- Open Access
Specialisation events of fungal metacommunities exposed to a persistent organic pollutant are suggestive of augmented pathogenic potential
© The Author(s). 2018
- Received: 22 June 2018
- Accepted: 2 November 2018
- Published: 22 November 2018
The impacts of man-made chemicals, in particular of persistent organic pollutants, are multifactorial as they may affect the integrity of ecosystems, alter biodiversity and have undesirable effects on many organisms. We have previously demonstrated that the belowground mycobiota of forest soils acts as a buffer against the biocide pollutant pentachlorophenol. However, the trade-offs made by mycobiota to mitigate this pollutant remain cryptic.
Herein, we demonstrate using a culture-dependent approach that exposure to pentachlorophenol led to alterations in the composition and functioning of the metacommunity, many of which were not fully alleviated when most of the biocide was degraded. Proteomic and physiological analyses showed that the carbon and nitrogen metabolisms were particularly affected. This dysregulation is possibly linked to the higher pathogenic potential of the metacommunity following exposure to the biocide, supported by the secretion of proteins related to pathogenicity and reduced susceptibility to a fungicide. Our findings provide additional evidence for the silent risks of environmental pollution, particularly as it may favour the development of pathogenic trade-offs in fungi, which may impose serious threats to animals and plant hosts.
Chemical pollution constitutes a major threat to the sustainability of Earth’s ecosystems; its impacts on biodiversity affect key ecosystem services, such as soil formation and nutrient recycling [1, 2]. Microbes—the unseen majority—are fundamental for the multi-functionality of ecosystems , yet progressively hindered by exposure to many disparate chemicals that are spread on a global scale. In particular, chronic exposure to persistent organic pollutants (POPs) released either locally or remotely through long-range atmospheric/oceanic transport is known to dramatically affect the structure, stability and function of microbial communities . Pentachlorophenol (PCP) has a history of use dating back 80 years. Although it was regarded as mostly safe for the first few decades, PCP was eventually included in the Pesticide Action Network’s Dirty Dozen list in 1998 and added to the Treaty of the Stockholm Convention list of banned POPs in 2015 , due to its far-reaching toxicity. Its long history of use, coupled with its persistence and ease of transboundary dispersal, has resulted in extensive environmental PCP contamination worldwide [5, 6]. Today, PCP is still detected in human bodily fluids and tissues following exposure in indoor and/or outdoor environments around the world .
Recently, we showed the existence of undefined active sources of PCP pollution in the Tabarka district (Tunisia), particularly in soils collected within cork oak forests [4, 7]. The soils were contaminated with PCP levels ranging from 13 to 28 μg/kg of soil. The source and history of the pollution in these soils is unknown [4, 7]. Furthermore, we demonstrated that fungi isolated from these PCP-polluted forest soils can extensively degrade PCP, in theory acting as a buffer against PCP pollution in these habitats . Due to their remarkable catabolic capacities, ubiquitous occurrence and lifestyle , saprotrophic fungi possess a peerless ability to degrade harmful chemicals, such as PCP [7, 9–11]. However, regardless of their ability to mitigate pollutants in soils, these activities raise several concerns: How are their communities affected by pollutants at the taxonomic and functional levels? Are there physiological costs underlying the trade-off between PCP degradation and survival?
To address these questions, we have relied on a culture-dependent approach to study the temporal response of a metacommunity of fungi to PCP exposure, uncovering the PCP-derived metabolome, physiological profile, metaproteome and metataxonomy (i.e. stable isotopic probing followed by amplicon sequencing). We show that when confronted with the half maximal effective concentration (EC50) of PCP, the metacommunity degraded nearly 70% of the biocide in only 10 days leading, in part, to its mineralisation. Furthermore, we show that PCP exposure altered the taxonomic diversity of the metacommunity, where the loss of some taxa was accompanied by the rise of key PCP-assimilators. It also influenced the proteome within the community; many of the affected proteins were associated with carbohydrate and nitrogen metabolisms. As a final point, PCP pollution was observed to induce functional shifts in the metacommunity suggestive of increased pathogenic potential, which in turn may increase the dispersal of airborne opportunistic pathogens capable of affecting both animal and plant hosts.
The trade-off between PCP degradation and physiological profile
To preliminarily uncover the functional costs of PCP degradation within the metacommunity, we analysed the community level physiological profiles (CLPP) at the first and last time points of PCP exposure (Fig. 1a). The biocide did not significantly alter either the functional diversity of the metacommunity (Shannon index, H′) or the number of used substrates compared to control conditions. At the final time point, these values ranged from H′ = 4.34 (± 0.06) to 4.41 (± 0.02) and Nsubstrates = 91.67 (± 0.79) to 94.33 (± 0.58) in the metacommunities exposed or not exposed to PCP, respectively. However, PCP effects on the utilisation of individual substrates were obvious: there was a 60% decrease in the utilisation of carbohydrates and 13% decrease in the utilisation of carboxylic acids; a 35% increase in the utilisation of nitrogen-containing substrates (grouped as miscellaneous) and 14% increase in the utilisation of amino-acids (Fig. 1c, Additional file 1: Table S2, Additional file 3: Dataset S2).
Scoring PCP assimilators within the metacommunity of fungi confronted with PCP
Seventy-seven strains were previously isolated by us from the same soil used here as the source of the metacommunity inoculum . As expected, the sequences of the internal transcribed spacer (ITS) region of 34 of these fungal strains matched a few of the OTUs obtained in the present study (defined by their accession number in the CBS-KNAW culture collection, Additional file 4: Dataset S3).
