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Department of Microbiology and Plant Pathology, Forestry and Agricultural Biotechnology Institute, Faculty of Natural and Agricultural Sciences, University of Pretoria, Pretoria, South Africa
Pedro W. Crous
Centraalbureau voor Schimmelcultures, Uppsalalaan 8, 3584 CT Utrecht, The Netherlands
Teresa A. Coutinho
Brenda D. Wingfield
Michael J. Wingfield 1
Department of Microbiology and Plant Pathology and Department of Genetics, Forestry and Agricultural, Biotechnology Institute, Faculty of Natural and Agricultural Sciences, University of Pretoria, Pretoria, South Africa
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ABSTRACT |
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Botryosphaeria lutea (anamorph Fusicoccum luteum) most easily is distinguished from other Botryosphaeria spp. by a yellow pigment that is formed in young cultures. This fungus has been reported from a number of cultivated hosts in New Zealand and Portugal. During a survey of Botryosphaeria fungi that occur on native Acacia species in Australia, a yellow pigment was observed in some cultures. These isolates were morphologically similar to B. lutea, but the pigment differed slightly from the one formed by authentic B. lutea isolates. Preliminary data also revealed small differences in ITS rDNA sequence data. The aim of this study was to determine whether these small differences were indicative of separate species or merely variations within B. lutea. Anamorph, teleomorph and culture morphology were compared between B. lutea and Acacia isolates from Australia. Sequence data of two other genome regions, namely the ß-tubulin and EF1-
gene and intron regions, were combined with ITS rDNA sequence data to determine the phylogenetic relationship between these isolates. Isolates of B. lutea and those from Australian Acacia species were not significantly different in spore morphology. The yellow pigment, however, was much more distinct in cultures of B. lutea than in cultures from Acacia. There were only a few base pair variations in each of the analyzed gene regions, but these variations were fixed in the two groups in all regions. By combining these data it was clear that B. lutea and the isolates from Acacia were distinct species, albeit very closely related. We, therefore, propose the new epithet B. australis for the fungus from Australia. Botryosphaeria australis also was isolated in this study from exotic Sequoiadendron trees in Australia. Re-analyses of GenBank data in this study showed that B. australis also occurs on other native Australian hosts, namely a Banksia sp. and a Eucalyptus sp., as well as a native Protea sp. in South Africa and on Pistachio in Italy. These records from GenBank have been identified previously as B. lutea. The common occurrence of B. australis on a variety of native hosts across Australia suggests that this fungus is native to this area.
Key words: culture, conidia, morphology, multiple genealogy concordance, native hosts, phylogeny, Southern Hemisphere
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INTRODUCTION |
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSTAXONOMYDISCUSSIONLITERATURE CITED |
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, Wingfield et al 2001a, b, Denman et al 2003). To establish and maintain these plantations, germplasm must be introduced into different countries, which can result in the accidental introduction of exotic pathogens to new environments (Palm 1999, Wingfield et al 2001a). In this regard, a group of pathogens that is overlooked easily is Botryosphaeria spp., which lives as endophytes in healthy plants and seeds for part of its life cycle (Smith et al 1996, Burgess and Wingfield 2002).
Once introduced into a new environment, Botryosphaeria spp. can threaten both native and exotic hosts (Burgess and Wingfield 2002). This is because many of these fungi have a wide host range (Wingfield et al 2001a). To reduce this threat, it is necessary to obtain a clear knowledge of the taxonomy and ecology of Botryosphaeria spp., both in their areas of natural occurrence and in countries where these trees are planted commercially (Palm 1999, Wingfield et al 2001b).
Members of the genus Botryosphaeria commonly are accepted to be difficult to identify to species level. For a number of years after the circumscription of the genus, ascomatal morphology and host range were considered characteristic for different species (Cesati and De Notaris 1863, Saccardo 1877, Trotter 1928). This resulted in considerable difficulty because the teleomorph is not found frequently in nature and is produced only rarely in culture. In addition, it currently is understood that some Botryosphaeria spp. can infect a wide variety of hosts (Stevens and Jenkins 1924, Punithalingham and Holliday 1973, Punithalingham and Waller 1973). Furthermore, teleomorph characters vary on different hosts and often are not distinctive at species level (von Arx and Müller 1954, Slippers et al 2004).
Conidial and cultural morphology often are used to distinguish different Botryosphaeria spp. (Shoemaker 1964, Pennycook and Samuels 1985, Denman et al 2000, Slippers et al 2004). The anamorphs of these fungi are encountered commonly, both in nature and in culture. Distinctive features of conidia are the shape, size, length/width ratio, septation, content, color, wall thickness and ornamentation. In addition, the general growth pattern, speed and color of a colony on agar sometimes are informative for species identification (Pennycook and Samuels 1985, Phillips et al 2002, Slippers et al 2004).
