Understory Dwarf Bamboo Affects Microbial Community Structures and Soil Properties in a Betula ermanii Forest in Northern Japan

Abstract

In order to understand the relationships between understory bamboo and soil properties, we compared microbial community structures in the soil of a Betula ermanii boreal forest with Sasa kurilensis present and removed using high-throughput DNA sequencing. The presence of understory S. kurilensis strongly affected soil properties, including total carbon, total nitrogen, nitrate, and the C:N ratio as well as relative soil moisture. Marked differences were also noted in fungal and bacterial communities between plots. The relative abundance of the fungal phylum Ascomycota was 13.9% in the Sasa-intact plot and only 0.54% in the Sasa-removed plot. Among the Ascomycota fungi identified, the most prevalent were members of the family Pezizaceae. We found that the abundance of Pezizaceae, known to act as mycorrhizal fungi, was related to the amount of total carbon in the Sasa-intact plot. The relative abundance of Proteobacteria was significantly higher, whereas those of Planctomycetes and Actinobacteria were lower in the Sasa-intact plot than in the Sasa-removed plot. Furthermore, the results obtained suggest that some species of the phylum Planctomycetes are more likely to occur in the presence of S. kurilensis. Collectively, these results indicate that the presence of S. kurilensis affects microbial communities and soil properties in a B. ermanii boreal forest.

Understory dwarf bamboos (genus Sasa; clonal evergreen plants) are widely distributed in the boreal forests of northern Japan (19, 41, 44, 46). In heavy snowfall areas, dwarf bamboos may quickly cover forests, growing to 0.3–3 m in height with vigorously extending rhizomes (33, 40). Dense dwarf bamboo cover impacts the regeneration of tree species and affects tree seedling growth and establishment (22, 30). Since the mass of bamboo’s intertwining roots forms rhizomes underground, understory dwarf bamboo is considered to compete with overstory plants for soil nutrients and water (28, 32, 37). Previous studies demonstrated that Sasa senanensis (Franch. & Sav.) Rehder plays an important role in mitigating the loss of nitrogen and carbon from soil (13). The removal of Sasa spp. from a mixed boreal forest was previously shown to affect the dynamics of dissolved inorganic nitrogen in soil (35) and promote nitrogen leaching (12). Moreover, the removal of Sasa kurilensis (Rupr.) Makino & Shibata has been suggested to significantly increase the availability of soil water and enhance the growth of Betula ermanii Cham. trees (41). These findings indicate that understory Sasa sp. is closely linked to the properties of its surrounding soil.

In nutrient-poor ecosystems, soil microbes are crucial regulators of plant productivity (49). Variations in the structures of soil microbial communities are considered to be a major factor affecting litter decomposition rates (39). A methanotrophic bacterial community called the upland soil cluster alpha was found to have a close relationship with Sasa spp. in boreal forests (47). Moreover, Sasa spp. may be infected by witches’ broom disease through their fungal communities (31, 42). Species-species information on endophytic fungi in Sasa spp. has been expanded (29). However, the complexity of microbial communities in forest habitats makes it difficult to elucidate the species composition of soil microorganism communities under natural conditions. To date, the entire microbial community in the rhizosphere soil of Sasa spp. as a typical understory plant in boreal forests has not yet been investigated.

Rapid advances in molecular ecological approaches have made it possible to analyze whole microbial communities in a relatively short time. In particular, Illumina MiSeq has been widely used in many studies and has the advantage of allowing a higher sequencing depth than the 454 pyrosequencing technique (4, 38, 48). In the present study, we used Illumina MiSeq to analyze the microbial community structures of soils with or without understory S. kurilensis in a Betula ermanii stand and attempted to clarify the relationships between community structures and soil physicochemical properties. The main objectives of this study were to answer the following questions: (i) what are the structures of microbial communities in the presence and absence of S. kurilensis? and (ii) how are these structures related to soil physicochemical properties?

Materials and Methods

Study site and sample collection

This study was conducted in the Uryu Experiment Forest of Hokkaido University (44°23′N, 142°19′E) in northern Japan. The tree layer of the forest was exclusively dominated by the birch species, B. ermanii, and the forest floor was densely covered with S. kurilensis. Two plots of 20×30 m were established in this forest in 1998 (19, 41). S. kurilensis has been removed continuously since 1998 in one plot (Sasa-removed plot; SR) and left intact in the other plot (Sasa-intact plot; SI). The distance between the two plots was approximately 50 m.