Unveiling the proteome responses of the metacommunity of fungi confronted with PCP
In addition to its effects on the metacommunity composition, PCP also greatly affected the utilisation profiles of carbon- and nitrogen-containing substrates. To verify if such alterations can be detected at the proteome level, changes in the levels of mycelial and extracellular proteins (i.e. secretome) of the metacommunity throughout the PCP exposure (relative to control conditions) were identified. The numbers of mycelial proteins with altered levels (relative to controls; referred to as differential proteins) were 94 and 74 on the third and tenth days of exposure to PCP, respectively. Of these, only 22 proteins were common to both sets. In the secretome, these numbers were 10 and 15, with only 5 common to both time points (Additional files 5 and 6: Datasets S4 and S5).
To investigate the biological significance of PCP effects on the mycelial metaproteome, we scrutinised the differential proteins exhibiting the highest log2FC. Unsurprisingly, the changes in the levels of many glycolytic enzymes were found to be among the largest changes observed (|7.4| ≤ log2FC ≤ |9.7|), either when PCP levels were close to the EC50 [aldehyde dehydrogenase; phosphoglycerate kinase; pyruvate kinase; enolases; GAPDH (glyceraldehyde-3-phosphate dehydrogenases)] or threefold lower [GAPDHs; phosphoglycerate kinase; enolases] (Additional file 1: Table S5, Additional file 6: Dataset S5). The levels of aldehyde and alcohol dehydrogenases greatly increased upon PCP exposure (P41751 and P08843, log2FC = 8.5 and 7.42). These enzymes have been previously linked to the degradation of many aromatic hydrocarbons, e.g., naphthalene . The involvement of these enzymes in the degradation of PCP (Fig. 1b) is therefore a possibility. Many other enzyme classes have been linked to PCP degradation, e.g., cytochrome P-450 monooxygenases, tyrosinases, reductive dehalogenases and transferases ; none of which exhibited increased levels in the mycelial metaproteome following PCP exposure (Additional file 6: Dataset S5). Finally, the ability of the biocide to uncouple oxidative-phosphorylation in mitochondria  may be linked to the major dysregulation of some mitochondrial proteins [viz. aconitate hydratase, ATP synthase subunit alpha; citrate synthase; (|7.1| ≤ log2FC ≤ |8.5|] (Additional file 1: Table S5, Additional file 6: Dataset S5). The levels of several mycelial proteins associated with the stress response functional category were also greatly increased by exposure to PCP [viz. heat shock protein (HSP) 70 kDa; HSP SSA1; thiamine thiazole synthases; (|7.5| ≤ log2FC ≤ |9.2|] (Additional file 1: Table S5). Increase levels of HSP, which act as molecular chaperones, assisting the correct folding of native and stress accumulated misfolded proteins, were reported in Mucor plumbeus exposed to PCP . Thiamine thiazole synthase levels increased during adaptation to various stress conditions and are possibly involved in DNA damage tolerance .
Regardless of the fact that only a small number of proteins were identified in the differential extracellular metaproteome, it adds important details to the snapshot analysis of the biocide effects (Fig. 5b). Incorporation of data from the extracellular metaproteome adds sporulation and antagonistic activity to the list of affected functional categories (at both time points sampled post PCP exposure). PCP also affected extracellular proteins involved in carbohydrate metabolism, amino acid metabolism, protein biosynthesis and stress response; a similar pattern to that observed in the mycelia (Fig. 5b). Among the extracellular proteins showing increased levels following 10 days of PCP exposure, we found cytochrome P450 (CYP55A2, log2FC = 6.3, Fig. 5b). Cytochrome P450 may play a role in the degradation pathway of PCP .
The burden of PCP augments the pathogenic potential of the metacommunity of fungi
When confronted with PCP, the metacommunity adjusted in order to degrade it, leading ultimately to its mineralisation (Figs. 1, 2 and 3). This was achieved via a trade-off resulting in the impairment of many functional categories (Fig. 5) and the increased use of varied nitrogen-containing substrates (Fig. 1c). The ability of fungi to resort to varied nitrogen sources, either to bypass nitrogen starvation or any other conditional metabolic limitation, is critical for the establishment of pathogenicity and considered as a virulence trigger. Taken as examples, the deletion of the gene encoding GAT1, which impaired nitrogen utilisation in Candida albicans, lowered its virulence in murine models , whereas deletion of AreA/Nit2 gene encoding the transcription factor that controls the expression of genes involved in the transport/catabolism of nitrogen was demonstrated to severely weaken phytopathogenicity in, e.g., Magnaporthe grisea and Fusarium oxysporum .
In line with the hypothesis that PCP may trigger pathogenicity in the metacommunity of fungi, we observed here that nearly half (8 out of 20) of the extracellular proteins that were increased at either sampled time point following PCP exposure have been associated with pathogenic or allergenic potentials, namely GAPDH , trypsin , catalase-peroxidase , alkaline proteinase , endochitinase , endo-1,3-β-glucanase  and cytochrome P450 55A2 (CYP55A2) (Fig. 5b, marked with an asterisk). In addition, throughout incubation in the presence of PCP, the metacommunity greatly increased the pH of the medium, which was unaltered in the controls (Additional file 1: Figure S2). The ability of fungi to change the surrounding pH and to grow at alkaline conditions has also been recognised as a key pathogenicity marker . Finally, the metacommunity grown in media without PCP, after acute treatment with miconazole, showed negligible metabolic activity (absorbance(570nm) = 0.07 ± 0.02), as expected (Additional file 1: Figure S3). On the contrary, and remarkably, following only 10 days of PCP exposure, the capacity of the metacommunity to bypass the effect of the fungicide increased dramatically (absorbance(570nm) = 0.3 ± 0.07), with a concurrent increase in pathogenic potential .
