used to make the REN1-EGFP fusion vectors. These vectors contain the GFP (EGFP) open reading frame (ORF), which is fused to the A. nidulans trpC promoter and terminator (MULLANEY et al. 1985 Down; INOUE et al. 2002 Down). In pYTGFP-N, the last codon of the GFP ORF is fused to 15 nucleotides encoding a glycine linker followed by BamHI, SmaI, PstI, and EcoRI sites (KIMURA et al. 2001 Down; INOUE et al. 2002 Down). In pYTGFP-C, the trpC promoter is followed by XbaI, BamHI, SmaI, and PstI sites and 15 nucleotides encoding a glycine linker fused to the initiation codon of the GFP ORF (INOUE et al. 2002 Down). For a control, we used the plasmid pYTGFPc, which carries only GFP under the control of the trpC promoter and terminator (INOUE et al. 2002 Down).

The REN1 cDNA was amplified from poly(A)+ RNA of Mel02010 by RT-PCR with primers REN1N-f (5'-GAGTGATCATGTCTACTGTCAAGTTCCAGT-3') and REN1N-r (5'-TTTCTGCAGTCATGCTCTTGGTGCAGGTTC-3'). REN1N-f has a BclI site (underlined) with the initiation codon (italics); REN1N-r has a PstI site (underlined) with the termination codon (italics). The amplified DNA was digested with BclI and PstI and cloned into the BamHI-PstI site of pYTEGFP-N to make pGFP-REN1, resulting in a N-terminal fusion of GFP to Ren1.

The REN1 cDNA was amplified from poly(A)+ RNA of Mel02010 by RT-PCR with primers REN1C-f (5'-GAGTCTAGATGTCTACTGTCAAGTTCCAGT-3') and REN1C-r (5'-CTCCTGCAGTGCTCTTGGTGCAGGTTCTGC-3'). REN1C-f contains a XbaI site (underlined) with the initiation codon (italics); REN1C-r contains a PstI site (underlined) fused to the last codon of REN1. The amplified DNA was digested with XbaI and PstI and cloned into the XbaI-PstI site of pYTGFP-C to make pREN1-GFP, resulting in a C-terminal fusion of GFP to Ren1.

All the PCR products cloned in the vectors were sequenced to confirm the fact that no nucleotide substitution had occurred during amplification.

Observation of intracellular localization of the GFP-tagged Ren1:
Transformants of the wild-type strain with pYTGFPc, pREN1-GFP, and pGFP-REN1 were grown in CMC and CM at 25° for 4 days. The resulting mycelia were observed under a fluorescence microscope (BX50) using U-MWIG filter (Olympus) for GFP fluorescence.


*  RESULTS
*TOP
 *ABSTRACT
 *MATERIALS AND METHODS
 *RESULTS
*DISCUSSION
 *LITERATURE CITED

The rensa mutant:
REMI transformants previously isolated from the wild-type strain Mel02010 (INOUE et al. 2001 Down) were grown on the conidiation medium CLA. F. oxysporum produces microconidia, macroconidia, and chlamydospores on this medium (FISHER et al. 1982 Down; TOGAWA 1992 Down). Of 1792 REMI transformants tested, we identified one strain, B50-19, with a defect in development of microconidia and macroconidia. Although Mel02010 formed microconidia and macroconidia from phialides by basipetal division (Fig 1A and Fig B), B50-19 lacked normal conidiophores and phialides and formed rod-shaped, conidium-like cells directly from hyphae by acropetal division (Fig 1D). The rod-shaped cells had no or one septum, and their cell width was slenderer than that of microconidia and macroconidia of the wild type (Fig 1D). By prolonged incubation, B50-19 frequently formed rod-shaped cells in branching chains (Fig 1E). We called this mutation rensa, which means "catenation" in Japanese. The rensa mutant produced chlamydospores acrogenously from hyphae or by the modification of hyphal cells, as did the wild type (Fig 1C and Fig F). The number of chlamydospores formed on the media between inocula and carnation leaf pieces was not significantly different between Mel02010 and B50-19: 3.70 ± 1.24 chlamydospores/mm2 and 3.11 ± 0.31 chlamydospores/mm2, respectively, in the average of three cultures.

Fusarium species are known to produce microconidia and macroconidia when they are grown in CMC on an orbital shaker (CAPPELLINI and PETERSON 1965 Down). The wild-type and rensa mutant strains were grown in CMC at 25° for 4 days. The wild type formed a number of microconidia and macroconidia (Fig 1G): 3.7 x 106 microconidia/ml and 1.8 x 106 macroconidia/ml in the averages of three cultures. The rensa mutant, however, formed a smaller number of rod-shaped, slender cells (Fig 1I): 0.4 x 106 cells/ml in the average of three cultures. The rod-shaped cells had no or one septum and were similar in size and morphology to conidium-like cells formed on CLA (Fig 1D and Fig I), suggesting that these cells are aberrant conidia.

Conidial cells were stained with fluostain I and Hoechst 33258 to visualize cell walls and nuclei, respectively. Microconidia and macroconidia from the wild type contain a single nucleus in each cell (Fig 1H). Rod-shaped cells from the mutant also contain a single nucleus in each cell (Fig 1J). This result suggests that the rensa mutation does not affect the coupling of cell and nuclear division during conidiation.