Soil temperature and moisture were monitored using TOMST thermometers (TOMST Ltd., Prague, Czech Republic). Three temperature readings (air temperature at 10 cm above the soil surface, soil surface temperature, and 15-cm-deep soil temperature) and soil moisture were recorded every 15 min. A TOMST thermometer measuring system was set at the center of each circle (16, 18, 24).

Soil samples were collected 5 times during the growing season: on 23 July 2014, 1 October 2014, 3 June 2015, 4 August 2015, and 1 October 2015, by avoiding the snowy season. Three clods of soil (1,000 cm³) were randomly collected at a depth of 0–10 cm from each of the three fixed circles (10 m in diameter) on a diagonal line in the two plots (Fig. 1). In the SI plot, soil samples including S. kurilensis rhizomes were shaken vigorously to separate roots and soil not tightly adhering to roots. Soil samples of three replicates from each circle were mixed as one sample, packed in sterile plastic bags (Ziploc; SC Johnson Co., Racine, WI, USA), and transported to the laboratory in an ice-cooled box. After being sieved through a 2-mm screen, each soil sample was divided into three parts and stored in a −80°C refrigerator, a 4°C refrigerator, or a dry, room temperature location, respectively.

Fig. 1

Locations of three sampling circles used in both study plots (Sasa-intact and Sasa-removed).

Soil property analysis

Thirty soil samples (5 sampling dates×2 plots×3 circles) from the two plots were collected for soil property analysis. Soil pH was measured using a glass electrode after shaking with deionized water (1:2.5 soil: water ratio) for 1 h. Total nitrogen (TN) and total carbon (TC) contents in air-dried soil samples were measured using an automatic analyzer (C-N Corder; Yanaco, Kyoto, Japan). In order to measure inorganic nitrogen, fresh soil samples were mixed with deionized water (1:5 soil:water) for nitrate nitrogen (NO₃-N) and nitrite nitrogen (NO₂-N), and 2M KCl (1:10 soil:KCl) for ammonium nitrogen (NH₄-N). The concentrations of NO₃-N and NO₂-N were measured with ion chromatography (Dionex Model ICS-1100; Thermo Fisher Scientific, Waltham, MA, USA) and ammonium using the indo-phenol blue method (20).

DNA extraction and library preparation

A PowerSoil™ DNA Isolation Kit (MO BIO Laboratories, Solana Beach, CA, USA) was used to extract DNA from 0.25 g of fresh soil samples according to the manufacturer’s instructions. The genomic DNA standard of each sample was greater than 200 ng and the concentration of DNA was greater than 6 ng μL⁻¹ without degradation, after testing with a Beckman DU800 spectrophotometer (Beckman Coulter, Inc., Fullerton, CA, USA). DNA isolated from each sample was amplified using forward Bakt_341F (5′-CCTACGGGNGGCWGCAG-3′) and reverse Bakt_805R (5′-GACTACHVGGGTATCTAATCC-3′) primers for the V3-V4 region of the bacterial 16S rRNA gene (15). Forward ITS3 (5′-GCATCGATGAAGAACGCAGC-3′) and reverse ITS4 (5′-TCCTCCGCTTATTGATATGC-3′) primers were also used for fungal ITS genes (1).

Fifteen sequencing libraries were prepared per plot with the random fragmentation of DNA samples, followed by 5′ and 3′ adapter ligation. Adapter-ligated fragments were then used for PCR, and gel amplicons were purified according to the Illumina library preparation protocol. DNA sequencing was performed by Macrogen Inc. (Seoul, Korea) using the Illumina Miseq platform (San Diego, CA, USA) according to the manufacturer’s instructions.

Sequence process and statistical analyses

Raw data formatted as FASTQ were analyzed with FLASH version 1.2.11 to merge paired-end 300-bp reads from next-generation sequencing experiments (26). The CD-HIT-OTU program (http://weizhong-lab.ucsd.edu/cd-hit-otu/) was used to identify operational taxonomic units (OTUs) (25). Three-step clustering was performed with (1) raw read filtering and trimming; (2) error-free read selection; and (3) OTU clustering at distant cut-offs (0.03). The taxonomy assignment of bacterial and fungal sequences was based on the full alignments of 16S rRNA and ITS genes, respectively. Cluster sequences were uploaded to the Silva SSU database for 16S rRNA genes and the UNITE database for ITS genes. Quantitative insights into microbial ecology (QIIME) software version 1.9.1 were used to perform alpha diversity analyses (Chao1, Shannon Index, Simpson Index) on bacterial and fungal communities (3). Differences in the number of OTUs and alpha diversity estimates were tested using a one-way ANOVA, followed by Tukey’s honest significant difference test (HSD).