In recent years, various DNA based techniques have been used to distinguish between Botryosphaeria spp. These techniques include dominant and codominant molecular markers such as RAPDs, ISSRs and microsatellites (Burgess et al 2001, Smith and Stanosz 2001, Zhou et al 2001) and sequence data for a number of DNA regions ( Jacobs and Rehner 1998, Denman et al 2000, Zhou and Stanosz 2001a, b, Phillips et al 2002, Slippers et al 2004). However, these data have not always been sufficient to distinguish boundaries between closely related or cryptic species. In such cases, multiple gene genealogies have been used (de Wet et al 2003, Slippers et al 2004). These molecular data, combined with morphological and ecological data, allow for robust identification of Botryosphaeria spp.
Pennycook and Samuels (1985) described an anamorph of a Botryosphaeria species, Fusicoccum luteum Pennycook & Samuels, from New Zealand. This species could be distinguished most easily from other botryosphaeriaceous fungi from Malus sp., Populus sp. and Actinidia deliciosa by a yellow pigment produced in young cultures. The teleomorph was unknown. A few years later, Phillips et al (2002) also noticed a yellow pigment in cultures derived from Botryosphaeria ascomata on Vitis vinifera in Portugal. Using ribosomal DNA (rDNA) sequence and SSCP, RAPD and morphological data, the Portuguese fungus was shown to be similar to F. luteum, for which the teleomorph B. lutea A.J.L. Phillips was described. Botryosphaeria lutea, thus, seems to be a more important pathogen of fruit and forestry crops than previously was recognized. This pathogen evidently has been mistaken as well for B. dothidea (Fr. : Moug.) Ces. & De Not. (Phillips et al 2002).
Botryosphaeria rhodina (Berk. & Curt.) Arx and B. dothidea both have been reported from native Australian Acacia spp., where these trees are planted as exotics (Roux 1998, Roux et al 2001). However, during a recent survey of Botryosphaeria spp. on native Australian flora, some cultures from Acacia sp. produced a yellow pigment in culture, similar to that described for B. lutea. Initial ITS rDNA sequence data confirmed a close relationship with B. lutea, but some sequence divergence also was obvious. The aim of this study, therefore, was to determine the relationship between these isolates from Acacia in Australia and B. lutea isolates from New Zealand and Portugal. To evaluate the phylogenetic significance of the sequence variation seen in the ITS region, sequence data from three gene regions (ITS rDNA, ß-tubulin and translation elongation factor 1 [EF-1]) were compared. Teleomorph, anamorph and cultural characters also were considered.
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MATERIALS AND METHODS |
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). Four similar isolates also were obtained from samples of diseased Sequoiadendron gigantea growing as an exotic in Canberra (TABLE I). Two isolates of B. lutea (one ex-type) were provided by AJL Phillips (CAP002, CAP037) (TABLE I). Two isolates originating from the original description of F. luteum (one ex-type) by Pennycook and Samuels (1985) also were included (TABLE I). Isolates were maintained on malt-yeast extract agar (MYA) (2% malt extract, 0.2% yeast extract and 2% agar; Biolab, Johannesburg, South Africa) at 25 C in the dark or under near UV light. Isolates are maintained in the Culture Collection (CMW) of the Forestry and Agricultural Biotechnology Institute (FABI), University of Pretoria, Pretoria, South Africa.
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and Smith et al (2001). Four isolates from Acacia and Sequoiadendron from Australia were used in phylogenetic comparisons, with two isolates from each of the studies of Pennycook and Samuels (1985) and Phillips et al (2002), including the ex-type cultures of B. lutea and F. luteum from these studies (TABLE I
). DNA sequences of other Botryosphaeria spp. that were included in the analysis for comparative purposes were from Slippers et al (2004) (TABLE I). Furthermore, Smith and Stanosz (2001) and Denman et al (2003) used ITS rDNA sequence comparisons to identify B. lutea or F. luteum isolates from native Banksia spp., Eucalyptus marginata and a Protea sp. in Australia and South Africa. ITS sequences from these studies were obtained from GenBank and compared with the isolates examined in the present study (TABLE I).