The tagged locus in the rensa mutant:
The rensa mutant B50-19 was generated by REMI transformation of Mel02010 with the plasmid pSH75 in the presence of BamHI. DNA gel blot analysis using the pSH75 probe demonstrated that this mutant had two copies of pSH75 as a tandem array (Fig 2). About half of one of the copies was deleted, and the BamHI site in the junction of deleted plasmid and chromosomal DNA had been lost (Fig 2). The analysis identified a 7.8-kb HindIII fragment, which included the complete pSH75 and the flanking genomic DNA from one side of the inserted plasmid (Fig 2). The 7.8-kb HindIII fragment was recovered by plasmid rescue as pRB5019H (Fig 2).

The 0.4-kb BamHI fragment (pBB50-19) from pRB5019H (Fig 2) was used as a probe to screen a cosmid genomic library of Mel02010. A positive clone, pcB5019-1, was isolated and partially restriction mapped (Fig 2). Restriction sites downstream of the tagged site in pRB5019H were identical to those of pcB5019-1 (Fig 2). However, restriction sites upstream of the tagged site were different (Fig 2), indicating that the plasmid integration had caused a deletion of genomic DNA in B50-19.

A putative open reading frame at the tagged locus:
Sequencing of the 5.5-kb region in pcB5019-1 found a putative ORF1 from the tagged site in B50-19 (Fig 2). ORF1 consists of three exons (45, 187, and 1940 bp) divided by two introns (184 and 139 bp) and potentially encodes a 724-amino-acid protein. The introns were initially deduced on the basis of consensus sequences for 5' and 3' splice signals typical of fungal genes (BRUCHEZ et al. 1993 Down). To confirm the introns, the cDNA was prepared from total RNA of Mel02010 by RT-PCR with primers Rf1 and Rr1 (Fig 2). The RT-PCR amplification produced a 2.2-kb fragment of DNA. Comparison of the genomic sequence with that of the RT-PCR product confirmed that the two introns are spliced. The sequence analysis of pRB5019H and pcB5019-1 showed that the insertion of the transformation vector pSH75 in B50-19 had occurred at the BamHI site in the first intron accompanied by deletion of the upstream region (Fig 2). Preliminary analysis found that >5.0 kb genomic DNA was deleted in B50-19.

The deduced amino acid sequence encoded by ORF1 reveals similarity to those of MedA of A. nidulans (GenBank accession no. AF080599), Acr1 of M. grisea (GenBank accession no. AB096705), and EAA33615 of N. crassa (GenBank accession no. AABX01000175): 28.6, 32.9, and 40.8% identical to MedA, Acr1, and EAA33615, respectively (Fig 3). MedA and Acr1 are presumed transcription regulators involved in the conidial development in these fungi (MILLER et al. 1993 Down; BUSBY et al. 1996 Down; LAU and HAMER 1998 Down; NISHIMURA et al. 2000 Down). Although EAA33615 was estimated as a hypothetical protein of N. crassa, its function has not been identified (GALAGAN et al. 2003 Down). The similarity was most evident in amino acids 395–554 in the F. oxysporum ORF1 (Fig 3). The BLAST searches with available genome sequence databases of filamentous fungi and yeasts found no other proteins containing this conserved region. These data suggest that this region is a highly conserved, unique motif in a novel class of presumed transcription regulators involved in conidial development of filamentous fungi. LAU and HAMER 1998 Down identified a glutamine-rich region in Acr1 (amino acids 281–330 in Fig 3), which shares similarity to several transcription factors including GBF of Dictyostelium discoideum (SCHNITZLER et al. 1994 Down) and SIN3 of Saccharomyces cerevisiae (WANG et al. 1990 Down). However, the ORF1 product, MedA, and EAA33615 lack such regions (Fig 3). The ORF1 product also shows weak similarity to proline- and hydroxyproline-rich proteins from higher plants, which constitute cell wall architecture (STIEFEL et al. 1988 Down; CAELLES et al. 1992 Down).



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  		Figure 3. Similarity of the ORF1-encoded protein to other proteins. Amino acid sequence encoded by ORF1 was aligned with those of MedA of A. nidulans (GenBank accession no. AF080599), Acr1 of M. grisea (GenBank accession no. AB096705), and EAA33615 (EAA) of N. crassa (GenBank accession no. AABX01000175). Amino acids that are conserved between the ORF1 product and any of the others are indicated as white letters on a black background. The most conserved region among four sequences is indicated by a line above the sequences (amino acids 395–554 of ORF1). The glutamine-rich region in Acr1 is underlined (amino acids 281–330 of Acr1).