Our results support the hypothesis that fungi pay a high functional cost during exposure to PCP pollution, regardless of superior capacity to degrade the biocide. In a culture-dependent set-up, PCP affected the overall diversity of the metacommunity, in particular it reduced the diversity of the less abundant taxa and promoted also the growth of the most abundant taxa, most of which were capable of assimilating, to some extent, the biocide. Carbohydrate metabolism was critically hindered throughout the entire exposure time, despite the fact that PCP levels were progressively reduced. The metacommunity of fungi circumvented the impacts of the biocide by utilising a variety of nitrogen-containing substrates, which potentially functioned as a virulence trigger. Essentially, PCP exposure greatly reduced the overall susceptibility of the fungal metacommunity to a fungicide and elicited the secretion of proteins that have been found to be associated with pathogenesis.
Atmospheric release of POPs constitutes a silent threat through the chronic contamination of soils on a global scale; yet a fundamental understanding of their impacts is still mostly lacking. The findings of our study extend far beyond the specific issue of PCP pollution. PCP can be considered an archetypal POP since its simple structure—a halogenated aromatic—is found in many POPs that are potentially degraded through biotic pathways that converge on the same pathways used in PCP degradation [8, 11]. Our approach does not intend to directly simulate the natural setting, but it did allow capturing key specialisation events of the metacommunity exposed to the biocide at multiple functional and taxonomic levels; this despite the study’s limits: the loss of some uncultivable taxa and assignment of most proteins sequences to well-known taxa. In this study, the taxa identified as dominant throughout PCP exposure were among the most abundant in the initial soil sample. One hypothesis is that the metacommunity of fungi, which originated from PCP-polluted soils, has been long-suffering the impacts of PCP at both functional and diversity levels. One critical question to be addressed in the near future is how the metacommunity of fungi evolves under chronic PCP exposure conditions, especially as a further imbalance of nitrogen utilisation, with a consequential rise of opportunistic fungal pathogens, should not be ignored. The depletion of nitrogen sources from soils potentially impacts the continuous supply of ecosystem services (e.g., soil fertility and water retention capacity). Therefore, our experimental observations indirectly interrogate if the atmospheric deposition of PCP in cork oak forests may be behind the deterioration observed in these agro-forestry landscapes. Surely, the importance of the link between pollution with PCP (or with other POPs containing similar structural units) and the increase of pathogenic potential in fungi goes way beyond matters of forest sustainability. Annually, fungi kill nearly 2 million people, worldwide . The inhalation of fungal spores, even of non-pathogenic fungi, can lead to devastating invasive infections in vulnerable immunocompromised/suppressed patients of all ages. The stimulation of increased fungal pathogenicity due to POP exposure is not something that can be ignored.
Microbial communities consist of sub-communities that often contain the same dominant strains, yet contain a distinct composition of the less abundant strains . Conventional culture-dependent assays may favour the development of only a subset of particular sub-communities. To establish a metacommunity of fungi comprising many distinct sub-communities, the community-based cultures were dispersed into many growth containers that were pooled at the end of the experiment, similar to the methodology applied for the establishment of metacommunities composed of several local bacterial communities . Briefly, each biological replicate comprised five 6-well plates (total of 30 wells), each well containing 5 mL of growth medium with or without 38 μM of 13C PCP (i.e. EC50). The growth media of each biological replicate was mixed with the metacommunity inoculum (ratio of 10:1), then distributed into 30 culture-wells. Cultures were incubated at 30 °C, 90 rpm (triplicates of 30 wells per condition) and harvested at the third, fifth, seventh and tenth day of exposure (triplicates). Culture aliquots were used for the physiological profiling. The mycelial and the extracellular fractions were separated using vacuum filtration, the fresh mycelia weight was recorded and both fractions conserved at − 80 °C until further use. The extracellular fractions were used to evaluate the degradation of PCP (viz. PCP residual levels by liquid chromatography and PCP-derived metabolites by mass spectrometry) and the secretome. The intracellular fractions were used to study the community composition (amplicon sequencing), the mycelial proteome and the intracellular PCP-derived metabolites (mass spectrometry). Complementary analyses included measures of the medium pH along cultivation as well as the effect of miconazole on the metabolic activity (MTT reduction assay) of the metacommunity after 10 days of exposure to PCP compared to control conditions (see Additional file 1: Figure S3).
If not explicitly stated otherwise, chemicals were of analytical grade and purchased from Sigma-Aldrich. All liquid chromatography (LC) and mass spectrometry (MS) solvents were of the highest analytical grade.