Sequences of three nuclear loci were used for phylogenetic comparisons between isolates. The region spanning the 3' end of the 16S (small-subunit) rRNA gene, the first internal transcribed spacer (ITS1), the complete 5.8S rRNA gene, the second ITS (ITS2) and the 5' end of the 26S (large-subunit) rRNA gene was amplified using the primers ITS1 and ITS4 (White et al 1990). A region of the ß-tubulin gene was amplified using the primers Bt2a and Bt2b (Glass and Donaldson 1995). In addition, a part of the EF1- was amplified using the primers EF1-728F and EF1-986R (Carbone et al 1999). PCR reaction mixtures, PCR conditions and visualization of amplicons are as described by Slippers et al (2004). The amplicons of all three DNA regions were purified and sequenced as described by Slippers et al (2004), using the same primers used to generate the amplicons.
Sequence data were analyzed with Sequence Navigator version 1.0.1TM (Perkin Elmer Applied Biosystems, Foster City, California) and manually aligned by inserting gaps. Gaps were treated as a fifth character, and all characters were unordered and of equal weight. A partition homogeneity test was done to determine whether the datasets were congruent (Farris et al 1995, Huelsenbeck et al 1996). Estimated levels of homoplasy and phylogenetic signal (retention and consistency indices and g1-value) (Hillis and Huelsenbeck 1992) were determined. Maximum-parsimonious trees were determined with PAUP (Phylogenetic Analysis Using Parsimony) version 4.0b10 (Swofford 1999), with heuristic searches of only informative characters and tree bisection and reconstruction (TBR) as branch-swapping algorithm (random stepwise addition). Maxtrees were unlimited, branches of zero length were collapsed, and all multiple equally parsimonious trees were saved. Branch and branch-node supports were determined using 1000 bootstrap replicates (Felsenstein 1985) and decay analysis of the branch nodes using Autodecay (Eriksson 1998). Phylogenetic species hypotheses were tested using distance analyses with the neighbor-joining algorithm, using both an uncorrected p-factor and HKY85 parameters alternatively in PAUP.
To test the consistency of branches in the combined dataset, the three partial gene sequence datasets were analyzed separately but in the same way as described above. The ITS rDNA dataset was expanded and analyzed separately to include isolates for which only ITS rDNA data were available from GenBank.
Morphological characterization. – All isolates were grown on sterilized pine needles that were placed on water agar (WA) (2% agar; Biolab Midrand, Johannesburg, South Africa) at 25 C under near UV light, to promote sporulation. Fruiting structures from in vivo and in vitro collections were sectioned with an American Optical Freezing Microtome or by hand and mounted in clear lactophenol. Morphological observations were made and images were recorded on a light microscope and Axiocam digital camera (Carl Zeiss, Germany). The morphology of these samples was compared with material of B. lutea (LISE94070 [holotype] and LISE94073) and F. luteum (PDD45400).
Growth rate, colony morphology and color (Rayner 1970) of isolates obtained during this study, as well as of ex-type isolates of B. lutea and F. luteum, were determined. Two isolates of each species were incubated on potato-dextrose agar (PDA) (0.4% potato extract, 2% dextrose, 1.5% agar; Biolab, Midrand, Johannesburg, South Africa) at 5 C intervals ranging from 10 to 35 C in the dark. Growth rate was measured at the leading edge in 24 h intervals. The experiment was repeated for the new species described below.
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RESULTS |
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) were amplified for all isolates. Sequence data at the 5' and 3' ends were deleted from the dataset if they were doubtful (GenBank AY339248–AY339271). The partition homogeneity test of the ITS-rDNA, ß-tubulin and EF1- datasets, indicated that they were congruent (P value = 0.53). The data from the three regions were combined and the total dataset consisted of 1324 characters after alignment (TreeBASE S1008 [study]; M1704 [matrix]). A seven base pair region in the EF1- region was repeated twice in most species. Isolates of B. ribis contained two extra of these repeats, which were coded to represent only two evolutionary events and not 14 as was the case before the coding. Of the remaining characters, 322 were parsimony informative and used in the analyses. This combined dataset contained significant phylogenetic signal compared to random trees (P < 0.01; g1 = –0.97) (Hillis and Huelsenbeck 1992). After heuristic searches in PAUP, three equally most-parsimonious trees of 540 steps were retained (CI = 0.843; RI = 0.909) (FIG. 1). Trees obtained using distance methods were the same as those obtained using parsimony.