REN1 is essential for conidiation:
We identified ORF1, which encodes a protein homologous to MedA and Acr1, in the tagged site in the rensa mutant. However, it appeared that the plasmid integration had been accompanied with deletion of chromosomal DNA in the mutant. To assess whether mutation of ORF1 is responsible for the rensa phenotype, homologous recombination was employed to replace ORF1 with the plasmid pGDR1, which contains the hph gene flanked by the 5' and 3' sequences from ORF1 (Fig 4A). The 0.5-kb BamHI-EcoRV fragment and the 1.2-kb ClaI-HindIII fragment containing the 5' and 3' regions of ORF1, respectively, were cloned into the transformation vector pSH75 to make the ORF1-targeting vector pGDR1 (Fig 4A).



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  		Figure 4. Transformation-mediated targeting of ORF1. (A) Structure of ORF1 before and after homologous integration of the ORF1-targeting vector pGDR1. The targeting vector pGDR1 contains hph flanked by the 5' sequence of 0.5 kb and the 3' sequence of 1.2 kb from ORF1 in pSH75. B, BamHI; C, ClaI; E, EcoRV; H, HindIII. (B) DNA gel blot analysis of pGDR1 transformants. Total DNA (2 µg/lane) from the wild-type strain and transformants was digested with BamHI and fractionated in a 0.8% agarose gel. The blot was probed with the 1.2-kb ClaI-HindIII fragment from pGDR1. Sizes (in kilobases) of marker DNA fragments (HindIII-digested {lambda}DNA) are indicated on the left. W, wild-type strain Mel02010; WT1–WT4, transformants showing normal conidiation; DR1–DR4, transformants showing rensa phenotype. (C) Scanning electron micrograph of conidium-like cells of the REMI mutant B50-19 and the REN1-targeted mutant DR1. Strains were grown on CLA at 25° for 5 days and observed with a scanning electron microscope. Bars, 10 µm.

The wild-type strain Mel02010 was transformed with pGDR1, and 42 transformants were isolated. Each transformant was tested for conidiation on CLA. All the transformants normally formed chlamydospores. Of 42 transformants, 28 produced microconidia and macroconidia, as did the wild type. However, the remaining 14 transformants exhibited the rensa phenotype: they produced rod-shaped, slender cells by acropetal division.

The integration mode of pGDR1 in four transformants (DR1–DR4) showing the rensa phenotype was analyzed by DNA gel blot analysis. As controls, four transformants (WT1–WT4) showing normal conidiation were also used. Total DNA of Mel02010 and transformants was digested with BamHI, and the blot was probed with the 1.2-kb ClaI-HindIII fragment integrated in pGDR1 (Fig 4A). The restriction map of pcB5019-1 predicts that the probe would hybridize to a 5.8-kb BamHI fragment in the wild type (Fig 4A); however, four bands of ~2.5, 5.8, 7.0, and 23.0 kb hybridized (Fig 4B). The 5.8-kb signal was intense, and the others were weak. Thus, the wild type has the ORF1 homologs. All WT transformants contained these four bands and additional bands, resulting from ectopic integration of pGDR1 (Fig 4B). All DR transformants, however, lacked 5.8-kb bands but had 8.8-kb bands, as expected when the targeting vector pGDR1 was integrated into chromosomal DNA by homologous recombination (Fig 4A and Fig B). DR transformants preserved 2.5-, 7.0-, and 23.0-kb bands (Fig 4B). These results clearly showed that the rensa phenotype of DR transformants resulted from disruption of ORF1. Thus, the gene encoding ORF1 was designated REN1.

We observed conidiogenesis of the REMI mutant B50-19 and the REN1-targeted mutant DR1 with a cryo-scanning electron microscope (Fig 4C). These mutants lacked normal conidiophores and phialides and formed rod-shaped, catenated cells directly from hyphae (Fig 4C). Formation pattern and morphology of rod-shaped cells were similar in B50-19 and DR1 (Fig 4C). Although the first cells from hyphae looked like conidiophores, they were slenderer than conidiophores of the wild type.

Expression of REN1:
Expression of REN1 was determined by RNA gel blot analysis. Mel02010 was grown in CMC, CM, and MM liquid media at 25° for 4 days on an orbital shaker. Mel02010 formed microconidia and macroconidia in CMC, but not in CM and MM. Poly(A)+ RNA was prepared from the cultures. The RNA gel blot was probed with pR1EP containing the REN1 fragment (Fig 2). Unexpectedly, the probe hybridized to three bands of ~2.6, 3.4, and 4.8 kb in RNA from fungal tissues grown in CMC (Fig 5A). The 3.4-kb signal was intense, and the others were weak. This result indicates that the REN1 region is transcribed in a complex manner. These three bands were also detected in RNA from mycelia grown in CM and MM (Fig 5A). Thus, F. oxysporum expresses REN1 during both conidiation and vegetative growth.



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  		Figure 5. RNA gel blot analysis of REN1. The wild-type strain Mel02010 was grown in CMC, CM, and MM at 25° for 4 days (A). The wild-type strain (W), the REMI mutant B50-19 (lane 1), and the REN1-targeted mutant DR1 (lane 2) were grown in CMC at 25° for 4 days (B). Poly(A)+ RNA was prepared from the cultures. RNA (5 µg/lane) was electrophoresed in a 1.5% agarose gel containing 2.2 M formaldehyde. The blots were probed with pR1EP containing the REN1 fragment (Fig 2). Sizes (in kilobases) of marker RNA fragments (Novagen, Madison, WI) are indicated on the left. The blots were also probed with pFOTUB1 containing the ß-tubulin gene fragment (ß-TUB).

