1. Introduction
Fungus-growing termites (Macrotermitinae) are important keystone species in the Asian and African tropics, where they have a great impact on the decomposition of dead plant material [1] [2] . These termites cultivate species of the mutualistic basidiomycete genus Termitomyces. The fungi, which grow in association with termites and their nests, rely on the organic substances obtained by the insects when they feed on dead plant material [3] . Grasse’ [4] first described Termitomyces as being associated with a single family of termites. Now over 330 species of fungus-growing termites in 11 genera are known [5] , and 30 species of Termitomyces have been described [6] . Of these, 12 species of Termitomyces have been found in Southeast Asia [7] . Elucidating the taxonomy of these fungi is a difficult process [8] , and it is likely that more species exist but have yet to be discovered.
The ectosymbiosis between termites and Termitomyces greatly affects the physical and chemical properties of the soil and its related microbial communities. Termitomyces is cultivated on a special substrate inside the termite nest or dispersed in the soil called the fungal comb or fungal garden [9] -[11] . Like fungus-growing ants and beetles, fungus-growing termites develop an “agricultural” mutualism by growing fungi for food [11] . The fungal combs are built with partially digested vegetal material and managed by termites to support the growth of Termitomyces and to prevent the combs’ colonization by competitive fungi.
Classification of Termitomyces species based on morphological and physiological characteristics is very difficult [12] . Often, the morphological characteristics do not distinguish different species of fungus [13] . Moreover, sexual characteristics generally are not useful for classification because approximately 20% of fungal species are considered to be asexual, and those that can reproduce sexually do not do so regularly [14] . Some Termitomyces species also mainly reproduce asexually and those fruiting bodies are rarely seen for some species [15] . The inoculation of the fungus comb in newly founded of some species colonies of the Macrotermitinae (Isoptera) from Nigeria [16] [17] . Therefore, molecular techniques are required to provide quantitative data to understand the specificity of the association between particular fungus species and termites.
Ribosomal DNA (rDNA) sequences can be used for taxonomic and phylogenetic analyses to study relationships among species. The internal transcribed spacer (ITS) is a component of the rDNA repeat, which consists of 18S, ITS1, 5.8S, ITS2, and 28S genes. Ribosomal genes and spacers always occur in tandem repeats that are thousands of copies long, each separated by what is termed an intergenic spacer (IGS) or non-transcribed spacer (NTS). Each repeat is composed of a transcription unit that codes for three rRNAs: a small subunit (SSU), a large subunit (LSU), and 5.8S. ITS1 is a noncoding region located in rDNA between the 18S and 5.8S rRNA genes, whereas ITS2 is located between the 5.8S and 28S rRNA genes [18] [19] . Among the regions of the ribosomal cistron, the ITS regions have the highest probability of successful identification for the broadest range of fungi, with the most clearly defined barcode gap between inter- and intra-specific variation [20] . ITS2 is more useful for molecular systematics at the species level. Variation among individual rDNA repeats can be observed within both the ITS and IGS regions [17] . As the ITS sequences show more divergence than their flanking coding regions (5.8S rDNA, and also 18S and 28S) and are easily amplified, they are routinely used to distinguish related species and to infer phylogenetic relationships among populations [21] . The aim of the present study was to confirm the identity of a Termitomyces species from Malaysia resembling T. aurantiacus.
2. Materials and Methods
2.1. Sample Collection
Four different fruiting body of termite were collected from an oil palm plantation located in the Seriserdang area during the months of July and August, 2008 (Table 1). The outermost layer of each fungus comb was peeled off and cut into 3 mm long segments. The segments were surface-sterilized in 70% ethanol followed by 0.05% sodium hypochlorite (or 5% Clorox® bleaching agent) for 1 - 2 min, rinsed with sterile distilled water, and blotted dry on sterilized Whatmann no. 17 filter papers. All segments were placed on a potato dextrose agar (PDA) (Difco; USA) plate and incubated for 6 days under ambient laboratory conditions (28˚C ± 2˚C, 12 h light and 12 h darkness). All subculturing of these isolates was performed using PDA that was prepared by adding 500 ml of distilled water sterilized at 121˚C for 15 min to 19 g of PDA. After the incubation period, fungus colonies could be seen as small whitish spots. Stock cultures were stored on agar slopes in 20 ml universal bottles maintained at 10˚C - 15˚C until used for further analysis.
