Ectomycorrhizal fungal communities of secondary tropical forests dominated by Tristaniopsis in Bangka Island, Indonesia
Helbert aff001; Maman Turjaman aff002; Kazuhide Nara aff001
Authors place of work:
Department of Natural Environmental Studies, The University of Tokyo, Kashiwa, Chiba, Japan
aff001; Forest Research and Development Centre (FRDC), Environment and Forestry Research, Development, Innovation Agency (FORDA), the Ministry of Environment and Forestry, Bogor, Indonesia
Published in the journal:
PLoS ONE 14(9)
In Southeast Asia, primary tropical rainforests are usually dominated by ectomycorrhizal (ECM) trees belonging to Dipterocarpaceae, although arbuscular mycorrhizal trees often outcompete them after disturbances such as forest fires and clear-cutting, thus preventing dipterocarp regeneration. In some secondary tropical forests, however, potentially ECM trees belonging to Tristaniopsis (Myrtaceae) become dominant and may help ECM dipterocarp forests to recover. However, we have no information about their mycorrhizal status in these settings. In this study, we analyzed ECM fungal communities in tropical secondary forests dominated by Tristaniopsis and investigated which ECM fungal species are shared with other tropical or temperate areas. In total, 100 samples were collected from four secondary forests dominated by Tristaniopsis on Bangka Island. ECM tips in the soil samples were subjected to molecular analyses to identify both ECM and host species. Based on a >97% ITS sequence similarity threshold, we identified 56 ECM fungal species dominated by Thelephoraceae, Russulaceae, and Clavulinaceae. Some of the ECM fungal species were shared between dominant Tristaniopsis and coexisting Eucalyptus or Quercus trees, including 5 common to ECM fungi recorded in a primary mixed dipterocarp forest at Lambir Hill, Malaysia. In contrast, no ECM fungal species were shared with other geographical regions, even with Tristaniopsis in New Caledonia. These results imply that secondary tropical forests dominated by Tristaniopsis harbor diverse ECM fungi, including those that inhabit primary dipterocarp forests in the same geographical region. They may function as refugia for ECM fungi, given that dipterocarp forests are disappearing quickly due to human activity.
Tropical forests account for approximately 44% of the world’s forest coverage. However, from 2000 to 2010, there was a net forest loss of 7 million hectares per year in tropical countries, mainly due to large-scale commercial agriculture. These dramatic losses and changes in tropical forests are becoming a serious threat to biodiversity, given that tropical rainforests sustain the largest number of species in the world.
Dominant trees in many forest ecosystems are associated with ectomycorrhizal (ECM) fungi and depend on them for soil nutrients, which they exchange for photosynthesis products[3,4]. Thus, ECM symbiosis is regarded as a prerequisite for host tree growth and survival in nature. In fact, the availability of ECM fungi and their composition could be the most significant determinant of seedling establishment in heavily disturbed areas. Therefore, ECM fungal communities have been studied repeatedly in disturbed areas under boreal, temperate, and subtropical climates. However, no previous studies documented ECM fungal communities in heavily disturbed tropical areas.
Available data of ECM fungi in Southeast Asia are mostly from undisturbed Dipterocarpaceae forests[10–13], largely because this dominant ECM host is often replaced by fast growing arbuscular mycorrhizal trees, such as Macaranga and Mallotus after disturbance, [14,15]. However, in some parts of Southeast Asia[16,17], potentially ECM trees belonging to Myrtaceae become dominant in disturbed sites, although we know nothing about their ECM colonization and ECM fungal communities.
Myrtaceae includes both arbuscular mycorrhizal and ECM lineages. The latter includes Eucalyptus, on which ECM fungi have been documented in native areas like Australia and in some areas to which they have been introduced, such as the Seychelles and Africa. Tristaniopsis is another ECM lineage in Myrtaceae, distributed in Cambodia, Myanmar, the Peninsula of Malaysia, Borneo, Java, Sumatra, and Australia. Waseem et al. (2017) recently reported ECM fungi associated with endemic Tristaniopsis species in New Caledonia. Some other Tristaniopsis species appear in secondary forests in Southeast Asia, where biogeographical, climate, and ecological conditions are fundamentally different from New Caledonia. We do not know whether Tristaniopsis trees are colonized by ECM fungi in these settings, and if colonized, what types of ECM fungal communities are present.