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). Although the branches separating these two clades were short, compared to the branches separating other well-defined species in the analysis, they were strongly supported (d5/96% and d5/100% decay values and bootstrap support). The separation also was supported in the individual analyses of the sequence datasets of the three gene regions (analyses done using the same parameters as for the combined data-set) (FIG. 2A–C). Analysis of the sequences between these two groups showed that the alleles were fixed in the two groups at 14 of the 15 polymorphic loci. Of these 15 polymorphic sites, four were indels, 10 transitions and a transversion. The bias toward transitions is considered in the distance analysis (HKY85 parameters) and does not change the interpretation of the results. Among the isolates studied here, these two clades are considered phylogenetically separate and the fungus from Australia is described here as new.
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, Denman et al 2003) separated into both B. lutea and B. australis clades, although the bootstrap values for both groups were low (63% and 73% respectively) (FIG. 3). Sequences from Actinidia (New Zealand) and Buck-inghamia (Australia) grouped with B. lutea. Isolates from Australian native hosts, including Eucalyptus and Banksia, and from a South African native Protea grouped with the newly identified Botryosphaeria sp. Three isolates from Banksia in Australia (Denman et al 2003) resided in a sister group of the B. lutea and B. australis clades.
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Morphological characterization. –
The isolates from Acacia spp. and Sequoiadendron giganteum produced anamorph structures on pine needles on WA within 2–3 wk. Teleomorph and anamorph structures of this fungus from field samples and from conidia formed in culture were similar in morphology to those of B. lutea and F. luteum (FIGS. 4–12). This new species produced a yellowish pigment in young cultures, as also was true for B. lutea. The fungus from Acacia and Sequoiadendron, however, could be distinguished from B. lutea and F. luteum by its longer conidia with a higher l/w ratio (TABLE II). Isolates of B. lutea also produce a much brighter yellow pigment in culture than the Australian isolates, especially at 25 C and higher. Unlike B. lutea, no yellow pigment was produced between 25–30 C by the Australian isolates.
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TAXONOMY |
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Botryosphaeria australis Slippers, Crous & M.J. Wingf., sp. nov. FIGS. 4–14
Anamorph. – Fusicoccum australe Slippers, Crous & M.J. Wingf., sp. nov.
Etymology. – Referring to the origin in the Southern Hemisphere.
Note. –
The name B. australis (Cooke) Petrak is reported by Gibson (1975) in a checklist of fungi from Eucalyptus. A literature survey, however, revealed that Petrak did not describe such a taxon. The listing in Gibson, therefore, is incorrect and the name is available for use.
Ascostromata per corticem erumpentia, 1.2 mm diametro. Ascomata pseudothecialia, 2–10 botyroide aggregata, interdum solitaria, globosa ostiolo centrale, papillata vel glabra, inclusa cum solum papillis emergentibus usque ad 
emergentia, nigra, 100–300 µm; paries pseudothecii e 5–8 stratis texturae angularis, extus e cellulis atrobrunneis vel brunneis composita, intus e cellulis hyalinis revestimentum loculi facientes. Asci bitunicati, clavati, 60–125 x 16–25 µm, inter pseudoparaphyses multas, filiformes, septatas, raro apicem versus ramosas, 3–4 µm latas. Ascosporae fusoideae vel ovoideae, 20–23(–25) x 7–8(–9) µm, unicellulares, hyalinae, laeves, contentis granularibus, in asco biseriatae. Conidiomata (in "WA" in acis pinorum sterilifactis in 7–21 diebus formata) pycnidialia, superficialia, globosa, plerumque solitaria mycelio tectaque. Conidia fusiformia, basibus subtruncatis vel obtuse rotundatis, (18–)23–26(–30) x 5–6(–7.5) µm, hyalina, unicellularia raro septum ante germinationem facientia, laevia contentis granularibus. Cellulae conidiogenae holoblasticae, hyalinae, subcylindricae, 10–14 x 2–3 µm, percurrenter proliferantes cum 1–2 proliferationibus, inspissatione periclinali. Spermatia non visa.