Expression of REN1 in the REN1-targeted mutants was determined by RNA gel blot analysis. Poly(A)+ RNA was prepared from fungal tissue of Mel02010, B50-19, and DR1 grown in CMC at 25° for 4 days. The RNA gel blot was probed with pR1EP (Fig 2). The probe hybridized to three bands of ~2.6, 3.4, and 4.8 kb in Mel02010, but to no bands in B50-19 and DR1 (Fig 5B). This result indicates that these three bands are all related to transcripts from the REN1 locus.

The timing of conidial development and REN1 expression was observed in CMC. Mel02010 and DR1 were grown in CM at 25° for 18 hr. The resulting mycelia were inoculated in CMC and incubated at 25° for 132 hr. In Mel02010, microconidia and macroconidia first appeared at 12 and 48 hr, respectively, after inoculation in CMC, and their numbers apparently increased to 120 hr (Fig 6A). Poly(A)+ RNA was prepared from fungal tissue, and the gel blot was probed with pR1EP (Fig 2). The probe weakly hybridized to only a 3.4-kb band in RNA of inoculated mycelia grown in CM for 18 hr (Fig 6B). After inoculation of the mycelia in CMC, two RNA bands of ~3.4 and 4.8 kb were detected at 12–60 hr, and three RNA bands of ~2.6, 3.4, and 4.8 kb were detected at 72–120 hr (Fig 6B). This result suggests that at least 3.4- and 4.8-kb transcripts from REN1 are essential for development of microconidia and macroconidia.



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  		Figure 6. Time course of conidial development of the wild-type strain Mel02010 and the REN1-targeted mutant DR1. (A) Mycelia of each strain grown in CM was inoculated in CMC and incubated at 25° for 132 hr. Numbers of microconidia (mi) and macroconidia (ma) of Mel02010 and of rod-shaped, conidium-like cells (rc) of DR1 were counted at 12-hr intervals with a microscope, and data represent means ±SD of five replications. (B) Fungal tissue of Mel02010 grown for indicated periods was collected, and poly(A)+ RNA was prepared from the tissue. RNA (5 µg/lane) was electrophoresed in a 1.5% agarose gel containing 2.2 M formaldehyde. The blots were probed with pR1EP containing the REN1 fragment (Fig 2). Sizes (in kilobases) of marker RNA fragments (Novagen) are indicated on the left. The blot was also probed with pFOTUB1 containing the ß-tubulin gene fragment (ß-TUB).

In DR1, conidium-like cells first occurred at 60 hr after inoculation in CMC, and the number gradually increased to 108 hr (Fig 6A). Thus, it appears that conidiation of the REN1 mutant is delayed.

Vegetative growth and pathogenicity of the REN1-targeted mutants:
Vegetative growth of the wild-type and REN1-targeted strains was evaluated by measuring colony diameters grown on PDA, CMA, and MMA at 25° for 5 days. Colony diameters of the REMI mutant B50-19 and the REN1-targeted mutants (DR1–DR3) were not significantly different from those of the wild type (Fig 7A). To the unaided eye there was no apparent difference in colony morphology between the wild-type and mutant strains (Fig 7B). These results indicate that REN1 is dispensable for vegetative growth.



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  		Figure 7. Vegetative growth and pathogenicity of REN1 mutants. (A and B) Colony diameter (A) and morphology (B) of REN1 mutants. The wild-type strain Mel02010, the REMI mutant B50-19, and the REN1-targeted mutants (DR1–DR3) were grown on PDA, CMA, and MMA at 25° for 5 days. Colony diameter was measured, and data represent means ±SD of three replications. (C) Pathogenicity of REN1 mutant. Mel02010 and DR1 were grown in CMC at 25° for 5 days, and the resulting conidial cells were collected. Seedlings of the cultivar Amus with a single true leaf were inoculated with cell suspension (~1 x 107 conidia/ml) of each strain by the root-dip method. Control plants were immersed in water. Photograph was taken 3 weeks after inoculation.

The REN1-targeted mutants were tested for pathogenicity to melon plants. The wild-type and mutant strains were grown in CMC, and the resulting conidial cells were used as inocula. Ten seedlings of susceptible cultivar Amus with a single true leaf were inoculated with cell suspension of each strain by the root-dip method (INOUE et al. 2001 Down), and disease symptoms were observed 3 weeks after inoculation. The wild-type and mutant strains caused typical wilt symptoms on all seedlings (Fig 7C). Thus, it appears that the rod-shaped cells of the REN1-targeted mutants preserve the abilities to infect host plant tissue and to cause disease symptoms under the conditions tested.