In this study, we investigated the ECM fungal communities of four secondary tropical forests dominated by Tristaniopsis on Bangka Island, Indonesia. Our objectives were (1) to confirm the ECM colonization of Tristaniopsis under secondary tropical forest settings, (2) to characterize ECM fungal diversity and species composition, and (3) to clarify how many fungal species are shared with known fungi on Tristaniopsis in New Caledonia and with fungi from other tropical or temperate areas. The knowledge obtained from this study will broaden our understanding of tropical ECM fungal ecology and biogeography, with implications for the regeneration of ECM forests in the tropics.
Materials and methods
Bangka Island is located off the eastern coast of Sumatra Island, across the Bangka Strait. Four secondary forests with various disturbance types were selected: Kelapa (site 1), Limbung (site 2), Namang (site 3), and Sungai Selan (site 4), as shown in Table 1 and S1 Fig. All of these forests are dominated by Tristaniopsis, coexisting with other pioneer tree species. The sampling areas varied from 0.5 to 1.8 ha, depending on the remaining forest area. The average annual precipitation on this island is 2426 mm, most of which falls in the rainy season from July to December. The average monthly temperature on this island is 27.21 ± 0.43°C, representing a typical tropical climate with little seasonal temperature variation.
No specific permission was required to access all sampling locations. Kelapa. Limbung and Sungai Kelan are village forests which belong to the local people. We met the village heads, and they guided us to sampling location. Namang is an EcoEduTourism forest. Since this is educational forests, we didn't need any specific permission to access and do sampling activities. This field study did not involve any endangered or protected species.
Twenty-five soil samples (of dimensions 5 x 5 x 10 cm) were randomly collected from each sampling site in April 2015. Each sampling point was selected near a selected Tristaniopsis tree, which was >5 m away from other selected trees. The geographical positions of individual sampling points were recorded using GPS (GPSMAP62SJ, Garmin, Olathe, KS, USA). Soil samples were placed separately in plastic bags and stored at ambient temperature and processed within six days. Some leaves and flowers from Tristaniopsis trees were collected from the sampling sites to obtain reference DNA for host identification.
Identification of ectomycorrhizal fungi
All ECM roots were carefully separated from each soil sample and cleaned in tap water. The cleaned ECM root tips were examined under a stereomicroscope (SZ61, Olympus Co., Tokyo, Japan) and grouped into morphotypes based on their morphological characteristics, including surface texture, mantle color, emanating hyphae, and rhizomorphs. Whenever available, three ECM root tips were sampled from each morphotype per soil sample and placed into separate 2.0-ml tubes for DNA extraction. Morphotyping was completed within 6 days of soil sampling.
DNA extraction and molecular analysis were carried out following Murata et al. (2013), with minor modification. Briefly, total DNA was extracted using the cetyltrimethyl ammonium bromide (CTAB) method. Internal transcribed spacer (ITS) regions (including ITS1, 5.8S, ITS2) of nuclear ribosomal DNA were amplified by polymerase chain reaction (PCR) with the ITS1F and ITS4 primers combination (S1 Table). For unsuccessfully amplified samples, other forward (ITS5 or ITS0FT) and reverse (LBW, LAW, or ITS4CG) primerswere used. A Platinum® Multiplex PCR Master Mix (Applied Biosystems, Foster City, CA, USA) was used for PCR. Successfully amplified PCR products were purified and subjected to Sanger sequencing reaction using BigDye Terminator Cycle Sequencing Kit (Applied Biosystem) with ITS1 as the sequence primer or ITS4 for poorly sequenced samples. Sequencing was performed on ABI 3730xl (Applied Biosystems).
All of the obtained sequences were verified against their original chromatograms, manually corrected, and grouped into molecular operational taxonomic units (hereafter referred to as ‘species’ for simplicity, following the practice in this field) based on sequence similarities greater than 97%, which we calculated using ATGC software (ver. 7.0; GENETYX Corp., Tokyo, Japan). Fungal identity was assigned based on BLAST search results against known taxa in the international sequence databases. Non-ECM sequence results were excluded from subsequent analysis.