Ascostromata erumpent through the bark, 1.2 mm diam. Ascomata pseudothecial, forming botryose aggregates of 2–10, sometimes solitary; globose with a central ostiole, papillate or not, imbedded with only papilla emerging up to emergent, black, 100–300 µm; pseudothecial wall comprising 5–8 layers of textura angularis, outer region of dark brown or brown cells, inner region 3–6 layers of hyaline cells lining the locules. Asci bitunicate, clavate, 60–125 x 16–25 µm, 8-spored, between numerous filiform, septate pseudoparaphyses, rarely branched in the upper parts, 3–4 µm wide. Ascospores fusoid to ovoid, 20–23(–25) x 7–8(–9) µm (average of 50 ascospores 21.9 x 7.6 µm, l/w 2.9), unicellular, hyaline, smooth with granular contents, biseriate in the ascus. Conidiomata (formed on WA on sterilized pine needles within 7–21 d) pycnidial, superficial, globose, mostly solitary and covered by mycelium. Conidia fusiform, base subtruncate, (18–)23–26(–30) x 5–6(–7.5) µm (average of 240 conidia 24.7 x 5.1 µm, l/w 4.8), hyaline, unicellular, rarely forming a septum before germination, smooth with granular contents. Conidiogenous cells holoblastic, hyaline, subcylindrical, 10–14 x 2–3 µm, phialidic with periclinal thickening or proliferating percurrently with 1–4 proliferations. Spermatia not observed. Cultures having buff (19''f) to light primrose (23''b) colonies, light yellowish pigment diffusing into the medium most noticeably between 15–20 C in the dark, becoming olivaceous buff (21'''d) to olivaceous gray (21'''''i) after 5–6 d, with a sparse to moderately dense, appressed mycelial mat in center with sparse tufts of aerial mycelium around edges, margin smooth. Optimum temperature for growth 25 C, colony reaching 48 mm diam on PDA after 4 d at 25 C in the dark.
Specimens examined. – AUSTRALIA. VICTORIA: Batemans Bay, Acacia sp., M.J. Wingfield (HOLOTY PE PREM57589) (culture CMW6838); Batemans Bay, Acacia sp., M.J. Wingfield (PREM57590); Batemans Bay, Acacia sp., M.J. Wingfield (PREM57592); Batemans Bay, Acacia sp., M.J. Wingfield (PREM57593); ACT: Canberra, Sequoiadendron sp., M.J. Wingfield (PREM57594); Canberra, Sequoiadendron sp., M.J. Wingfield (PREM57595).
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DISCUSSION |
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The genetic and subsequent taxonomic separation of the closely related species B. lutea and B. australis was confirmed using the phylogenetic-species concept. Sequence variation within the ITS, ß-tubulin and EF1- regions were small and were considered insignificant, if compared to the divergence between other well-defined Botryosphaeria spp. The alleles, however, were distributed in the same manner or fixed for the two groups in each of the three gene regions. These fixed alleles over multiple gene regions indicate a barrier to genetic exchange and are considered indicative of phylogenetic species (Taylor et al 2000). This phylogenetic separation confirmed the taxonomic value of small but distinct phenotypic variation that otherwise would have been overlooked. The combination of these DNA based and phenotypic data are considered sufficiently robust evidence to treat these fungi as separate taxa.
The distinction between B. lutea and B. australis was not recognized in previous studies based only on ITS rDNA sequence data (Smith and Stanosz 2001, Zhou and Stanosz 2001a, Denman et al 2003). This was due to the small ITS sequence divergence between them. The fact that we had access to a much larger collection of isolates also facilitated the discovery of the new taxon. ITS data alone thus can obscure the true species diversity in Botryosphaeria. This is similar to B. ribis and B. parva (Slippers et al 2004), or Diplodia pinea (Desm.) Kickx. (= S. sapinea) and D. scrobiculata de Wet, Slippers & M.J. Wingf. (de Wet et al 2003), that were considered to represent single species based on their ITS data alone. Multiple gene genealogies, however, showed that these species are phylogenetically distinct (de Wet et al 2003, Slippers et al 2004). These case studies provide good evidence to show that single gene genealogies are insufficient to distinguish cryptic Botryosphaeria spp.
Based on ITS rDNA sequences from GenBank, three isolates grouped closer to B. lutea and B. australis than any other Botryosphaeria spp. included in the study, but was separate from both of them. Due to the small differences between the species based on ITS data, it is not clear whether these isolates represent a further closely related species or an ITS variation of either B. lutea or B. australis. More gene sequence data is needed to clarify the true identity of these isolates. Similarly the small ITS sequence difference between the isolate from Pistacia in Italy and other B. australis isolates warrants further investigation.
Internal-transcribed spacer sequences provided by Smith and Stanosz (2001) and Zhou and Stanosz (2001a) for one isolate from a Eucalyptus sp. and one from a Banksia sp. were included in this study. Comparisons show that these isolates, previously treated as B. lutea, actually represent B. australis. In the studies of Smith and Stanosz (2001) and Zhou and Stanosz (2001a), B. australis isolates, however, could not be separated from ex-type isolates of F. luteum based on RAPD data. These authors also were not able to separate two other cryptic Botryosphaeria sp., namely B. ribis and B. parva, using RAPD data. Another similar example, in which RAPD data have been insufficient to define species, has been with the three recognized "morphotypes" of D. pinea. These three groups are distinguished using RAPD data but correspond to only two phylogenetic species (de Wet et al 2000, 2003).