Inoculum of the metacommunity of fungi
The inoculum of the metacommunity of fungi originated from soils sampled inside cork oak forests in Tunisia (E008° 51′ 00.00 N36° 46′ 00.00, Tabarka district, Tunisia) as previously described . In brief, each soil sample is composed by soil collected in each quadrant defined by 1 × 1 m2, using a 3-cm-diameter gauge auger at a single depth: 0–20 cm, which was pooled and sieved (< 2 mm). Herein, the three Aîn Hamraia forest soil samples corresponding to distinct forest locations (Additional file 1: Table S7) were carefully combined before use (total soil volume of ca. 2 L). To recover the mycobiota, a soil aliquot (15 g) was immersed (1:10, w/v) into a solution of 0.1% peptone (w/v) and 0.1% chloramphenicol (v/v) (60 min, soft agitation, vacuum cycle every 20 min), then sieved (pore sizes of 500 μm, 210 μm then 100 μm) and finally distributed into 1-mL aliquots that were stored at − 80 °C, as established previously .
Half maximal effective concentration of PCP against the metacommunity of fungi
The half maximal effective concentration (EC50) of PCP was determined using 5-mL cultures (6-well plates; 2 plates per replicate). Growth media (1% w/v of glucose in a mineral minimal media [10, 12], MMG) containing 19, 38, 95, 190, 380 or 760 μM of PCP were mixed with the metacommunity inoculum (ratio of 10:1), incubated at 30 °C, 90 rpm for 7 days (triplicates, including negative controls without PCP). Following incubation, 50 μL from each biological replicate (pool of 12 wells) were spread onto MEA and the number of colony forming units (CFUs) monitored daily during 5 days and compared to that of the negative controls (triplicates). To obtain the EC50 value, results were adjusted to a logistic regression using the dose effect tool of XL-STAT software version 2009.1.02 (Addinsoft).
PCP was quantified using ultra-performance liquid chromatography (UPLC) as previously described . Chromatographic profiles were acquired at 212 nm and PCP quantification limits were 0.38–56 μM (retention time of 5.9 min). The diversity of PCP-derived metabolites and sub-products in both the extra- and intra-cellular compartments at the third, fifth, seventh or tenth day of exposure to PCP were resolved using ultra high performance liquid chromatography–electrospray–high-resolution mass spectrometry (UHPLC-ESI-HRMS) operated in negative ESI mode using a Q-Exactive Orbitrap MS system (Thermo-Fisher Scientific) as previously described [7, 12, 30]. MS data were processed by ExactFinder™ 2.0 software (Thermo-Fisher Scientific), applying a user target database list and validated, whenever possible, using standard compounds.
Carbon and nitrogen metabolism
The ability of the metacommunity of fungi to use specific carbon and nitrogen sources was analysed using Biolog FF plates following the manufacturers’ guidelines. The cultures were grown in MMG with or without 38 μM of PCP during 3 or 10 days, as described above, before testing. The plates were incubated at 30 °C and the absorbance of each plate at 490 nm and 750 nm was measured daily for 5 days. Functional diversity (Shannon index, H′) and richness were calculated as previously described . Carbon and nitrogen sources were grouped by category . To reveal functional categories affected on the third or tenth day of PCP exposure compared to controls, the ratios of the increase or decrease of use of each substrate were normalised, and a histogram constructed using XL-STAT software version 2014.5.03 (Addinsoft, France).
Metataxonomics of the metacommunity-based cultures
The metacommunity diversity on the third and tenth day of cultivation, both in the presence and absence of the stable isotope 13C-labelled PCP, was analysed, as well as that of the inoculum, i.e. the metacommunity directly recovered from soils that originated from the cork oak forests. 13C-labelled PCP was used to mark OTUs capable of PCP assimilation (see below Isopycnic ultracentrifugation).
The frozen mycelia were macerated using a pestle and mortar, then further ground with the aid of an extraction buffer (50 mM of NaH2PO4, 50 mM NaCl, 500 mM Tris-HCl, 5% SDS, pH 8; 600 μL per culture) and glass beads (1 g, equal amounts of 0.5 and 0.1 mm beads) using a TissueLyzer LT Adapter (Qiagen, Germany), for 5 min at top speed. Afterwards, the sample was mixed with a half volume of each: phenol and chloroform containing isoamyl alcohol (24:1; hereafter defined as solution A); shaken for 2 min and centrifuged (5 min, 2,400 g) to recover the upper supernatant (i.e. aqueous phase) which was re-extracted with an equal volume of solution A, and recovered as described before. To this mixture, 1/3 volume of 6 M NaCl and 1/10 volume of 10% of cetyl trimethylammonium bromide (CTAB) in 0.7 M of NaCl were added, and the mixture was incubated for 30 min at 65 °C. After cooling to room temperature, an equal volume of solution A was added, shaken and centrifuged (20 min, 1400 g) to recover the supernatant. Finally, DNA was precipitated in 2/3 volume of isopropanol and 1/10 volume of acetate solution (3 M) during 20 min at room temperature, and recovered by centrifugation (20 min, 6800 g). The DNA pellet was washed with 200 μL of ethanol (70%), recovered by centrifugation as before, air dried for 60 min, eluted in 50 μL of TE buffer (Qiagen, Germany) and finally stored at − 20 °C. Prior to use, the DNA samples were cleaned using the GeneClean Turbo kit for 100–300 kb fragments (MP Biomedicals, USA) following the manufacturer instructions.