2.2. Liquid Culture of Isolates
Fungus isolates from each of the four termite mounds were cultured in potato dextrose broth (PDB) (Difco) that was prepared according to the manufacturer’s specifications [10] . Aliquots of 100 ml of medium were decanted
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Table 1. Isolates of Termitomyces aurantiacus analyzed in this study.
into individual 250 ml Erlenmeyer flasks with cotton wool stoppers placed over the flask mouths and then autoclaved at 121˚C for 15 min. When cooled, each flask was aseptically inoculated with five agar disc pure cultures of fungi cut from actively growing hyphal tips using a 5 mm diameter cork borer. Once inoculated, the cotton wool stoppers were replaced with aluminum foil and the flasks were sealed with parafilm during the growth phase as static cultures under room temperature conditions (28˚C ± 2˚C; 12 h darkness and 12 h light). The flasks were maintained as still cultures for 10 days under ambient laboratory conditions. The mycelia mats were harvested by filtration through a double-layered muslin cloth and washed several times with sterile distilled water. The mycelia mats from each of the isolates were then transferred into individual plastic bags (with excess liquid squeezed out), labeled, and deep frozen overnight at ?20˚C. The frozen mycelia mats were immediately ground in a mortar and pestle swabbed with ethanol prior to use. The slurry obtained was stored at ?20˚C or used immediately for DNA extraction.
2.3. DNA Extraction
The total fungal DNA was extracted using the phenol-chloroform method, as described in White et al. [22] . Approximately 50 mg of ground mycelium were added to 500 µl of extraction buffer (1 M Tris HCl [pH 8.5], 1 M NaCl [pH 8.5], 1 M EDTA [pH 8.0] and 10% sodium dodecyl sulphate). The reaction tubes were placed in a water bath for 8 h at 38˚C. After incubation, 350 µl of buffered phenol and 150 µl of chloroform were added and homogenously mixed for 10 min. The resulting suspension was centrifuged at 13,000 × g at 4 ˚C for 10 min. The upper aqueous layer was collected and transferred to a sterile centrifuge tube to which 3 µl of RNAse solution were added. This mixture was incubated at 38˚C in a water bath for 15 min. After incubation, an equal volume of chloroform was gently added to the sample and mixed for 10 min. The mixture was then centrifuged once more (13,000 × g for 10 min at 4˚C). The upper aqueous phase was again collected and transferred to a new tube. The DNA was precipitated with 250 µl of iso-propan-2-ol and kept overnight at ?20˚C. The next day the tube was centrifuged at 13,000 × g for 10 min at 4˚C. The resultant pellets were thoroughly washed twice with 500 µl of 70% ethanol, vacuum dried, and diluted in ddH2O. Finally, the DNA pellets were suspended in 50 µl of ddH2O and kept at ?20˚C. Next, the quality of the DNA samples was checked by performing gel electrophoresis on 1.5% agarose gel using a 50 bp (Promega, USA) ladder as a size standard. The electrophoresis was carried out in a 1 × TBE (0.045 M Tris-borate and 1 mM EDTA [pH 8.2]) running buffer at 70 V for 1 - 2 h. The gels were then stained with ethidium bromide (0.5 µl/ml) and visualized under UV light. The appearance of bands indicated the presence of a DNA template, which thereby allowed their use for polymerase chain reaction (PCR).