Significant differences in soil physicochemical properties between the SI and SR plots on the five sampling dates were tested using generalized linear mixed models, followed by Tukey’s HSD test. Generalized linear mixed models were also used to examine the relationships between the number of OTUs of microbial communities and soil physicochemical properties in the SI and SR plots. Differences between the relative abundance of microbial communities were tested with the Kruskal–Wallis method (21). All statistical calculations were performed in R version 3.2 (36). Values p<0.05 were considered to be significant. A redundancy analysis (RDA) is a constrained ordination technique that was used to test whether the occurrence of microbial communities matches specific environmental source profiles (8, 27), which was performed with abundance and environmental data using Canoco version 4.5 (43).

Results

Soil characteristics

Significant differences were observed in most of the physicochemical soil properties tested between the SI and SR plots. Soil moisture was markedly lower in the SI plot than in the SR plot (Fig. 2A). Although no significant difference was observed in soil temperatures (Fig. 2B) or pH, all other values were significantly different between the two plots (Fig. 3). Total carbon and the C:N ratio were higher in the SI plot than in the SR plot, while ammonium was lower, regardless of the sampling dates. The nitrate N concentration was significantly different between the SI and SR plots for all sampling dates, except 1 Oct 2014. Nitrite N was not detected (<1 mg NO₂-N kg⁻¹ soil) during the sampling period (data not shown).

Fig. 2

Monthly mean (A) soil moisture (squares) and (B) temperature (circles) of three sampling circles in Sasa-intact (filled) and Sasa-removed (open) plots between July 2014 and June 2015. T1: air temperature; T2: soil surface temperature; T3: 15-cm-deep soil temperature.

Fig. 3

Differences in soil physicochemical properties between Sasa-intact (gray) and Sasa-removed (white) plots according to a generalized linear mixed model. The superscript asterisk indicates significance at p<0.05. The response variable was the concentration of soil properties, the fixed effect was the two study plots, and the random effect was the five sampling dates. Mean values with different letters denote significant differences among the pooled data (i.e., data for five sampling dates for both plots) (p<0.05; Tukey’s HSD, n=9). TN: total nitrogen; TC: total carbon; NH₄-N: ammonium; NO₃-N: nitrate. Vertical lines indicate standard errors.

Abundance of 16S and ITS sequences

After multiple levels of quality control to filter the raw reads, we obtained an average of 26,665 sequences for the 16S rRNA genes and an average of 31,080 sequences for the ITS genes from all samples. All rarefaction curves were generated via CD-HIT-OTU using a 97% identity cut-off; coverage was more than 99% for all the samples. These results indicated that the volume of sequenced reads was reasonable and sufficient to evaluate the total number of OTUs (Fig. 4). Most bacterial samples were saturated at approximately 720–1,125 OTUs, whereas fungal samples were saturated at approximately 27–55 OTUs. Only the Shannon diversity index for alpha diversity estimates of microbial communities for 23 July 2014 was significantly different between the SI and SR plots (Table 1).

Fig. 4

Rarefaction curves for microbial OTUs in the three circles on five sampling dates, with clustering at a 97% rRNA sequence similarity. Solid and dashed lines represent the OTUs of the bacterial and fungal communities, respectively.

Table 1 Alpha diversity estimates of microbial communities in SI (Sasa-intact) and SR (Sasa-removed) plots for five sampling dates.

