Bacteria from the endosphere and rhizosphere of Quercus spp. use mainly cell wall-associated enzymes to decompose organic matter.

Due to the ability of soil bacteria to solubilize minerals, fix N2 and mobilize nutrients entrapped in the organic matter, their role in nutrient turnover and plant fitness is of high relevance in forest ecosystems. Although several authors have already studied the organic matter decomposing enzymes produced by soil and plant root-interacting bacteria, most of the works did not account for the activity of cell wall-attached enzymes. Therefore, the enzyme deployment strategy of three bacterial collections (genera Luteibacter, Pseudomonas and Arthrobacter) associated with Quercus spp. roots was investigated by exploring both cell-bound and freely-released hydrolytic enzymes. We also studied the potential of these bacterial collections to produce enzymes involved in the transformation of plant and fungal biomass. Remarkably, the cell-associated enzymes accounted for the vast majority of the total activity detected among Luteibacter strains, suggesting that they could have developed a strategy to maintain the decomposition products in their vicinity, and therefore to reduce the diffusional losses of the products. The spectrum of the enzymes synthesized and the titres of activity were diverse among the three bacterial genera. While cellulolytic and hemicellulolytic enzymes were rather common among Luteibacter and Pseudomonas strains and less detected in Arthrobacter collection, the activity of lipase was widespread among all the tested strains. Our results indicate that a large fraction of the extracellular enzymatic activity is due to cell wall-attached enzymes for some bacteria, and that Quercus spp. root bacteria could contribute at different levels to carbon (C), phosphorus (P) and nitrogen (N) cycles.

Introduction

Globally, forests are considered relevant ecosystems since they provide essential environmental services; for instance, they contribute to the protection of biodiversity and soils [1]. Temperate deciduous forests contain approximately 0.66 trillion trees [2] and they represent a n class="Chemical">carbon (C) sinpan>k of high importanpan>ce, especially inpan> Europe, Asia anpan>d Northernpan> America [3]. Therefore, the funpan>ctionpan>inpan>g of these ecosystems has beenpan> a research topic of great inpan>terest for lonpan>g time. Forest microbiota–especially funpan>gal anpan>d bacterial communpan>ities onpan> planpan>t litter, deadwood, soil anpan>d rhizosphere–conpan>tributes to the homeostasis of forest ecosystem by decomposinpan>g dead biomass, mediatinpan>g the biogeochemical cycles anpan>d the nutrienpan>t turnpan>over, anpan>d inpan>teractinpan>g with their planpan>t hosts as symbionpan>ts or pathogenpan>s [4]. Although both saprotrophic anpan>d mycorrhizal funpan>gal communpan>ities dwellinpan>g inpan> forest soils have beenpan> studied exhaustively [5, 6], the knpan>owledge of the inpan>volvemenpan>t of bacteria inpan> forest ecosystem processes remainpan>s fragmenpan>tary [4].

The degradation of lignon class="Chemical">cellulose is a vital step inpan> the C cycle inpan> terrestrial ecosystems sinpan>ce planpan>t biomass is composed primarily of this complex mixture of pan> class="Chemical">biopolymers. Traditionally, fungi have been considered the main drivers of plant material decomposition [7], however there are progressively more works describing the potential contribution of bacteria to decomposition processes in forest litter and soils [8, 9]. Recently, Lladó et al. [10] described the ability of members of several bacterial phyla to degrade cellulose and hemicelluloses, which are the main non-polyphenolic constituents of lignocellulose. These authors revealed the important metabolic potential of Acidobacteria to degrade plant polysaccharides, while the cellulolytic ability of different bacterial genera isolated from a deciduous forest such as Mucilaginibacter, Pedobacter and Luteibacter was demonstrated in a genome- and proteome-based approach [11]. Several genera belonging to different orders of the phylum Actinobacteria (e.g. Streptomyces, Cellulomonas, Acidothermus, Thermobifida, Cellulosimicrobium, Micrococcus, Clavibacter, among others) [12-18] are also able to utilize complex biopolymers, namely cellulose or some types of hemicelluloses, although it has been suggested that this ability varies among strains [19]. Taken together, these results highlight the relevance of phylogenetically diverse bacteria in the global C cycle. Chitin is the second most abundant biopolymer on Earth just preceded by cellulose [20], as it is one of the main compounds of fungal cell walls and arthropod exoskeletons [21]. Many bacterial genera adscribed to different phyla are capable of producing chitinases to access the C and nitrogen (N) contained in this polymer, among which genera Streptomyces [22], Glycomyces, Cellulomonas, Actinoplanes, Actinokineospora, Kitasatospora, Nonomurea [23], Pseudomonas, Ewingella, Pedobacter, Variovorax, Stenotrophomonas and Chitinophaga are well known [24]. Thus, hydrolysis of chitin supposes a combination of an antagonism mechanism against soil fungi and a nutritional adaptation. Through the action of chitinases bacteria can degrade one of the main structural compounds of fungal cell wall during antagonistic interactions. However, the fact that bacteria are the most important decomposers of dead fungal mycelia [25] and N-acetalglucoasaminidase activity is increased during bacterial growth on this substrate [26] along with the fact that many bacteria feed on the final products of chitin decomposition, N-acetylglucosamine [10], indicate the nutritional role of chitin decomposition and the importance of chitinolytic bacteria in C and N cycles. Bacteria are also able to access one of the most limiting nutrients in many soils, phosphorus (P). As reviewed by Lladó et al. [4], members of several bacterial phyla dominated different processes related to P turnover, which include both the solubilization and uptake of inorganic P and the release of phosphate from organic sources through phosphatase enzymes. While these recent works shed some light on the activity of bacteria inhabiting litter and bulk soil, the information on bacterial inhabitants of the endospheres and rhizospheres of forest trees is scarce.