2.4. PCR Amplification of the ITS Regions of the rDNA
The universal forward primer ITS1 (5’ TCC GTA GGT GAA CCT GCG G 3’) and the reverse primer ITS4 (5’ TCC TCC GCT TAT TGA TAT GC 3’) were used for the amplification of the ITS1 and ITS2 regions of the rDNA [23] . The PCR amplifications were performed in a total reaction volume of 50 μl consisting of 50 ng genomic DNA, 10 mM dNTPs, 100 mM MgCl2, 5,000 units/ml of Taq DNA polymerase placed in a reaction buffer concentration of 10 × PCR buffer (200 mM Tris HCl, pH 8.4 and 500 mM KCl), and 1 µM primers of ITS1 and ITS4. The reactions were conducted in a Peltier Thermal Cycler-200 as follows: an initial denaturation for 5 min at 95˚C followed by 36 cycles of 1 min at 94˚C, annealing at 55˚C for 1 min, extension at 72˚C for 3 min, and a final extension at 72˚C for 10 min.
2.5. Gel Electrophoresis
The PCR products were run on a 1.5% agarose gel with a 100 bp (Promega) ladder as the size standard. Electrophoresis was performed in 1 × TBE running buffer (0.045 M Tris-borate and 1 mM EDTA, pH 8.2) at 70 V for 1 - 2 h. The gels were then stained with ethidium bromide (0.5 μl/ml). After 15 - 30 min the gels were visualized under UV light and photographed using an Alphamager® 2200 version 5.5 gel documentation systems.
2.6. DNA Sequencing and Alignment
The PCR products (50 µl) were purified using a commercial kit (QIAquick® PCR Purification Kit, Canada). The purified PCR products were sequenced using the BigDye Terminator v3.1 kit on an AB13130 DNA Sequencer (Applied Biosystems, USA). All of the sequence data were subjected to multiple alignments using the Bio-Edit Sequence Alignment Editor Software. Multiple sequence alignments were performed in NEXUS format using the default option in CLUSTAL-W software version 1.83 [24] in BioEdit Sequence Alignment Editor. The alignment was then optimized manually. Single gaps were treated as a fifth nucleotide (A, C, G, T, and gaps). Nucleotide sequences were subjected to GenBank searches to look for similar sequences. Isolate TA 004 sequences were submitted and deposited in a GenBank under accession number GU594650 for the ITS1 and ITS2 regions of the rDNA.
2.7. Phylogenetic Tree Analysis
Phylogenetic analyses were performed in MEGA6 software package [25] . The phylogenetic tree was reconstructed using the neighbor-joining (NJ) method of Saitou and Nei [26] . Bootstrap tests with 1,000 replications were conducted to examine the support of the interior branches and the validity of the phylogenetic analysis was obtained. Distance was defined as the probability of the nucleotide substitutions per site, based on the Kimura 2-parameter model (K2P) [27] .
3. Results
3.1. Morphology Observation
The colony growth rate of T. aurantiacus was 10 - 15 mm per day on PDA at room temperature. The colony was initially watery-white but turned a grayish slightly light white color in the centre of the Petri dish after 4 days of culture. When the colony fully covered the whole plate, it was grayish in color. By days 7 - 8, 50% - 60% of the colony was dark gray and the remaining 40% - 50% was dull gray (Figure 1) looking at the bottom of the dish, the colony was red in color (Figure 1).
The diameter of the pileus of the isolates was 5 - 8 cm. The pileus were convexo-mucronate with a pointed perforatorium, finally applanate with a recurved margin and the surface was rusty ochraceous to orange, the color was dark brown over the perforatorium, which was finely striated, somewhat scrobiculate towards the centre, and glabrous or with fine, and scattered velar remnants (Figure 2 and Figure 3, respectively). The stipe was a 6 - 8 × 0.7 - 1.0 cm long cylindrical solid with a white or whitish surface, and the annular zone was indistinct or absent. The pseudorhiza was 20 - 25 cm long and white in color.