	Dates	Number of OTUsa		Chao1b		Shannonc		Simpsond		Coveragee
		SI plot	SR plot	SI plot	SR plot	SI plot	SR plot	SI plot	SR plot	SI plot	SR plot
Bacteria	23 Jul 2014	847 (64)	852 (15)	999 (52)	1071 (44)	7.6 (0.1)	7.2 (0.1)	0.99 (0)	0.98 (0)	0.99 (0)	0.99 (0)
	1 Oct 2014	960 (37)	863 (55)	1141 (42)	1021 (49)	7.6 (0.1)	7.5 (0.2)	0.99 (0)	0.99 (0)	0.99 (0)	0.99 (0)
	3 Jun 2015	935 (31)	955 (33)	1146 (37)	1138 (42)	7.8 (0)	7.8 (0.1)	0.99 (0)	0.99 (0)	0.99 (0)	0.99 (0)
	4 Aug 2015	919 (68)	962 (48)	1107 (90)	1155 (49)	7.7 (0.2)	7.7 (0.1)	0.99 (0)	0.99 (0)	0.99 (0)	0.99 (0)
	1 Oct 2015	1043 (43)	998 (22)	1207 (45)	1201 (45)	7.8 (0.1)	7.8 (0.1)	0.99 (0)	0.99 (0)	0.99 (0)	0.99 (0)
Fungi	23 Jul 2014	42 (1)	40 (7)	43 (2)	42 (7)	2.6 (0.4)	2.7 (0.2)	0.72 (0.06)	0.74 (0.02)	1 (0)	1 (0)
	1 Oct 2014	47 (2)	36 (4)	50 (2)	43 (6)	3.2 (0.1)	2.1 (0.7)	0.77 (0.04)	0.55 (0.14)	1 (0)	1 (0)
	3 Jun 2015	43 (5)	46 (5)	44 (6)	48 (6)	2.8 (0.4)	3.7 (0.3)	0.76 (0.07)	0.87 (0.03)	1 (0)	1 (0)
	4 Aug 2015	50 (5)	46 (4)	53 (5)	46 (5)	2.8 (03)	2.9 (0.7)	0.76 (0.06)	0.70 (0.16)	1 (0)	1 (0)
	1 Oct 2015	46 (2)	44 (4)	46 (2)	44 (5)	2.2 (0.1)	3.0 (0.5)	0.62 (0.01)	0.73 (0.13)	1 (0)	1 (0)

Values represent mean (SD) (n=3). Values in bold denote a significant difference between the SI (Sasa-intact) and SR (Sasa-removed) plots (p<0.05; one-way ANOVA), otherwise no significant difference.

^a  Species level, a 97% similarity threshold was used to define operational taxonomic units (OTUs).

^b  Chao1: Chao1 estimator with species richness.

^c  Shannon: Shannon Index.

^d  Simpson: Simpson Index.

^e  Coverage: Coverage C was calculated as C=1− (s/n), where s is the number of unique OTUs and n is the number of individuals in the sample.

Bacterial OTUs were assigned to 13 different phyla. Seven different phyla (Acidobacteria, Proteobacteria, Bacteroidetes, Verrucomicrobia, Firmicutes, Planctomycetes, and Actinobacteria) together comprised more than 90% of the relative abundance in every library (Fig. 5A). Since each of the six other phyla comprised <1% in both the SI and SR plots, they were excluded from further analyses. Proteobacteria (20.3% in the SI plot and 17.9% in the SR plot), Planctomycetes (4.99% and 5.71%), and Actinobacteria (3.43% and 4.01%) were tested using the non-parametric Kruskal–Wallis method, which revealed significant differences between the two plots. The other phyla were not significantly different between the plots: Acidobacteria (28.0% in the SI plot and 29.0% in the SR plot), Bacteroidetes (18.4% and 17.7%), Verrucomicrobia (10.8% and 11.2%), and Firmicutes (7.11% and 7.09%). The seven dominant phyla occurred in soil irrespective of the presence of S. kurilensis. Overall, the number of OTUs of fungal communities was fewer than those of bacterial communities.

Fig. 5

Differences in the relative abundance of soil microbial communities in Sasa-intact and Sasa-removed plots for five sampling dates according to a Kruskal–Wallis test. The asterisk indicates significance (p<0.05; n=15). (A) Bacterial phyla; (B) Fungal phyla; (C) Fungal classes.

Fungal sequences belonged to four different phyla: Ascomycota, Basidiomycota, Zygomycota, and Chytridiomycota (Fig. 5B). Basidiomycota had an average abundance of 64.9% in the SI plot and 67.8% in the SR plot over all the sampling dates. Zygomycota comprised 15.0% and 17.2% in the SI plot and SR plot, respectively. Chytridiomycota was excluded from further analyses because abundance was <1% in both plots. Notably, Ascomycota had a very different abundance between the two plots, making up 13.9% of the SI plot, but only 0.54% of the SR plot. The relative abundance of the fungal class Pezizomycetes (phylum Ascomycota) in the SI plot was greater than that in the SR plot (Fig. 5C), while Tremellomycetes (phylum Basidiomycota) was less abundant in the SI plot than in the SR plot for all sampling dates. Most of the abundances in the phyla Ascomycota and Basidiomycota were attributed to the family Pezizaceae and genus Cryptococcus, respectively (Table 2).