Isopycnic ultracentrifugation was used to separate the “heavy” (i.e. that incorporated 13C) and the “light” DNA fractions, both of which were used to generate amplicon sequencing data (Additional file 4: Dataset S3). The separation of the 13C-labelled DNA from the unlabelled DNA was carried out following an established protocol with some modifications . Specifically, the DNA samples were re-suspended in 10 mM ethylenediaminetetraacetic acid (EDTA, final volume of 4 mL), then mixed with 4.7 g of cesium chloride (CsCl) and 10 μL of RedSafe (Chembio Diagnostics, USA) and transferred to 4.7 mL OptiSeal tubes (Beckman Coulter, USA) and centrifuged in an Beckman Optima Max XP, equipped with a TLA-110 rotor, for 40 h, 311,438 g, k-factor = 21.2, with no break. The light and heavy DNA bands were visualised under a fluorescent light (514 nm) and were recovered by piercing the tube with a syringe. DNA was extracted using a 2:1 butanol/NaCl solution (v/v, saturated NaCl), washed with ethanol, then eluted in MilliQ water and stored at − 20 °C.
For the analysis of fungal community composition, the ITS2 region of fungal rDNA was PCR-amplified in a GeneAmp PCR system 2720 (Applied Biosystems) using barcoded gITS7 and ITS4 primers (gITS7, 5′-GTG ART CAT CGA RTC TTT G-3′; ITS4, 5′-TCC TCC GCT TAT TGA TAT GC-3′)  in technical triplicates, including quality controls, as previously described . The quality of the PCR products was monitored using gel electrophoresis. The technical replicates were pooled and sequenced on an Illumina MiSeq system. NGS analysis was performed by the Gene Expression Unit at Instituto Gulbenkian de Ciência (Oeiras, Portugal).
Amplicon sequencing data analysis
The amplicon sequencing data were processed using the pipeline SEED 2.1 . Briefly, paired-end reads were joined using FASTQ-join . The ITS2 region was extracted using ITSx1.0.11  before processing. Chimeras were identified using USEARCH 8.1.1861 and deleted. Sequences were clustered using UPARSE implemented within USEARCH  at a 97% similarity level. The most abundant sequences were selected for each cluster, and the closest hits were identified using BLASTn against GenBank. Singletons were discarded. The cladograms based on the ITS2 sequence similarity of the identified OTUs were generated using PhyML to illustrate the diversity of the taxonomy within the metacommunity, regardless that the high variability of the ITS2 region does not allow a precise topology. The cladograms were then visualised and edited graphically using FigTree 1.4.3.
Metaproteomics of the metacommunity-based cultures
Extraction of mycelial proteins
Mycelial proteins were extracted using a modified trichloroacetic acid (TCA)/acetone protocol . Briefly, the frozen mycelia (in liquid nitrogen) were ground using a pestle and mortar and homogenised in extraction buffer: 50 mM of Tris-HCl at pH 7.5, 200 mM NaCl, 5 mM EDTA, 0.5% Triton X-100 and EDTA-free EASYpack protease inhibitors (Roche, Switzerland). To facilitate homogenisation and cell rupture, a TissueLyzer LT Adapter (Qiagen, Germany) was used, first 1 g of glass beads (half of each size: 0.5 and 0.1 mm) were added and then two consecutive cycles of 5 min at top speed were applied. Proteins were precipitated in acetone containing 10% (v/v) trichloroacetic acid (TCA) and 40 mM of dithiothreitol (DTT) (1:10 w/v) for 1 h at − 20 °C; the pellet recovered by centrifugation at 10,400 g for 15 min, washed three times in 10 mL of acetone containing 40 mM of DTT, finally dried under a nitrogen flow and stored at − 80 °C until further analysis.
The extracellular culture fractions were first concentrated ca. 30-fold using Vivaspin Turbo 15 ultra-filtration systems (Sartorius, Germany). The concentrated samples were mixed with 200 mL of a boiling SDS solution (2% SDS, 40 mM of Tris-base and 60 mM of DTT) and shaken at 99 °C and 350 rpm for 5 min in a Thermomixer (Eppendorf, Germany), then maintained at − 20 °C overnight. Finally, proteins were precipitated in acetone with 60 mM DTT for 1 h at − 20 °C, and recovered by centrifugation (4 °C, 15 min, 21,630 g), washed five times with acetone containing 60 mM DTT, finally dried under nitrogen flow and stored at − 80 °C until further analysis.
Mass spectrometry analyses of protein extracts
Proteins were recovered from the culture filtrates using denaturing precipitation conditions . Then, 10 μg of protein (quantification performed with RC DC™ protein assay kit, Bio-Rad) was loaded on to a precast gel (Criterion ™ XT precast 1D gel 4–12% Bis-Tris, Bio-Rad) and separated using a short migration. The gel was stained with Instant Blue (Gentaur BVBA, Kampenhout, Belgium), sliced into bands. Proteins were first reduced, then alkylated and de-stained and finally digested using trypsin (sequencing mass grade, Promega). Peptides were extracted, dried and stored at − 20 °C until LC-MS analysis. Peptides were analysed with a nano-HPLC system (NanoLC-2D, Eksigent, Sciex) coupled to a Triple TOF 5600+ mass spectrometer (Sciex, Darmstadt, Germany) operated on positive ESI mode with a Nanospray III source. In detail, after desalting and enrichment on C18 pre-column (C18 PepMap™, 5 μm, 5 mm × 300 μm, Thermo scientific), peptides were separated with a C18 reverse-phase column (C18 PepMap™ 100, 3 μm, 100 Å, 75 μm × 15 cm, Thermo scientific) using a linear binary gradient (A: 0.1% formic acid; B: 80% acetonitrile, 0.1% formic acid) at a flow rate of 300 nL/min. Peptides were eluted from 5 to 55% solvent B over 45 min. Solvent B was then increased to 100% to wash the column before re-equilibrating for 25 min prior to the next injection. The 20 most intense precursors were selected for fragmentation. The CID spectra were processed with Mascot (version 2.4.2) using Mascot Daemon interface (version 2.4.2, Matrix Science, London, UK) by searching against the SwissProt Fungi (31527 sequences) database released on May 2015 and the Emericella nidulans (36,970 sequences; 18,794,350 residues) database released on the 13 November 2015. Only the proteins identified with a significance MASCOT-calculated threshold p value < 0.05 and at least two significant peptides per proteins were accepted.