3.2. Phylogenetic Analysis
The products of PCR amplification of the ITS 1-5.8S-ITS 2 regions of T. aurantiacus of TA008, TA004, TA010 and TA012 isolates were ~500 bp in length, as expected (Figure 4). Comparisons of the sequences were showed that the four fungus isolates from the fungus combs sampled from the four termite mounds were very similar. The DNA sequences of the ITS1-5.8S-ITS 2 regions of these four fungus isolates were showed more than 99% nucleotide identity to one another (Figure 5). Strains of TA008, TA004, TA010 and TA012 and ex-strains of GU594650 (Termitomyces aurantiacus strain TA 06; [28] , JN585945 (T. aurantiacus strain Cs/10/2; [29] ) JQ228252 (T. aurantiacus strain CB55; [30] ) were showed approximately 99% nucleotide identity to each other in Clade 1. Strains of 93073101 (EU179869; [31] ), 95060509 (EU179866; [32] ), XF1 (HQ435673; [33] ), XF15 (HQ435671; [33] ), 2735 (EU272539; [34] ) and XF10 (Xylaria; HQ435666; [33] ) were showed about 77% nucleotide identity to each other in Clade 2. The grouping of the data (Clades 1 and 2) was supported to different the grouping in the cases. These results suggested that the four isolates were Termitomyces-related basidiomy
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Figure 1. Seven days old colony of Termitomyces aurantiacus onto PDA media (left) and the reverse (right).
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Figure 2. T. aurantiacus attached to termite nest (left) and after collection (right).
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Figure 3. A schematic illustration of T. aurantiacus.
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Figure 4. Banding patterns produced of T. aurantiacus isolates by using the primer ITS-1 and ITS-4.
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Figure 5. Phylogenetic tree (neighbor-joining (NJ) is showing relationship of isolates with other related fungal species retrieved from GenBank based on their sequence of the ITS 1-5.8S-ITS 2 regions of the rDNA.
cetes and confirm that T. aurantiacus was the symbiont found growing on the fungus comb as fungus nodules. The phylogenetic tree analyses of the ITS1-5.8S-ITS2 regions found that all strains in clade 3 clustered with Tricholoma fulvocastaneum (T. fulvoca, DQ067895; [35] ), Lepista nebularis (Lnebular, DQ149728; [36] ), Termitomyces associated with Macrotermes subhylainus (GQ922686; [37] ), Termitomyces sp. (AF321369, AF321370 and AF321373; [11] ), and Termitomyces associated with Microtermes sp. (GQ922672 and GQ922676; [37] ) shown in Figure 4. This clustering was fully supported by the statistical analyses and showed 83% bootstrap values for the NJ method.
4. Discussion
Termites of the subfamily Macrotermitinae live in a mutualistic symbiosis with basidiomycete fungi of the genus Termitomyces. Termitomyces is commonly found in equatorial and southern Africa and in Southeast Asia. These genera are edible mushrooms, widely collected and traded in many countries of Southeast Asia [7] . It is closely related to Termitomyces striatus (Beeli) Heim, and is described from equatorial Africa as a variety of that species. Termitomyces aurantiacus is a familiar edible species in Thailand. In Africa, the symbotic association is with the termite, Pseudacanthotermes militaris Hagen [7] . Termites of subfamily Macrotermitinae cultivate the mycelium of basidiomycetes on comb-like structures made of small spheres of plant material quickly passed through the termite gut. The termites consumed small nodule that produced by the fungus, along with the degraded comb. This symbiotic association is quite similar to the protozoic endosymbionts of non-fungus growing termites [38] . Sometimes, frequently in correlation with rain seasons, the fungal mycelium of the termite combs produces mushrooms, which penetrate the termite nests and soil to spread their spores [8] .
Grassé [4] reported that every genus of fungus-growing termites is associated with a single species of Termitomyces that probably encompasses different morphospecies. Fifty years ago, Sands [39] reported some degree of specificity between termite genera and the associated fungal species. Heim [8] later suggested a strict system of one host and one fungal species. However, this premise was contradicted by other studies based on morphological characterizations of fungi, which suggested that certain fungi were shared by different termite host species and even genera [2] .