Botryosphaeria lutea and B. australis cannot be distinguished based on teleomorph fruiting structures or ascospores. The conidial dimensions are equally misleading because they are similar in form and general appearance and their length and width dimensions overlap. This is not uncommon among Fusicoccum spp. Pennycook and Samuels (1985), Phillips et al (2002) and Slippers et al (2004) all have reported significant overlap in the sizes of Fusicoccum spp. In these cases and in our study the species, however, could be separated when averages of conidial sizes and septation were considered. Thus, on average, conidia of F. australe are longer and appear more slender (higher length/width ratio) than those of F. luteum.
Culture morphology was useful to distinguish between isolates of B. lutea and B. australis. Botryosphaeria australis produced a distinctly lighter and duller (more cream than yellow) pigment in young cultures than B. lutea. In the description of F. luteum (Pennycook and Samuels 1985) and B. lutea (Phillips et al 2002), the production of a yellow pigment in culture was the easiest way to distinguish this taxon from other species. Before these studies, this pigment was not considered taxonomically useful (Witcher and Clayton 1963). Recent studies of other botryosphaeriaceous fungi also have recognized the value of culture morphology as a useful tool to distinguish Botryosphaeria spp. ( Jacobs 2002, de Wet et al 2003, Slippers et al 2004).
Botryosphaeria australis differs in morphology and etiology from other botryosphaeriaceous fungi described from native Australian Acacia spp., Banksia spp. and Eucalyptus spp. Hansford (1954) described B. banksiae Hansford from Banksia marginata from Australia. However, the ascospores of this species are 1-seriate in the ascus and significantly different in size (17–20 x 13–15 µm). Botryosphaeria acaciae (Hansford) Dingley (= Physalospora acaciae Hansford) causes galls and cankers on Acacia spp. in Australia and New Zealand (Hansford 1954, Dingley 1970). Both of the latter studies, however, report that the teleomorph structures and galls also are associated with a Diplodia sp. Dingley (1970) reports "small papilla on one end" of the ascospores, which is absent in B. australis. This disease also was described from Australian Acacia by Scurfield (1966), who identified the causal agent as a fungus in the Sphaeriaceae. Based on the differences in anamorph, the lack of an association with a gall-forming disease and differences in ascospore morphology, we are confident that B. australis is not the same fungus as either of those mentioned above.
Botryosphaeria australis appears to be native to the Southern Hemisphere, most likely Australia. This hypothesis is based on the current known host and geographic distribution of this taxon. Botryosphaeria australis was the only Botryosphaeria sp. found on native species of Acacia in the different areas and over the two seasons that our collections were made. Isolates from previous studies also are identified here as B. australis, e.g., from E. marginata and Banksia caleyi in Australia and Protea cynaroides in South Africa (Smith and Stanosz 2001, Zhou and Stanosz 2001a, Denman et al 2003). Only one isolate from outside these regions grouped with B. australis; this was from Pistacia in Italy. Thus we are of the opinion that the exotic S. giganteum trees sampled during this study in Australia have become infected with a native pathogen.
Botryosphaeria lutea is common throughout Australasia and Portugal, but its origin is unknown. All reports from New Zealand have been from introduced hosts. Pennycook and Samuels (1985) collected this fungus from Malus, Populus and Actinidia species in New Zealand. Hartill (1991) also reported it from avocado from this area. The isolates from a native Australian Buckinghamia sp. (Denman et al 2003), however, also group with B. lutea. Smith and Stanosz (2001) identified F. luteum from the Australian native hosts, Banksia, Jacksonia horrida, Isopogon tribolus, Dryandra tenuifolia and a Leucopogon sp. These identifications, however, were based only on RAPD data, which did not separate B. lutea and B. australis. In Portugal B. lutea also occurs on introduced (Vitis and Sophora japonica) and indigenous (Fraxinus angustifolia) hosts (Phillips et al 2002). This fungus, thus, occurs on native and exotic hosts in both Europe and Australasia, which makes it difficult to predict its natural range.
Botryosphaeria australis and B. lutea have been moved between the Northern and Southern hemispheres, most likely on germplasm of commercially valuable species. This observation is based on the pattern of distribution and host ranges revealed in this study. It also is clear from our study that both these fungi can infect native and introduced or cultivated hosts in both regions. These introductions, thus, can have significant implications for agricultural and forestry industries and conservation of native flora. Population studies are needed to find the areas of greatest diversity and understand patterns of gene flow between populations of these two fungi. Such information will help to assess the current threat of these pathogens and help curtail their continued spread.