The host associated with each ECM root tip was determined based on sequences in plastid trnL or rbcL regions of chloroplast DNA. Primers trnC (5′-cgaaatcggtagacgctacg-3′) or rbcla-F (5′-atgtcaccacaaacagagactaaagc-3′), in combination with trnD (5′-ggggatagagggacttgaac-3′) or rbcla-R (5′-gtaaaatcaagtccaccrcg-3′), were used for PCR amplification. All of the amplicons were purified and sequenced using trnC or rbcla-F as the sequencing primer. The sequences obtained from Tristaniopsis leaves were used as references.
The frequency of each ECM species was defined as the number of soil samples containing that species. The species richness of ECM fungi at all sampling sites was estimated using EstimateS software ver. 9, and Jackknife2 with 1000 randomizations was used. The similarities between the ECM fungal communities of different sampling sites were visualized using a non-metric dimensional scaling (NMDS) procedure implemented in the ‘vegan’ package of R software ver. 3.3.1 with the Bray–Curtis distance and 999 permutations. The statistical differences between the ECM fungal community compositions of the sampling sites were evaluated using the Adonis (permutation multivariate analysis of variance) function of the ‘vegan’ package, using the Bray–Curtis distance and 999 permutations. The Betadisper test (Permutational analysis of multivariate dispersions) in ‘vegan’ was also used to determine the data dispersions of the communities between groups.
To evaluate how many ECM fungal species were shared with those found on Tristaniopsis in New Caledonia, our ITS sequences were compared with those in Waseem et al. (2017). If the similarity was >97% in a pairwise comparison between the two regions, we regarded it as the same species and as shared between the regions. To determine whether the fungal species found in this study had already been recorded in other geographical regions, a BLAST search was carried out against sequences deposited in the International Nucleotide Sequence Database (INSD). If BLAST matches showed similarities >97%, we derived their geographical positions from the metadata of the matched sequences.
Of the 100 soil samples collected from the four sites, 43 contained Tristaniopsis ECM roots. Quercus and Eucalyptus were confirmed in 4 and 3 soil samples, respectively. As a minor host, Shorea was detected only once. Thirty soil samples did not contain ECM root-tips. In terms of ECM root abundance, Tristaniopsis was dominant, accounting for 77.3% of ECM roots examined.
In total, we identified 56 ECM fungal species (accession number LC483889 –LC483944), of which 36 species were collected from Tristaniopsis roots (S2 Table). Quercus and Eucalyptus were associated with 4 ECM fungal species. Of the 36 species identified on Tristaniopsis, 2 species each were shared with Quercus and Eucalyptus. These shared species were found relatively frequently in the forests. An average of 1.77 (excluding null samples) ECM fungal species were detected per soil sample, with a maximum of 4 species.
The Jack2 richness estimator indicated that at least 129 ECM fungal species would inhabit these forests, and for Tristaniopsis alone, 82 species were expected. The observed ECM fungal richness (and Jack2 estimates) at Kelapa, Limbung, Namang, and Sungai Kelan were 19 (41), 25 (60), 15 (36), and 9 (22), respectively. The species accumulation curves for all hosts and for Tristaniopsis did not approach the asymptote at our maximum sampling effort, indicating that additional species will be found with greater sampling effort (Fig 1). The diversity parameters are summarized in Table 2.
ECM fungal communities were dominated by a few species. Only 3 ECM fungal species were identified in more than 5 soil samples. In contrast, 42 species were singletons. The frequencies of Cenococcum geophilum, Thelephoraceae sp.1, and Thelephoraceae sp.2 were high on Tristaniopsis roots, found in 15, 7, and 6 soil samples, respectively. Thelephoraceae (11 spp.) was the most species-rich ECM fungal lineage, followed by Russulaceae (6 spp.), Clavulinaceae (5 spp.), and Amanitaceae (4 spp.).
ECM fungal communities were not separated by sampling location (R2 = 0.55, P = 0.227). A Mantel test revealed that the geographic distance did not affect the structure of ECM communities (R = -0.24, α = 0.89).