Classification of fungi based on the observation of various morphological features originally played a key role in providing putative species names, but accurate identification of species was very complicated, laborious, and subjective. Davet and Rouxel [40] noted that traditional identification methods could result in an overestimate of species, whereas those in the mycelial state or those with slow growth in culture were largely overlooked. In our opinion, the taxonomic classification of Termitomyces fungi still has limitations. Many species that appear to be similar under culture conditions and exhibit similar morphology are in fact completely different species. Processing of fungus cultures can be time consuming and laborious when a large number of isolates have to be handled, and the risk of culture contamination is always high, especially for the fast-growing fungi that overgrow the entire culture medium. As such, it is recommended that a multi-disciplinary approach be used for the accurate identification of Termitomyces species.
Molecular techniques allow the analysis of genetic markers and establish the identity of individuals as well as the taxonomic and phylogenetic relationships among individuals. The rDNA regions are commonly used for taxonomic and phylogenetic studies because they contain variable and conserved domains, which permit discrimination at the genus, species, and sub-species levels. The noncoding ITS1 and ITS2 regions in particular can be used for discrimination among closely related species within a fungal genus [12] .
The ITS 1 and 2 regions of the rDNA of isolates (TA004, TA008, TA010 and TA012) were successfully amplified by PCR with expected length of ~500 bp. Homology searching against GenBank revealed that these sequences were 100% similar with those of T. aurantiacus, and that none of the sequenced isolates belonged to the genus Xylaria. A phylogenetic relationship was established through alignment and cladistic analysis of homologous nucleotide sequences among these fungal species (Figure 5); the isolates were found to belong to the genus Termitomyces. According to this phylogenetic analysis, isolates were a species variant of T. aurantiacus.
The phylogenetic study showed the monophyletic tree from pure Malaysian Termitomyces isolates and mixture of Asia and African Termitomyces samples and suggested that both Asia and African Termitomyces species should have evolved from the same Clade 1 (Figure 5). The mutualistic symbiosis between fungus-growing termites and Termitomyces fungi originated in Africa and showed a moderate degree of interaction specificity. Approximately 30 species of Termitomyces from Africa and Asia have been described [6] . Osiemo et al. [41] combined available ITS sequence data from West, Central, and South Africa with data of 39 new samples from East Africa to achieve the most comprehensive view of the diversity and host specificity of Termitomyces symbionts across Africa. A high amount of sequence divergence in the ITS sequences is found; 11 different Termitomyces lineages in East Africa and >30 lineages across Africa are identified, and the expected diversity is estimated to be about 41 lineages.
Analysis of phylogenetic tree based on Xyleria ITS sequences are well-fitted in clade 2, with similarity boot strap value of 77%. Rogers et al. [42] reported that Xylaria-like fungi inhabited the fungus comb as mycelia. However, they never produce spores or stroma until the fungus comb is removed from the nest or termite abandon the nest. When fungus comb from a healthy nest incubates in the absence of termites, it is often covered by vigorous mycelium of Xylaria within a few days [43] [44] . Sannasi [45] described X. nigripes as the cultivated symbiont of Odontotermes redemanni, without mentioning Termitomyces. Visser et al. [46] reported that the identical ITS types occurred on fungus combs from different termite genera and species.
The above conclusion is that based on morphology and phylogeny, the identity of the species is T. aurantiacus. In conclusion, the above discussion strongly suggested that the combined morphology and phylogeny characters are undoubtedly useful for accurately identifications at the species level as a paradigm reference for further identification of T. aurantiacus species.
Acknowledgements
The authors acknowledge the valuable contributions of the late Prof. Dr. Faridah Abdullah. This work was supported by the Ministry of Science, Technology and Innovation Malaysia (MOSTI) under vote No. 01-02-04- 6020 EA001.
NOTES
*Corresponding author.