The amplicon sequencing data attained without any isotopic separation was first treated to assess the overall relative abundances between conditions (incubation with PCP and controls, at the third and tenth day). Descriptive statistics of the OTUs relative abundance and a Jaccard-based hierarchical cluster analysis of their diversity (presence versus absence) were performed using XL-STAT software version 2014.5.03 (Addinsoft, France). The histogram analysis used as weights the normalised number of reads of each OTU (relative abundance) per sample (SIP separation not considered), sub-sampled for the depth of the Illumina MiSeq run (100,000 reads).
To study the differential relative abundance of each specific OTU in the light and heavy DNA fractions, we estimated the probability of major fold changes (FC) between the two conditions (negative binomial distribution) as follows: the OTU counts were normalised within each sample and sub-sampled as mentioned above, set to integers and then analysed using the RStudio (version 1.0.153) Bioconductor package DESeq2 . Those presenting differential abundance (normalised counts bigger than 100 reads) between fractions or between the fractions and the controls were classified as 13C assimilators. Non-metric multidimensional scaling (NMDS) was used to visualise treatment effects. To build the NMDS, the normalised and sub-sampled counts were standardised within each OTU and then a Bray-Curtis resemblance matrix was built and plotted using a minimum stress of 0.01, using PRIMER 6.1.13 (PRIMER-E, Ltd). The assimilation category of each OTU was used as label.
To test differences at the pH measurements and MTT assays (comparing values obtained after incubation with PCP and controls), Student’s two sample t tests were performed after Cohen’s D test (to assess the power of variance comparisons, f > 0.04) using the tool of XL-STAT software version 2014.5.03 (Addinsoft, France).
Only the proteins that were present in at least two out of three biological replicates were considered for further analyses. The relative quantification of the proteins has been calculated using the normalised spectral abundance factor (NSAF) . The spectral counts of each mass were normalised and further analysed using the RStudio (version 1.0.153) Bioconductor package edger  following generalised linear models [42, 43]. This approach was used to analyse both the mycelial and the extracellular metaproteome. The cumulative log2FC for each functional category was plotted using Microsoft Excel, discriminating the contributions of the distinct taxonomic classes.
The authors are extremely thankful to Maria C. Leitão (ITQB NOVA) and Carlos Elias (IGC) for support in the chromatographic analyses and the isopycnic ultracentrifugation, respectively. The authors are also thankful to James Yates (ITQB NOVA) for the English proofreading of the manuscript.
We acknowledge funding from the European Research Council through grant ERC 2014-CoG-647928; from Fundação para a Ciência e Tecnologia (FCT), grant UID/Multi/04551/2013 (Research unit GREEN-it “Bioresources for Sustainability”); from the Spanish Ministry of Economy and Competitiveness, project CTQ2015-63968-C2-1-P; and from the Agency for Administration of University Research Grants (Generalitat de Catalunya, Spain), project 2017SGR310. CM is grateful to FCT for the fellowship SFRH/BD/118377/2016.
Availability of data and materials
Additional file 1 word document is available, containing more detailed tables and figures that support the figure panels at the main text. Additional file 2: data file S1 provides mass spectrometry datasets (xls format) on the metabonomics of the metacommunity. Additional file 3: data file S2 contains Biolog FF datasets (xls format): normalised datasets of the absorbance of each substrate, disclosing alterations upon exposure to PCP compared to control conditions. Additional file 4: data file S3 provides the amplicon sequencing raw count data, including description of the identified OTUs and discrimination of OTUs as 13C-labelled PCP assimilators. Additional file 5: data file S4 shows the mass spectrometry datasets on the proteomes of the metacommunity. Additional file 6: data file S5 lists all the mycelial proteins that underwent alterations after exposure to PCP compared to control conditions. The amplicon sequencing data has been deposited in the Sequence Read Archive (NCBI) with the submission code SRP145967. The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE  partner repository with the dataset identifier PXD009798 and https://doi.org/10.6019/PXD009798.
CSP supervised the project and the interpretation of data and prepared the final version of the manuscript. All authors have made substantial contributions to the acquisition, analysis and interpretation of data and contributed to the drafting of the manuscript: CM (experimental set up design, data analysis and statistics, preparation of the initial draft of the manuscript); CM and AV (metacommunity experiments); CCL and JR (proteomic analyses); ON (metabolome analyses); CM, TV and PB (amplicon sequencing data processing). All authors read and approved the final version of the manuscript.