Table 2 Percentage (%) of sequences classified for two fungal classes, Pezizomycetes and Tremellomycetes, in SI (Sasa-intact) and SR (Sasa-removed) plots for five sampling dates.

Dates		SI plot					SR plot
		23 Jul 2014	1 Oct 2014	3 Jun 2015	4 Aug 2015	1 Oct 2015	23 Jul 2014	1 Oct 2014	3 Jun 2015	4 Aug 2015	1 Oct 2015
Class	Pezizomycetes
Order	Pezizales	100	100	100	100	100	100	100	100	100	100
Family	Pezizaceae	100	100	100	100	100	100	100	100	100	100
Class	Tremellomycetes
Order	Filobasidiales	100	100	100	98	100	99	100	99	98	99
	Tremellales	0	0	0	2	0	1	0	1	2	1
Family	Filobasidiaceae	100	100	100	98	100	99	100	99	98	99
	Incertae sedis	0	0	0	2	0	1	0	1	2	1
Genus	Cryptococcus	100	100	100	98	100	99	100	99	98	99
	Unknown spec.	0	0	0	2	0	1	0	1	2	1

Relationships between microbial communities and soil properties

A generalized linear mixed model was used to test whether environmental factors were related to the relative abundances of microbial species. In Table 3, Firmicutes had a close relationship with NH₄-N concentrations and Planctomycetes was strongly related to TC and TN contents in the SI plot. In the SR plot, the bacterial phylum Firmicutes was related to soil pH, Proteobacteria was related to TN contents, and the fugal phylum Basidiomycota was related to NH₄-N concentrations.

Table 3 Relationship between soil properties and the number of OTUs of main phyla in SI (Sasa-intact) and SR (Sasa-removed) plots based on a generalized linear mixed model. The response variable was the number of OTUs of the main phyla. The fixed effect was the concentration of soil properties, and the random effect was the study plot. Only significant results with p<0.05 were listed.

Phylum	Soil properties	Intercept	Estimate	SE	z-value	p
SI plot
Firmicutes	Ammonium	−2.17	0.11	0.03	3.77	<0.001
Planctomycetes	Total nitrogen	−1.47	0.34	0.15	−2.23	0.03
	Total carbon	−1.44	0.03	0.01	−2.58	0.01
SR plot
Firmicutes	pH	−0.46	−0.37	0.18	−2.09	0.04
Proteobacteria	Total nitrogen	−1.84	0.61	0.27	2.27	0.02
Basidiomycota	Ammonium	−0.75	0.01	0	2.08	0.04

RDA has generally been used in microbial ecology to examine whether variations in microbial taxa changes correspond to environmental characteristics. As shown in Fig. 6A, phyla Bacteroidetes and Firmicutes were related to NO₃-N concentrations or pH, and five other bacterial phyla were each strongly and negatively related to the TN content, TC content, NH₄-N concentration, or C:N value in the SI plot. Although the species richness of fungi was low, the RDA analysis showed that the fungal phylum Basidiomycota was closely related to pH. Phyla Ascomycota and Zygomycota were both positively related to the TN content, TC content, NH₄-N concentration, and C:N value in the SI plot, but negatively related to the NO₃-N concentration in the SR plot (Fig. 6B).

Fig. 6

Redundancy analysis of main (A) bacterial and (B) fungal communities in Sasa-intact (solid circles) and Sasa-removed (open circles) plots based on Canoco 4.5. The purple, light green, orange, aqua, and pink colors represent the sampling dates of 23 July 2014, 1 October 2014, 3 June 2015, 4 August 2015, and 1 October 2015, respectively. Blue and dark green arrows indicate the abundance of microbes and values of soil properties, respectively. TN: total nitrogen; TC: total carbon; NH₄-N: ammonium; NO₃-N: nitrate.