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FOOTNOTES |
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1 Corresponding author. E-mail: bernard.slippers{at}fabi.up.ac.za
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LITERATURE CITED |
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———, ———. 2002. Impact of fungal pathogens in natural forest ecosystems: a focus on Eucalyptus. In: Sivasithamparam K, Dixon KW, eds. Microorganisms in plant conservation and biodiversity. Dordrecht, The Netherlands: Kluwer Academic Press. p 285–306.
Carbone I, Anderson JB, Kohn LM. 1999. A method for designing primer sets for the speciation studies in filamentous ascomycetes. Mycologia 91:553–556.
Cesati V, de Notaris G. 1863. Schema di classificazione degli sferiacei italici. Comment Soc Crittog Ital 1, 4:177–240.
Denman S, Crous PW, Taylor JE, Kang JC, Pascoe I, Wingfield MJ. 2000. An overview of the taxonomic history of Botryosphaeria and a re-evaluation of its anamorphs based on morphology and ITS rDNA phylogeny. Stud Mycol 45:129–140.
———, ———, Groenewald JZ, Slippers B, Wingfield BD, Wingfield MJ. 2003. Circumscription of Botryosphaeria species associated with Proteaceae based on morphology and DNA sequence data. Mycologia 95:294–307.
de Wet J, Wingfield MJ, Coutinho TA, Wingfield BD. 2000. Characterization of Sphaeropsis sapinea isolates from South Africa, Mexico and Indonesia. Plant Dis 84:151–156.
———, Burgess T, Slippers B, Preisig O, Wingfield BD, Wingfield MJ. 2003. Multiple gene genealogies and microsatellite markers reflect relationships between morphotypes of Sphaeropsis sapinea and distinguish a new species of Diplodia. Mycol Res 107:557–566.[Medline]
Dingley JM. 1970. Records of fungi parasitic on plants in New Zealand 1966–1968. NZ J Agric Res 13:325–337.
Eriksson T. 1998. Autodecay version 4.0 (program distributed by the author). Department of Botany, Stockholm University, Stockholm.
Evans J. 1984. Plantation forestry in the tropics. Oxford: Clarendon Press. 472 p.
Farris JS, Kallersjo M, Kluge AG, Bult C. 1995. Testing significance of incongruence. Cladistics 10:315–319.
Felsenstein J. 1985. Confidence intervals on phylogenetics: an approach using bootstrap. Evolution 39:783–791.
Gibson IAS. 1975. Diseases of forest trees widely planted as exotics in the tropics and southern hemisphere. Part 1. Important members of the Myrtaceae, Leguminosae, Verbenaceae and Meliaceae. Kew, Surrey, England: Commonwealth Mycological Institute. 51 p.
Glass NL, Donaldson GC. 1995. Development of primer sets designed for use with the PCR to amplify conserved genes from filamentous Ascomycetes. Appl Environ Microbiol 61:1323–1330.[Abstract]
Hansford CG. 1954. Australian fungi II. New records and revisions. Proc Linn Soc NSW 79:97–144.
Hartill WFT. 1991. Postharvest diseases of avocado fruit in New Zealand. NZ J Crop Hort Sci 19:297–304.
Hillis DM, Huelsenbeck JP. 1992. Signal, noise, and reliability in molecular phylogenetic analyses. J Hered 83: 189–195.
Huelsenbeck JP, Bull JJ, Cunningham CW. 1996. Combining data in phylogenetic analysis. TREE 11:152–158.
Jacobs R. 2002. Characterization of Botryosphaeria species from mango in South Africa [Master’s thesis]. Pretoria, South Africa: University of Pretoria. 162 p.
Jacobs KA, Rehner SA. 1998. Comparison of cultural and morphological characters and ITS sequences in anamorphs of Botryosphaeria and related taxa. Mycologia 90:601–610.
Palm ME. 1999. Mycology and world trade: a view from the front line. Mycologia 91:1–12.
Pennycook SR, Samuels GJ. 1985. Botryosphaeria and Fusicoccum species associated with ripe fruit rot of Actinidia deliciosa (Kiwifruit) in New Zealand. Mycotaxon 24: 445–458.
Phillips AJL, Fonseca F, Povoa V, Castilho R, Nolasco G. 2002. A reassessment of the anamorphic fungus Fusicoccum luteum and description of its teleomorph Botryosphaeria lutea sp. nov. Sydowia 54:59–77.
Punithalingam E, Holliday P. 1973. Botryosphaeria ribis. CMI descriptions of pathogenic fungi and bacteria, No. 395. Kew, Surrey, England: Commonwealth Mycological Institute. 2 p.