Most ECM fungi detected in this study shared no similar sequence (>97%) records in INSD and Unite, indicating newly confirmed species. Only 6 of the 56 ECM fungi had matches with deposited sequences at >97% similarities. Five of these (Agaricomycetes sp1, Amanita sp3, Amanita sp4, Boletaceae sp1, and Cortinariaceae sp1) are likely to be the same species as found at Lambir Hill National Park, Sarawak. Another species matched the sequence of Heimioporus sp. sporocarp collected on Bangka Island (Accession no. KR061493). None of the ECM fungal species found in this study matched with sequences obtained from Tristaniopsis in New Caledonia. Although numerous ECM fungal sequences are available, none of them had ITS similarity to our sequences of >97%, except for the above-mentioned records in Southeast Asia.
In this study, we found 56 ECM fungal species in 100 soil samples (58 soil samples containing ECM roots) collected from four Tristaniopsis forests. The observed species richness is far lower than that of temperate forests, after being rarefied to the same sampling effort. ECM fungal richness is usually low in early successional stages, and increases with succession in temperate areas[8,28]. Although no previous studies have examined ECM fungal succession in the tropics, we may regard the lower richness as early successional ECM fungal communities affected by recent disturbance. Indeed, the diversity indices observed in this study were lower than other less-disturbed tropical forests documented in Borneo and Thailand, where the Simpson indices were 0.038 and 0.053, respectively. The lower observed diversity may also be explained in part by the global pattern of ECM fungal diversity, as tropical areas have inherently less diverse ECM fungi.
The ECM fungal communities did not vary significantly between sampling sites. This does not indicate that ECM fungal communities are less affected by geographical positions and environmental conditions (e.g., temperature, rainfall, and elevation), but rather indicates that such effects would be inconspicuous at our sampling scale, as all of the studied sites were located on the same small island, with little climate variation. No ECM fungi were shared with Tristaniopsis in New Caledonia. The geographic location and associated differences in environmental conditions may affect the ECM fungal composition, even associated with the same host genus, if we expand the geographical scale up to >6700 km, the distance between Bangka and New Caledonia. Bahram et al  showed tropical ECM fungal communities exhibited stronger distance-decay pattern.
There were no significant differences between the ECM fungal communities of co-existing host genera, partly because hosts other than Tristaniopsis were rare and were thus represented by fewer soil samples. However, two of the four ECM fungi found on Eucalyptus in this study were actually shared with Tristaniopsis, indicating their compatibility with both host genera. Because these two genera belong to the same family, Myrtaceae, they may be associated with similar ECM fungal communities in the same region. However, it would be premature to conclude this based on this study alone. It should also be noted that none of the Eucalyptus ECM fungi in other geographical regions matched our Tristaniopsis ECM fungi at the >97% sequence similarity threshold. In temperate areas, many ECM fungi were shared within the same host family, e.g. Pinaceae, across different continents, probably because of land bridges in ice ages. Biogeographical boundaries in the tropics (e.g., Wallace Line) remained disconnected even during ice ages[31,32], so the biogeographical effects of ECM fungal communities may be larger in the tropics than in temperate areas.
Five of the 56 ECM fungal species were recorded in a mixed dipterocarp forest at Lambir Hill, Sarawak, Malaysia, indicating their wide geographic distribution, with a range of at least 1100 km, but within the same biogeographical region, called Sundaland. Although the host species were not identified in Peay et al. (2010), it is likely that Dipterocarpaceae were the host, given the above-ground dominance of this tree group at Lambir Hill. Thus, the existence of the shared ECM fungi suggests their wide host range, including different host families. Indeed, two of the four ECM fungal species found on Quercus (Fagaceae) in this study were also found on Tristaniopsis (Myrtaceae). The ECM fungal sharing between the primary Lambir Hill forest and secondary Tristaniopsis forests implies that the pioneer Tristaniopsis trees could function as refugia for ECM fungi inhabiting dipterocarp forests. As ECM fungi on pioneer trees facilitate the establishment of successional ECM tree species in temperate regions, Tristaniopsis ECM fungi may help dipterocarp seedling establishment and forest recovery. It would be worth confirming this in future studies, given that dipterocarp forests have largely disappeared and there is currently no sign of recovery in many places in Southeast Asia.