Intracellular localization of the GFP-tagged Ren1:
The predicted amino acid sequence of Ren1 is significantly similar to those of MedA of A. nidulans and Acr1 of M. grisea (Fig 3). Although medA and ACR1 have been suggested to encode transcription regulators (MILLER et al. 1993 Down; BUSBY et al. 1996 Down; LAU and HAMER 1998 Down; NISHIMURA et al. 2000 Down), their nuclear localization has not been verified. Ren1 also shows weak similarity to proline- and hydroxyproline-rich proteins, cell wall proteins of higher plants. To test intracellular localization of Ren1, we made strains expressing Ren1-GFP and GFP-Ren1 fusion proteins and observed intracellular distribution of the GFP fluorescence in the strains under fluorescence microscopy. We constructed the REN1-GFP and GFP-REN1 gene fusions under the control of the A. nidulans trpC promoter (MULLANEY et al. 1985 Down) as pREN1-GFP and pGFP-REN1, respectively. These constructs were introduced into Mel02010 by cotransformation with the plasmid pSH75 conferring hygromycin B resistance. For a control, Mel02010 was transformed with the plasmid pYTGFPc, which carries GFP under the control of the trpC promoter.

Transformants were grown in CMC and CM, and their mycelia were observed under fluorescence microscopy. Of 10 pYTGFPc transformants, 7 expressed GFP. In these transformants, GFP fluorescence did not localize in any cell components throughout mycelia grown in CMC and CM (Fig 8). Of 13 pREN1-GFP transformants, 9 emitted GFP fluorescence; of 14 pGFP-REN1 transformants, 3 emitted GFP fluorescence. In all the transformants expressing Ren1-GFP and GFP-Ren1 fusions, GFP fluorescence was targeted in nuclei in mycelial cells grown in CMC and CM (Fig 8), suggesting that Ren1 localizes in nuclei and acts as a transcription regulator.



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  		Figure 8. Intracellular localization of the GFP-tagged Ren1. Transformants with pYTGFPc (A and D), pREN1-GFP (B and E), and pGFP-REN1 (C and F) were grown in CMC and CM at 25° for 4 days. (A–C) Differential interference contrast images. (D–F) GFP fluorescence images. Bars, 20 µm.

The REN1 homologs:
DNA gel blot analysis showed the presence of the REN1 homologs in the wild-type strain Mel02010. As shown in Fig 4B, the 5.8-kb BamHI fragment contains REN1, and the 2.5-, 7.0-, and 23.0-kb fragments contain the homologs. To isolate the homologs, a cosmid genomic library of Mel02010 was screened with a probe of the 1.2-kb ClaI-HindIII fragment used in Fig 4B. Positive clones were digested with BamHI, and pcREN1h-1, pcREN1h-2, and pcREN1h-3, which contained the 2.5-, 7.0-, and 23.0-kb BamHI fragments, respectively, were isolated. The REN1 homolog (REN1h-1) in pcREN1h-1 was sequenced. Comparison of sequences of REN1 and REN1h-1 detected a highly conserved region of ~0.6 kb (91.4% identity) within the third exon of REN1. However, REN1h-1 has a termination codon in this region. Their 5' and 3' regions flanking to the conserved region have lower identity (~50%), and REN1h-1 contains many termination codons in these regions (data not shown). Partial sequencing of the REN1 homologs in pcREN1h-2 and pcREN1h-3 revealed that the homologs show strong similarity to REN1h-1 and also have many termination codons (data not shown). These results strongly suggest that the REN1 homologs are pseudogenes.


*  DISCUSSION
*TOP
 *ABSTRACT
 *MATERIALS AND METHODS
 *RESULTS
 *DISCUSSION
*LITERATURE CITED

Molecular analysis of the REMI mutant B50-19 of the plant pathogenic fungus F. oxysporum identified the REN1 gene, essential for development of microconidia and macroconidia. In F. oxysporum, microconidia are formed from phialides in false heads by basipetal division; macroconidia are formed from phialides on conidiophores by basipetal division. The REN1 mutants lack normal conidiophores and phialides and form rod-shaped, slender cells directly from hyphae by acropetal division. Thus, REN1 is required for the correct differentiation of conidiophores and phialides. The mutants produce rod-shaped cells in a single chain at the early stage of development and frequently form the cells in branching chains at the later stage of development. Since the wild-type strain never forms microconidia and macroconidia in a chain, cell division switches from acropetal to basipetal mode at the phialide stage. REN1 also may be essential for the switch from acropetal to basipetal division during conidiogenesis.

The REN1 mutants form normal chlamydospores. The number of chlamydospores of the mutants was also similar to that of the wild type. These results indicate that REN1 is not required for chlamydospore formation. Chlamydospores are formed acrogenously from hyphae or by the modification of hyphal cells. Thus, it appears that the developmental pathway of chlamydospores is genetically independent from those of microconidia and macroconidia.