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- Cardinale BJ, Duffy JE, Gonzalez A, Hooper DU, Perrings C, Venail P, Narwani A, Mace GM, Tilman D, Wardle DA, et al. Biodiversity loss and its impact on humanity. Nature. 2012;486:59–67.View ArticleGoogle Scholar
- Backhaus T, Snape J, Lazorchak J. The impact of chemical pollution on biodiversity and ecosystem services: the need for an improved understanding. Integr Environ Assess Manag. 2012;8:575–6.View ArticleGoogle Scholar
- Naeem S, Duffy JE, Zavaleta E. The functions of biological diversity in an age of extinction. Science. 2012;336:1401–6.View ArticleGoogle Scholar
- Varela A, Martins C, Silva Pereira C. A three-act play: pentachlorophenol threats to the cork oak forest soils mycobiome. Curr Opin Microbiol. 2017;37:142–9.View ArticleGoogle Scholar
- Czaplicka M. Sources and transformations of chlorophenols in the natural environment. Sci Total Environ. 2004;322:21–39.View ArticleGoogle Scholar
- Morgan M, Jones P, Sobus J. Short-term variability and predictors of urinary pentachlorophenol levels in Ohio preschool children. Int J Environ Res Public Health. 2015;12:800–15.View ArticleGoogle Scholar
- Varela A, Martins C, Núñez O, Martins I, Houbraken JA, Martins TM, Leitão MC, McLellan I, Vetter W, Galceran MT, Silva Pereira C. Understanding fungal functional biodiversity during the mitigation of environmentally dispersed pentachlorophenol in cork oak forest soils. Environ Microbiol. 2015;17:2922–34.View ArticleGoogle Scholar
- Harms H, Schlosser D, Wick LY. Untapped potential: exploiting fungi in bioremediation of hazardous chemicals. Nat Rev Microbiol. 2011;9:177–92.View ArticleGoogle Scholar
- Carvalho MB, Martins I, Medeiros J, Tavares S, Planchon S, Renaut J, Nunez O, Gallart-Ayala H, Galceran MT, Hursthouse A, Silva Pereira C. The response of Mucor plumbeus to pentachlorophenol: a toxicoproteomics study. J Proteome. 2013;78:159–71.View ArticleGoogle Scholar
- Carvalho MB, Tavares S, Medeiros J, Núñez O, Gallart-Ayalla H, Leitão MC, Galceran MT, Hursthouse A, Silva Pereira C. Degradation pathway of pentachlorophenol by Mucor plumbeus involves phase II conjugation and oxidation-reduction reactions. J Hazard Mater. 2011;198:133–42.View ArticleGoogle Scholar
- Gadd GM. Fungi in bioremediation: Cambridge University Press; 2001.Google Scholar
- Martins TM, Nunez O, Gallart-Ayala H, Leitao MC, Galceran MT, Silva Pereira C. New branches in the degradation pathway of monochlorocatechols by Aspergillus nidulans: a metabolomics analysis. J Hazard Mater. 2014;268:264–72.View ArticleGoogle Scholar
- Větrovský T, Baldrian P, Morais D. SEED 2: a user-friendly platform for amplicon high-throughput sequencing data analyses. Bioinformatics. 2018;34(13):2292–294View ArticleGoogle Scholar
- Žifčáková L, Větrovský T, Howe A, Baldrian P. Microbial activity in forest soil reflects the changes in ecosystem properties between summer and winter. Environ Microbiol. 2016;18:288–301.View ArticleGoogle Scholar
- Morel G, Sterck L, Swennen D, Marcet-Houben M, Onesime D, Levasseur A, Jacques N, Mallet S, Couloux A, Labadie K, et al. Differential gene retention as an evolutionary mechanism to generate biodiversity and adaptation in yeasts. Sci Rep. 2015;5:11571.View ArticleGoogle Scholar
- Fuchs G, Boll M, Heider J. Microbial degradation of aromatic compounds—from one strategy to four. Nat Rev Microbiol. 2011;9:803.View ArticleGoogle Scholar
- Medina-Silva R, Barros MP, Galhardo RS, Netto LE, Colepicolo P, Menck CF. Heat stress promotes mitochondrial instability and oxidative responses in yeast deficient in thiazole biosynthesis. Res Microbiol. 2006;157:275–81.View ArticleGoogle Scholar
- Limjindaporn T, Khalaf RA, Fonzi WA. Nitrogen metabolism and virulence of Candida albicans require the GATA-type transcriptional activator encoded by GAT1. Mol Microbiol. 2003;50:993–1004.View ArticleGoogle Scholar
- Bolton MD, Thomma BP. The complexity of nitrogen metabolism and nitrogen-regulated gene expression in plant pathogenic fungi. Physiol Mol Plant Pathol. 2008;72:104–10.View ArticleGoogle Scholar
- Seidler NW. GAPDH, as a virulence factor. In: In GAPDH: Biological Properties and Diversity Springer; 2013. p. 149–78.View ArticleGoogle Scholar
- Dubovenko AG, Dunaevsky YE, Belozersky MA, Oppert B, Lord JC, Elpidina EN. Trypsin-like proteins of the fungi as possible markers of pathogenicity. Fungal Biol. 2010;114:151–9.View ArticleGoogle Scholar
- Mir AA, Park S-Y, Sadat MA, Kim S, Choi J, Jeon J, Lee Y-H. Systematic characterization of the peroxidase gene family provides new insights into fungal pathogenicity in Magnaporthe oryzae. Sci Rep. 2015;5:11831.View ArticleGoogle Scholar