Secondary tropical rainforests dominated by Tristaniopsis trees in Bangka island were found to harbor diverse ECM fungi, many of which were new species that were not identified in previous studies. None of the ECM fungi were shared with Tristaniopsis in New Caledonia. In contrast, some ECM fungi were shared between Tristaniopsis and other coexisting tree genera at the study sites, and five species were common to those detected in primary dipterocarp forests in the same biogeographic region. While many tropical rainforests become arbuscular mycorrhizal ecosystems after disturbance, secondary forests dominated by Tristaniopsis trees remain ECM ecosystems. Hence, they could function as refugia for ECM fungi that inhabit primary mixed dipterocarp forests in Southeast Asia.
S2 Table [docx]
Ectomycorrhizal fungi; their frequency and host identity confirm in secondary forests, Bangka, Indonesia.
1. FAO. State of the World’s Forests 2016. Forests and agriculture: land-use challenges and opportunities. Rome; 2016
2. Fitzherbert EB, Struebig MJ, Morel A, Danielsen F, Bruhl CA, Donald PF, et al. How will oil palm expansion affect biodiversity? Trends Ecol Evol. 2008;23(10): 538–545. doi: 10.1016/j.tree.2008.06.012 18775582
3. Perez-Moreno J, Read DJ. Mobilization and Transfer of Nutrients from Litter to Tree Seedlings via the Vegetative Mycelium of Ectomycorrhizal Plants. New Phytol. 2000;145(2): 301–309.
4. Rousseau JVD, Sylvia DM, Fox AJ. Contribution of ectomycorrhiza to the potential nutrient-absorbing surface of pine. New Phytol. 1994;128(4): 639–644.
5. Smith SE, Read DJ. Mycorrhizal Symbiosis 3rd ed. Academic press; 2008.
6. Nara K. Ectomycorrhizal networks and seedling establishment during early primary succession. New Phytol. 2006;169(1):169–178. doi: 10.1111/j.1469-8137.2005.01545.x 16390428
7. Qu L, Makoto K, Choi DS, Quoreshi AM, Koike T. The Role of Ectomycorrhiza in Boreal Forest Ecosystem. In: Osawa A, Zyryanova O, Matsuura Y, Kajimoto T, Wein R, editors. Permafrost Ecosystems: Ecological Studies (Analysis and Synthesis), vol 209. Dordrecht: Springer; 2010 pp. 413–425.
9. Toju H, Sato H, Tanabe AS. Diversity and Spatial Structure of Belowground Plant–Fungal Symbiosis in a Mixed Subtropical Forest of Ectomycorrhizal and Arbuscular Mycorrhizal Plants. PLoS One. 2014;9(1): e86566. doi: 10.1371/journal.pone.0086566 24489745
10. Henkel TW, Terborgh J, Vilgalys RJ. Ectomycorrhizal fungi and their leguminous hosts in the Pakaraima Mountains of Guyana. Mycol Res. 2002;106(May):515–531.
11. Sirikantaramas S, Sugioka N, Lee SS, Mohamed LA, Lee HS, Szmidt AE, et al. Molecular identification of ectomycorrhizal fungi associated with Dipterocarpaceae. Tropics. 2003;13(2): 69–77.
12. Peay KG, Kennedy PG, Davies SJ, Tan S, Bruns TD. Potential link between plant and fungal distributions in a dipterocarp rainforest: community and phylogenetic structure of tropical ectomycorrhizal fungi across a plant and soil ecotone. New Phytol. 2010;185(2): 529–42. doi: 10.1111/j.1469-8137.2009.03075.x 19878464
13. Phosri C, Põlme S, Taylor AFS, Kõljalg U, Suwannasai N, Tedersoo L. Diversity and community composition of ectomycorrhizal fungi in a dry deciduous dipterocarp forest in Thailand. Biodivers Conserv. 2012;21(9): 2287–2298.
14. Ferry Slik JW, Keßler PJA, van Welzen PC. Macaranga and Mallotus species (Euphorbiaceae) as indicators for disturbance in the mixed lowland dipterocarp forest of East Kalimantan (Indonesia). Ecol Indic. 2003;2(4): 311–324.
15. Brearley FQ, Prajadinata S, Kidd PS, Proctor J, Suriantata. Structure and floristics of an old secondary rain forest in Central Kalimantan, Indonesia, and a comparison with adjacent primary forest. For Ecol Manage. 2004;195(3): 385–397.