Ren1 shows significant similarity to MedA of A. nidulans and Acr1 of M. grisea. Modes of conidiogenesis are highly complex in conidial ascomycete fungi, and at least 20 modes of conidial ontogeny have been described (COLE 1986 Down). Conidial ontogeny in F. oxysporum and A. nidulans is phialidic, and that in M. grisea is sympodial (Fig 9). In A. nidulans, the conidiophore vesicle bears two types of sterigmata (metulae and phialides), and chains of conidia are produced from phialides (Fig 9B). A mutation at medA results in aberrant conidiophores with branching chains of metulae, delayed conidial differentiation, and frequent reinitiation of the secondary conidiophore (Fig 9B; CLUTTERBUCK 1969 Down; GEMS and CLUTTERBUCK 1994 Down; BUSBY et al. 1996 Down). In M. grisea, conidiogenesis involves the production of three-celled conidia, borne sympodially on an aerial conidiophore (Fig 9C). A mutation at ACR1 results in the production of head-to-tail (acropetal) arrays of conidia (Fig 9C; LAU and HAMER 1998 Down; NISHIMURA et al. 2000 Down). These observations demonstrate that mutations at REN1, medA, and ACR1 in these fungi result in a similar phenotype, in which conidiogenesis cells are reiterated in chains (Fig 9).



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  		Figure 9. Schematic of conidiogenesis of REN1, medA, and ACR1 mutants of F. oxysporum (A), A. nidulans (B), and M. grisea (C), respectively. ma, macroconidium; mi, microconidium; cs, chlamydospore.

Although MedA and Acr1 have been suggested to be transcription regulators involved in conidiation of these fungi (CLUTTERBUCK 1969 Down; MILLER et al. 1993 Down; GEMS and CLUTTERBUCK 1994 Down; BUSBY et al. 1996 Down; LAU and HAMER 1998 Down; NISHIMURA et al. 2000 Down), their nuclear localization has not been verified. We verified nuclear import of Ren1 by using strains expressing the GFP-tagged Ren1. Both the Ren1-GFP and GFP-Ren1 fusion proteins were targeted to nuclei. The fact that the nuclear localization of Ren1 is not affected by either N-terminal or C-terminal fusions of GFP suggests that Ren1 has the nuclear import signal in the internal region. The structural similarity among Ren1, MedA, and Acr1 and the nuclear localization of Ren1 strongly suggest that these proteins represent members of a novel class of conserved regulators controlling conidial pattern formation. Recently, the genome sequence of F. graminearum has become available on the website of the Whitehead Institute (http://www-genome.wi.mit.edu/annotation/fungi/fusarium/). We searched the REN1 homolog of F. graminearum on the website and found a putative gene, which has the exon/intron organization similar to REN1 and encodes a protein strongly similar to Ren1.

In A. nidulans, five transcription regulator genes (brlA, abaA, wetA, medA, and stuA) have been identified as controlling conidial development (CLUTTERBUCK 1969 Down; BOYLAN et al. 1987 Down; ADAMS and TIMBERLAKE 1988 Down; MIRABITO et al. 1989 Down; MILLER et al. 1992 Down; BUSBY et al. 1996 Down; ADAMS et al. 1998 Down). BrlA, AbaA, and WetA comprise the core pathway required for the transition from vegetative hyphae to conidia (BOYLAN et al. 1987 Down; SEWALL et al. 1990 Down; MARSHALL and TIMBERLAKE 1991 Down; ADAMS et al. 1998 Down). BrlA is required to initiate conidiation (HAN et al. 1993 Down; PRADE and TIMBERLAKE 1993 Down). AbaA is required for phialide differentiation, and WetA is essential for maturation of conidia (SEWALL et al. 1990 Down; MARSHALL and TIMBERLAKE 1991 Down). Some target genes have been identified for BrlA and AbaA (ARAMAYO and TIMBERLAKE 1993 Down; CHANG and TIMBERLAKE 1993 Down; ANDRIANOPOULOS and TIMBERLAKE 1994 Down).

StuA and MedA represent components of a developmental modifier pathway required for correct cellular differentiation (CLUTTERBUCK 1969 Down; MILLER et al. 1992 Down; BUSBY et al. 1996 Down; WU and MILLER 1997 Down). StuA modulates expression of the core regulatory genes brlA and abaA (MILLER et al. 1992 Down). MedA represses premature expression of brlA during early development and downregulates brlA during later stages (BUSBY et al. 1996 Down). MedA is also required as a coactivator of the abaA expression (BUSBY et al. 1996 Down). Conidiation of the medA mutant is not completely blocked, but is delayed (CLUTTERBUCK 1969 Down; GEMS and CLUTTERBUCK 1994 Down). However, a mutation at REN1 in F. oxysporum leads to a lack of normal conidiophores and phialides and to production of aberrant conidia. The aberrant conidia also branch, unlike normal conidiogenesis cells and conidia. We propose that REN1 comprises the core pathway for the development of microconidia and macroconidia in F. oxysporum. Identification of the target genes of Ren1 is needed to assess the precise function of Ren1 in conidial development of F. oxysporum.

The REN1 locus was found to have at least three mRNAs of ~2.6, 3.4, and 4.8 kb. When vegetative mycelia grown in CM were inoculated in CMC to induce conidiation, microconidia and macroconidia occurred from 12 and 48 hr, respectively, after inoculation, and their numbers increased to 120 hr. During incubation in CMC, two mRNA of ~3.4 and 4.8 kb accumulated in fungal tissue at the early stage (12–60 hr), and an additional ~2.6-kb mRNA also accumulated at the later stage (72–120 hr). Thus, at least 3.4- and 4.8-kb mRNAs seem to be necessary for development of microconidia and macroconidia. These three mRNAs were also detected in mycelia grown in the nonconidiation media CM and MM for 96 hr, although REN1 is dispensable for vegetative growth. The Ren1-GFP fusion proteins localized in nuclei in mycelial cells grown in CMC and also in CM. Thus, the REN1 expression and nuclear localization of Ren1 are essential, but not enough, for conidial development.