Punithalingam E, Waller JM. 1973. Botryosphaeria obtusa. CMI descriptions of pathogenic fungi and bacteria, No. 394. Kew, Surrey, England: Commonwealth Mycological Institute. 2 p.
Raeder U, Broda P. 1985. Rapid preparation of DNA from filamentous fungi. Lett Appl Microbiol 1:17–20.
Rayner RW. 1970. A mycological colour chart. Kew, Surrey, UK: CMI and British Mycological Society. 34 p.
Roux J. 1998. Diseases of Acacia mearnsii in South Africa, with particular reference to Ceratocystis wilt [Doctoral thesis]. Pretoria, South Africa: University of Pretoria. 238 p.
———, Coutinho TA, Mujuni Byabashaija D, Wingfield MJ. 2001. Diseases of plantation Eucalyptus in Uganda. S Afr J Sci 97:16–18.
Saccardo PA. 1877. Fungi Veneti novi vel critici. Michelia 1: 1–72.
Scurfield G. 1966. The cankers of Acacia mucronata Willd. Ex H. Windl. Aust J Bot 14:293–302.
Shoemaker RA. 1964. Conidial states of some Botryosphaeria species on Vitis and Quercus. Can J Bot 42:1297–1301.
Slippers B, Crous PW, Denman S, Coutinho TA, Wingfield BD, Wingfield MJ. 2003. Combined multiple gene genealogies and phenotypic characters differentiate several species previously identified as Botryosphaeria dothidea. Mycologia 96:83–101.
Smith H, Wingfield MJ, Crous PW, Coutinho TA. 1996. Sphaeropsis sapinea and Botryosphaeria dothidea endophytic in Pinus spp. and Eucalyptus spp. in South Africa. S Afr J Bot 62:86–88.
———, Crous PW, Wingfield MJ, Coutinho TA, Wingfield BD. 2001. Botryosphaeria eucalyptorum sp. nov., a new species in the B. dothidea-complex on Eucalyptus in South Africa. Mycologia 93:277–284.
Smith DR, Stanosz GR. 2001. Molecular and morphological differentiation of Botryosphaeria dothidea (anamorph Fusicoccum aesculi) from some other fungi with Fusicoccum anamorphs. Mycologia 93:505–515.
Stevens NE, Jenkins AE. 1924. Occurrence of the current cane blight fungus on other hosts. J Agric Res 27:837–844.
Swofford DL. 1999. PAUP*. Phylogenetic analysis using parsimony (*and other methods). Version 4. Sunderland, Massachusetts: Sinauer Associates.
Taylor JW, Jacobson DJ, Kroken S, Kasuga T, Geiser DM, Hibbett DS, Fisher MC. 2000. Phylogenetic species recognition and species concepts in fungi. Fungal Genet Biol 31:21–32.[Medline]
Trotter A. 1928. Sylloge fungorum omnium hucusque cognitorum 24(2):810–815.
von Arx JA, Müller E. 1954. Die Gattungen der amerosporen Pyrenomyceten. Beitr Kryptogamenfl Schweiz 11, 2:1–434.
White TJ, Bruns T, Lee S, Taylor J. 1990. Amplification and direct sequencing of fungal ribosomal RNA genes for phylogenetics. In: Innis MA, Gelfand DH, Snisky JJ, White TJ, eds. PCR protocols: a guide to methods and applications. San Diego: Academic Press. p 315–322.
Wingfield MJ, Slippers B, Roux J, Wingfield BD. 2001a. Worldwide movement of exotic forest fungi, especially in the tropics and the southern hemisphere. BioScience 51:134–140.
———, Roux J, Coutinho T, Govender P, Wingfield BD. 2001b. Plantation disease and pest management in the next century. S Afr For J 190:67–71.
Witcher W, Clayton CN. 1963. Blueberry stem blight caused by Botryosphaeria dothidea (B. ribis). Phytopathology 42:521–525.
Zhou S, Smith DR, Stanosz GR. 2001. Differentiation of Botryosphaeria species and related anamorphic fungi using Inter Simple or Short Sequence Repeat (ISSR) fingerprinting. Mycol Res 105:919–926.
———, Stanosz GR. 2001a. Relationships among Botryosphaeria species and associated anamorphic fungi inferred from the analyses of ITS and 5.8S rDNA sequences. Mycologia 93:516–527.
———, ———. 2001b. Primers for amplification of mt SSU rDNA, and a phylogenetic study of Botryosphaeria and associated anamorphic fungi. Mycol Res 105:1033–1044.
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