16. Nurtjahya E, Setiadi D, Guhardja E, Muhadiono, Setiadi Y. Succession on tin-mined land in Bangka Island. Blumea. 2009;54(1–3): 131–138.
17. Fukushima M, Kanzaki M, Hara M, Ohkubo T, Preechapanya P, Choocharoen C. Secondary forest succession after the cessation of swidden cultivation in the montane forest area in Northern Thailand. For Ecol Manage. 2008;255(5–6):1994–2006.
18. Adams F, Reddell P, Webb MJ, Shipton WA. Arbuscular mycorrhizas and ectomycorrhizas on Eucalyptus grandis (Myrtaceae) trees and seedlings in native forests of tropical north-eastern Australia. Aust J Bot. 2006;54(3):271–281.
19. Tedersoo L, Suvi T, Beaver K, Kõljalg U. Ectomycorrhizal fungi of the Seychelles: Diversity patterns and host shifts from the native Vateriopsis seychellarum (Dipterocarpaceae) and Intsia bijuga (Caesalpiniaceae) to the introduced Eucalyptus robusta (Myrtaceae), but not Pinus caribea (Pinaceae). New Phytol. 2007;175(2): 321–333. doi: 10.1111/j.1469-8137.2007.02104.x 17587380
20. Ducousso M, Duponnois R, Thoen D, Prin Y. Diversity of Ectomycorrhizal Fungi Associated with Eucalyptus in Africa and Madagascar. Int J For Res. 2012;2012: 1–10.
21. Govaerts R, Sobral M, Ashton P, Barrie F, Holst B, Landrum L, et al. World Checklist of Myrtaceae;2019. Available from: http://wcsp.science.kew.org/.
22. Waseem M, Ducousso M, Prin Y, Domergue O, Hannibal L, Majorel C, et al. Ectomycorrhizal fungal diversity associated with endemic Tristaniopsis spp. (Myrtaceae) in ultramafic and volcano-sedimentary soils in New Caledonia. Mycorrhiza; 2017;27(4): 407–413. doi: 10.1007/s00572-017-0761-4 28091750
23. Agerer R. Exploration types of ectomycorrhizae: A proposal to classify ectomycorrhizal mycelial systems according to their patterns of differentiation and putative ecological importance. Mycorrhiza. 2001;11(2): 107–114.
24. Murata M, Kinoshita A, Nara K. Revisiting the host effect on ectomycorrhizal fungal communities: Implications from host-fungal associations in relict Pseudotsuga japonica forests. Mycorrhiza; 2013: 641–653. doi: 10.1007/s00572-013-0504-0 23702643
25. Colwell R. EstimateS: Biodiversity Estimation. Diversity. 2009: 1–23. Available from: http://viceroy.eeb.uconn.edu/estimates
26. R Development Core Team R. R: A Language and Environment for Statistical Computing. R Foundation for Statistical Computing. R Foundation for Statistical Computing; 2011: 409. Available from: http://www.r-project.org
27. Tedersoo L, Nara K. General latitudinal gradient of biodiversity is reversed in ectomycorrhizal fungi. New Phytol. 2010;185(2): 351–354. Available from: doi: 10.1111/j.1469-8137.2009.03134.x 20088976
28. Nara K, Nakaya H, Wu B, Zhou Z, Hogetsu T. Underground primary succession of ectomycorrhizal fungi in a volcanic desert on Mount Fuji. New Phytol. 2003;159(3): 743–756.
29. Bahram M, Kõljalg U, Courty P-E, Diédhiou AG, Kjøller R, Põlme S, et al. The distance decay of similarity in communities of ectomycorrhizal fungi in different ecosystems and scales. J Ecol. 2013;101(5):1335–1344.
30. Miyamoto Y, Narimatsu M, Nara K. Effects of climate, distance, and a geographic barrier on ectomycorrhizal fugal communities in Japan: A comparison across Blakiston’s Line. Fungal Ecol. 2018;33: 125–133.
31. Bird MI, Taylor D, Hunt C. Palaeoenvironments of insular Southeast Asia during the Last Glacial Period: A savanna corridor in Sundaland? Quat Sci Rev. 2005;24(20–21): 2228–2242.
32. Cannon CH, Manos PS. Phylogeography of the Southeast Asian stone oaks (Lithocarpus). J Biogeogr. 2003;30(3): 211–226.