The A. nidulans medA locus has two transcription start sites that give rise to two mRNAs (MILLER et al. 1993 Down). Both mRNAs have long reader sequences that contain multiple mini-ORFs, although the roles of two transcripts and mini-ORFs have not been characterized (MILLER et al. 1993 Down). Although transcription start sites of three mRNAs of REN1 have not been identified, three mini-ORFs (225, 210, and 270 bp) were found within the 1.5-kb region upstream of the REN1 ORF (data not shown). These mini-ORFs are probably not exons of REN1, because we could not find introns with consensus sequences for 5' and 3' splice signals to join mini-ORFs and REN1 ORF as a single ORF. The brlA and stuA loci in A. nidulans also have two overlapping transcription units (brlA{alpha} and brlAß in brlA and stuA{alpha} and stuAß in stuA), which are different in transcription start sites (MILLER et al. 1992 Down; HAN et al. 1993 Down; PRADE and TIMBERLAKE 1993 Down; WU and MILLER 1997 Down). Both transcription units in brlA and stuA are essential for normal development of conidia (MILLER et al. 1992 Down; HAN et al. 1993 Down; PRADE and TIMBERLAKE 1993 Down; WU and MILLER 1997 Down). Complexity in transcriptional and translational regulation is probably a common feature in the developmentally regulatory genes for conidiation in these fungi.

The REN1 mutants of F. oxysporum could cause wilt symptoms in susceptible melon plants, as did the wild type, under the conditions tested. In contrast, a mutation at ACR1 in M. grisea results in a drastic reduction of virulence in rice plants (LAU and HAMER 1998 Down). The lifestyles and infection mechanisms of the soil-borne pathogen F. oxysporum and the foliar pathogen M. grisea are highly divergent. F. oxysporum infects host plants in a manner typical of soil-borne pathogens: conidia germinate in response to root exudates, produce penetration hyphae that attach to root surface and penetrate it directly, and grow invasively in host plant tissue (RODRIGUEZ-GALVEZ and MENDGEN 1995 Down). Conversely, conidia of M. grisea attach to the leaf, germinate, and differentiate dome-shaped, melanized appressoria, able to generate sufficient turgor pressure to penetrate the plant cuticlar surface (TALBOT 1995 Down). Reduced virulence phenotype of the ACR1 mutants is due mainly to inability to form appressoria (LAU and HAMER 1998 Down). A variety of conidiation mutants of M. grisea also fail to produce normal appressoria, resulting in nonpathogenic or reduced virulent phenotypes (HAMER et al. 1989 Down; SHI and LEUNG 1995 Down; SHI et al. 1998 Down). These observations demonstrate that conidiation and appressorium formation in M. grisea may involve an overlapping set of gene products (HAMER et al. 1989 Down; LAU and HAMER 1998 Down; SHI et al. 1998 Down). F. oxysporum directly penetrate root surface without formation of typical appressoria (RODRIGUEZ-GALVEZ and MENDGEN 1995 Down). Thus, Ren1 probably is not essential for penetration of root surface or for colonization in the plant tissue.


*  FOOTNOTES

Sequence data from this article have been deposited with the DDBJ/EMBL/GenBank Data Libraries under accession nos. AB096070 (REN1) and AB113797 (REN1h-1). Back


*  ACKNOWLEDGMENTS

We are grateful to Sally A. Leong and Yoshitaka Takano for providing pMLF2 and the EGFP gene, respectively. We thank Marie Nishimura, Takayuki Aoki, Masayuki Togawa, Hirofumi Yoshioka, Kazuhito Kawakita, and Noriyuki Doke for valuable suggestions, and the Radioisotope Research Center, Nagoya University, for technical assistance. This work was supported by research grants from the Japanese Society for Promotion of Sciences (nos. 13460022, 14656017, and 15208005).

Manuscript received July 8, 2003; Accepted for publication August 14, 2003.


*  LITERATURE CITED
*TOP
 *ABSTRACT
 *MATERIALS AND METHODS
 *RESULTS
 *DISCUSSION
 *LITERATURE CITED

ADAMS, T. H. and W. E. TIMBERLAKE, 1988  brlA is necessary and sufficient to direct conidiophore development in Aspergillus nidulans.. Cell 54:353-362.[CrossRef][Medline]

ADAMS, T. H., J. K. WIESER, and J. H. YU, 1998  Asexual sporulation in Aspergillus nidulans.. Microbiol. Mol. Biol. Rev. 62:35-54.[Abstract/Free Full Text]

ALTSCHUL, S. F., T. L. MADDEN, A. A. SCHÄFER, J. ZHANG, and Z. ZHANG et al., 1997  Gapped BLAST and PSI-BLAST: a new generation of protein database search programs. Nucleic Acids Res. 25:3389-3402.[Abstract/Free Full Text]