Discussion

Microbial community in the presence of S. kurilensis

We found that the abundance of mycorrhizal fungi of the phylum Ascomycota was markedly higher in the SI plot (13.9%) than in the SR plot (0.54%) (Fig. 5B). Members of the family Pezizaceae were predominant among the Ascomycota identified in this study (Table 2); some Pezizaceae species are known to form truffles, while others act as mycorrhizal fungi (14, 23). These findings suggest that S. kurilensis serves as a host to a large reservoir of bamboo-associated mycorrhizal fungi. In the present study, the relative abundances of the main bacterial phyla identified (Proteobacteria, Planctomycetes, and Actinobacteria) were significantly different between the SI and SR plots (Fig. 5A), and the phyla Planctomycetes and Actinobacteria were slightly more abundant in the Sasa-removed plot than in the Sasa-intact plot (Fig. 6A). In soil, Proteobacteria, Planctomycetes, and Actinobacteria were found to be the main bacterial phyla co-occurring with the fungal class Pezizomycetes in the United States at almost the same latitude as our study site (50). Moreover, in the same study plots, Tsutsumi et al. found that the presence of S. kurilensis was closely related to the composition of methanotrophic bacterial communities (47). This result is consistent with our finding that the rhizome soil of S. kurilensis had a significant effect on the composition of bacterial communities (in addition to fungal ones). Therefore, we hypothesized that the presence of S. kurilensis affected the fungal family Pezizaceae (phylum Ascomycota) and bacterial phyla Proteobacteria, Planctomycetes, and Actinobacteria.

Microbial community structures may mediate soil properties

Due to their rich organic matter and low microbial decomposition rate, boreal forests act as a terrestrial net carbon sink in which a large amount of carbon is stored in tree roots and root-associated microorganisms (5, 34). Previous studies reported that the C:N ratio is a good indicator of microbial community structures in boreal forests (17). In the present study, we showed that the values of TC, TN, and C:N differed between the SI and SR plots (Fig. 3). Tripathi et al. (44, 45) reported differences in soil properties and nitrogen availabilities among bamboo stands including the SI and SR plots used in our study. These findings suggest that the composition of microbial communities, S. kurilensis, and soil properties in Betula forests are closely related, possibly because of their interactions with one other.

Root-associated Ascomycota may thrive in stressed environments because their mycelia have a complex structure of fungal cell walls that contain chitin and melanin and are resistant to microbial degradation (2, 7). As a result, Ascomycota mycelia are more likely to leave a large proportion of a fungal necromass that serves to store carbon in boreal soil (6, 9). Our results showed that the abundance of mycorrhizal fungi of the phylum Ascomycota increased with higher TC contents in the Sasa-intact plot (Fig. 6B); however, Ascomycota species richness was low. If the abundance of this mycorrhizal fungus is parallel to its greater biomass, one possible explanation for the greater TC in the SI plot is a close relationship between the presence of S. kurilensis and the mycorrhizal family Pezizaceae (phylum Ascomycota). According to our results, S. kurilensis appeared to promote the presence of the mycorrhizal family Pezizaceae (phylum Ascomycota), and the existence of this fungi appeared to increase the TC content in root-free soil. Further studies are needed in order to confirm this theory.

In addition, recent studies have shown that the mycorrhizal helper bacteria of herbaceous plants cooperate with mycorrhizal fungi owing to the presence of trehalose (10, 11). The results of the present study imply that some species of the phylum Planctomycetes co-occur with mycorrhizal fungi in S. kurilensis rhizomes, according to our analysis of the number of OTUs (Table 3). This result suggests that fungi and bacteria co-occur as a result of a biological interaction. However, since some significant relationships were detected between the phyla present and environmental factors, this co-occurrence may be an artefact due to mutual dependence on the same environmental factors.

Conclusion

Our results indicate that the presence of S. kurilensis in a B. ermanii boreal forest affected the compositions of soil fungal and bacterial communities and the corresponding soil properties. More soil water was retained after S. kurilensis was removed. Low fungal species richness was found in the Sasa-intact and Sasa-removed plots. The presence of S. kurilensis appeared to promote the colonization of soil mycorrhizal fungi of the family Pezizaceae (phylum Ascomycota), which may have meditated the amount of soil carbon in the dry soil environment. The present study enriches our understanding of how the presence of understory bamboo affects soil properties and corresponding microbial communities in a boreal forest.

Acknowledgements

We would like to thank the staff of the Uryu Field Research Center, Hokkaido University, for supporting our sampling. We also thank Hokkaido University and the Ministry of Education, Culture, Sports, Science and Technology (MEXT), Japan, for funding.

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