- Selvam RM, Nithya R, Devi PN, Shree RSB, Nila MV, Demonte NL, Thangavel C, Maheshwari JJ, Lalitha P, Prajna NV, Dharmalingam K. Exoproteome of Aspergillus flavus corneal isolates and saprophytes: identification of proteoforms of an oversecreted alkaline protease. J Proteome. 2015;115:23–35.View ArticleGoogle Scholar
- Huang Z, Hao Y, Gao T, Huang Y, Ren S, Keyhani NO. The Ifchit1 chitinase gene acts as a critical virulence factor in the insect pathogenic fungus Isaria fumosorosea. Appl Microbiol Biotechnol. 2016;100:5491–503.View ArticleGoogle Scholar
- Garfoot AL, Dearing KL, VanSchoiack AD, Wysocki VH, Rappleye CA. Eng1 and Exg8 are the major β-glucanases secreted by the fungal pathogen Histoplasma capsulatum. J Biol Chem. 2017;292:4801–10.View ArticleGoogle Scholar
- Davis DA. How human pathogenic fungi sense and adapt to pH: the link to virulence. Curr Opin Microbiol. 2009;12:365–70.View ArticleGoogle Scholar
- Fairlamb AH, Gow NA, Matthews KR, Waters AP. Drug resistance in eukaryotic microorganisms. Nat Microbiol. 2016;1:16092.View ArticleGoogle Scholar
- Denning DW, Bromley MJ. How to bolster the antifungal pipeline. Science. 2015;347:1414–6.View ArticleGoogle Scholar
- Low-Décarie E, Kolber M, Homme P, Lofano A, Dumbrell A, Gonzalez A, Bell G. Community rescue in experimental metacommunities. Proc Natl Acad Sci U S A. 2015;112:14307–12.View ArticleGoogle Scholar
- Martins I, Garcia H, Varela A, Núñez O, Planchon S, Galceran MT, Renaut J, Rebelo LP, Silva Pereira C. Investigating Aspergillus nidulans secretome during colonisation of cork cell walls. J Proteome. 2014;98:175–88.View ArticleGoogle Scholar
- Liu B, Tu C, Hu S, Gumpertz M, Ristaino JB. Effect of organic, sustainable, and conventional management strategies in grower fields on soil physical, chemical, and biological factors and the incidence of southern blight. Appl Soil Ecol. 2007;37:202–14.View ArticleGoogle Scholar
- Preston-Mafham J, Boddy L, Randerson PF. Analysis of microbial community functional diversity using sole-carbon-source utilisation profiles–a critique. FEMS Microbiol Ecol. 2002;42:1–14.PubMedGoogle Scholar
- Neufeld JD, Vohra J, Dumont MG, Lueders T, Manefield M, Friedrich MW, Murrell JC. DNA stable-isotope probing. Nat Protoc. 2007;2:860.View ArticleGoogle Scholar
- Ihrmark K, Bödeker I, Cruz-Martinez K, Friberg H, Kubartova A, Schenck J, Strid Y, Stenlid J, Brandström-Durling M, Clemmensen KE. New primers to amplify the fungal ITS2 region–evaluation by 454-sequencing of artificial and natural communities. FEMS Microbiol Ecol. 2012;82:666–77.View ArticleGoogle Scholar
- Aronesty E. Comparison of sequencing utility programs. Open Bioinf J. 2013;7:1-8.View ArticleGoogle Scholar
- Nilsson RH, Veldre V, Hartmann M, Unterseher M, Amend A, Bergsten J, Kristiansson E, Ryberg M, Jumpponen A, Abarenkov K. An open source software package for automated extraction of ITS1 and ITS2 from fungal ITS sequences for use in high-throughput community assays and molecular ecology. Fungal Ecol. 2010;3:284–7.View ArticleGoogle Scholar
- Edgar RC. UPARSE: highly accurate OTU sequences from microbial amplicon reads. Nat Methods. 2013;10:996.View ArticleGoogle Scholar
- Méchin V, Damerval C, Zivy M. Total protein extraction with TCA-acetone. In: Thiellement H, Zivy M, Damerval C, Méchin V, editors. Plant proteomics. Totowa: Springer; 2007. p. 1–8.Google Scholar
- Love MI, Huber W, Anders S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 2014;15:550.View ArticleGoogle Scholar
- Zybailov B, Mosley AL, Sardiu ME, Coleman MK, Florens L, Washburn MP. Statistical analysis of membrane proteome expression changes in Saccharomyces c erevisiae. J Proteome Res. 2006;5:2339–47.View ArticleGoogle Scholar
- Robinson MD, McCarthy DJ, Smyth GK. edgeR: a bioconductor package for differential expression analysis of digital gene expression data. Bioinformatics. 2010;26:139–40.View ArticleGoogle Scholar
- Kammers K, Cole RN, Tiengwe C, Ruczinski I. Detecting significant changes in protein abundance. EuPA Open Proteomics. 2015;7:11–9.View ArticleGoogle Scholar
- Gatto L, Breckels LM, Naake T, Gibb S. Visualization of proteomics data using R and bioconductor. Proteomics. 2015;15:1375–89.View ArticleGoogle Scholar
- Vizcaíno JA, Csordas A, Del-Toro N, Dianes JA, Griss J, Lavidas I, Mayer G, Perez-Riverol Y, Reisinger F, Ternent T. 2016 update of the PRIDE database and its related tools. Nucleic Acids Res. 2015;44:D447–56.View ArticleGoogle Scholar