AN, Z., M. L. FARMAN, A. BUDDE, S. TAURA, and S. A. LEONG, 1996  New cosmid vectors for library construction, chromosome walking and restriction mapping in filamentous fungi. Gene 176:93-96.[CrossRef][Medline]

ANDRIANOPOULOS, A. and W. E. TIMBERLAKE, 1994  The Aspergillus nidulans abaA gene encodes a transcriptional activator that acts as a genetic switch to control development. Mol. Cell. Biol. 14:2503-2515.[Abstract/Free Full Text]

ARAMAYO, R. and W. E. TIMBERLAKE, 1993  The Aspergillus nidulans yA gene is regulated by abaA.. EMBO J. 12:2039-2048.[Medline]

ARMSTRONG, G. M., and J. K. ARMSTRONG, 1981 Formae speciales and races of Fusarium oxysporum causing wilt diseases, pp. 391–399 in Fusarium Disease, Biology and Taxonomy, edited by P. E. NELSON, T. A. TOUSSOUM and R. J. COOK. Pennsylvania State University Press, University Park, PA.

BECKMAN, C. H., 1987 The Nature of Wilt Diseases of Plants. The American Phytopathological Society Press, St. Paul.

BORNEMAN, A. R., M. J. HYNES, and A. ANDRIANOPOULOS, 2000  The abaA homologue of Penicillium merneffei participates in two developmental programmes: conidiation and dimorphic growth. Mol. Microbiol. 38:1034-1047.[CrossRef][Medline]

BOYLAN, M. T., P. M. MIRABITO, C. E. WILLET, C. R. ZIMMERMANN, and W. E. TIMBERLAKE, 1987  Isolation and physical characterization of three essential conidiation genes from Aspergillus nidulans.. Mol. Cell. Biol. 7:3113-3118.[Abstract/Free Full Text]

BRUCHEZ, J. J. P., J. EBERLE, and V. E. RUSSO, 1993  Regulatory sequences in the transcription of Neurospora crassa gene: CAAT box, TATA box, intron, poly(A) tail formation sequences. Fungal Genet. Newsl. 40:89-96.

BUSBY, T. M., K. Y. MILLER, and B. L. MILLER, 1996  Suppression and enhancement of the Aspergillus nidulans medusa mutation by altered dosage of the bristle and stunted genes. Genetics 143:155-163.[Abstract]

CAELLES, C., M. DELSENY, and P. PUIGDOMENECH, 1992  The hydroxyproline-rich glycoprotein gene from Oryza sativa.. Plant Mol. Biol. 18:617-619.[CrossRef][Medline]

CAPPELLINI, R. A. and J. L. PETERSON, 1965  Macroconidium formation in submerged cultures by a nonsporulating strain of Gibberella zeae.. Mycologia 57:962-966.

CHANG, Y. G. and W. E. TIMBERLAKE, 1993  Identification of Aspergillus brlA response elements (BREs) by genetic selection in yeast. Genetics 133:29-38.[Abstract]

CLUTTERBUCK, A. J., 1969  A mutational analysis of conidial development in Aspergillus nidulans.. Genetics 63:29-38.

COLE, G. T, 1986  Models of cell differentiation in conidial fungi. Microbiol. Rev. 50:95-132.[Free Full Text]

COUTEAUDIER, Y. and C. ALABOUVETTE, 1990  Survival and inoculum potential of conidia and chlamydospores of Fusarium oxysporum f. sp. lini in soil. Can. J. Microbiol. 36:551-556.[Medline]

DAHLBERG, K. R. and J. L. VAN ETTEN, 1982  Physiology and biochemistry of fungal sporulation. Annu. Rev. Phytopathol. 20:218-301.

FISHER, N. L., L. W. BURGESS, T. A. TOUSSOUN, and P. E. NELSON, 1982  Carnation leaves as a substrate and for preserving cultures of Fusarium species. Phytopathology 72:151-153.

GALAGAN, J. E., S. E. CALVO, K. A. BORKOVICH, E. U. SELKER, and N. D. READ et al., 2003  The genome sequence of the filamentous fungus Neurospora crassa.. Nature 422:859-868.[CrossRef][Medline]

GEMS, D. H. and A. J. CLUTTERBUCK, 1994  Enhancers of conidiation mutants in Aspergillus nidulans.. Genetics 137:79-85.[Abstract]

GRITZ, L. and J. DAVIES, 1983  Plasmid-encoded hygromycin B resistance: the sequence of hygromycin B phosphotransferase gene and its expression in Escherichia coli and Saccharomyces cerevisiae.. Gene 25:179-188.[CrossRef][Medline]

HAMER, J. E., B. VALENT, and F. G. CHUMLEY, 1989  Mutations at the SMO locus affect the shape of diverse cell types in the rice blast fungus. Genetics 122:351-361.[Abstract/Free Full Text]

HAN, S., J. NAVARRO, R. A. GREVE, and T. H. ADAMS, 1993  Translational repression of brlA expression prevents premature development in Aspergillus.. EMBO J. 12:2449-2457.