n class="Disease">Organic matter tranpan>sformationpan> by bacteria is mediated by extracellular enpan>zymes that are released inpan>to the soil or associated with the parenpan>t cell membranpan>e, either attached to or inpan>tegrated inpan>to it [27]. Onpan>ce free-diffusible enpan>zymes have beenpan> released inpan>to the surrounpan>dinpan>g enpan>vironpan>menpan>t, they face a set of hostile conpan>ditionpan>s [28]. Outside the cell, free enpan>zymes may be subjected to adsorptionpan>, inpan>activationpan> anpan>d degradationpan> by proteases [29]. Onpan> the other hanpan>d, free enpan>zymes may have higher probability to inpan>teract with their substrate [27]. While both cell-associated anpan>d free enpan>zymes genpan>erate products available to all soil microorganpan>isms, the producer cell has higher probability to access those produced close to its surface [30]. Furthermore, the fact that enpan>zymes oftenpan> conpan>tainpan> substrate-binpan>dinpan>g domainpan>s [11] may allow bacteria with cell-bounpan>d enpan>zymes to associate with their substrate, e.g. pan> class="Chemical">cellulose or other polysaccharides. As observed by Reintjes et al. [31] extracellular enzymes are produced preferentially as associated with cell membranes in marine bacteria, although the ecological relevance of the location of these enzymes has not been elucidated yet. In the rhizosphere–a highly competitive environment, especially in terms of nutrient uptake–those bacteria which have developed efficient nutritional strategies to compete against other microorganisms will likely become successful and proliferate. Thus, it could be expected that cell-bound enzymes will account for a large part of total activity in bacteria interacting with and having an effect on their plant hosts, such as rhizospheric and endospheric bacteria.

The aim of the present work was to characterize the ability of bacteria isolated from the rhizosphere and root endosphere of n class="Species">Quercus spp. trees to tranpan>sform pan> class="Disease">organic matter. Strains inhabiting the rhizosphere of burned Quercus ilex subsp. ballota and showing plant growth promotion traits were selected from a previous study [32], and those found in the root endosphere and rhizosphere of Quercus pyrenaica Willd. trees were also analysed. We tried to disentangle the contribution of both bacterial collections to forest ecosystem functionality by screening their ability to produce different enzymes involved in the C, N and P cycles. The spatial distribution of the extracellular enzymes with respect to producer cells was also assessed.

Materials and methods

Sample collection, bacterial isolation and identification

All bacterial strains characterized in this work were isolated from three different forests located in the Sierra Nevada National and Natural Park, in Southeast Spain. The Director of the Sierra Nevada National and Natural Park authorised the permission for the sampling. The field studies did not involve endangered or protected species. The geographic coordinates of each sampling location were N 36° 57’ 26”, W 3° 27’ 48” (BOF1); N 36° 57’ 11.2”, W 03° 26’ 21.0” (HAF1) and N 36° 58’ 23.4”, W 03° 24’ 36.4” (NPF1) (see S1 Table). The first site was covered by a holm oak (n class="Species">Quercus ilex subsp. ballota) forest located inpan> the valley of the Lanpan>jarón river, which was affected by a wildfire anpan>d where resproutinpan>g holm oak trees were founpan>d three years after the wildfire (BOF1, Burnpan>ed Oak Forest). Onpan> the other hanpan>d, two sites located inpan> the munpan>icipal district of Cáñar were selected: a natural, mature pan> class="Species">Quercus pyrenaica Willd. (melojo oak) forest located at the Higher Altitudinal limit of the Forest (HAF1) and another covered by a Scots pine (Pinus sylvestris) forest which was thinned out and naturalized with melojo oak plantlets in 2013 (NPF1, Naturalized Pine Forest). In each site, three trees with a diameter of at least 15 cm at breast height (in the case of BOF1 and HAF1 sites) and separated by more than 5 m were selected. BOF1 and HAF1 were the same sites described in a previous work [33, 34], and the positions of all the experimental areas were recorded with the Global Positioning System and are summarised in S1 Table.

Rhizospheric soil samples from holm oak (BOF1) and n class="Chemical">melojo oak trees (HAF1) were collected inpan> previous works [33, 35]. Briefly, rhizospheric soil samples were takenpan> by followinpan>g the mainpan> roots unpan>til younpan>g cork-free roots were founpan>d, at a distanpan>ce of approximately less thanpan> 50 cm from the trunpan>k. To avoid the samplinpan>g of nonpan>-rhizospheric soil, the leaf litter from topsoil anpan>d minpan>or roots from herbaceous planpan>ts were discarded collectinpan>g rhizospheric samples at depths from 5 to 25 cm. Samples cominpan>g from the three trees corresponpan>dinpan>g to the same site were mixed anpan>d sieved through a 2 mm mesh, anpan>d stored immediately at -80°C unpan>til processinpan>g them. Isolationpan> anpan>d characterizationpan> of bacteria from holm oak rhizosphere was previously described by Fernpan>ández-Gonpan>zález et al. [32]. Isolationpan> of bacteria inpan>habitinpan>g the rhizosphere of pan> class="Chemical">melojo oak trees was performed with an initial pre-enrichment step where 5 g of soil obtained from melojo oak were resuspended in 50 mL mineral salts medium [36] supplemented with antipyrin, pyramidon, phenylalanine or tannic acid at a final concentration of 0.4%. After an incubation on a rotatory shaker for 7 days at 30°C, the biggest soil particles were removed. Afterwards, 100 μL of this soil suspension and the corresponding serial dilutions up to 10−7 were spread onto solid mineral salts medium supplemented with each of the aforementioned carbon sources. All the Petri dishes were incubated for 10 days at 30°C.

Endophytic bacteria were obtained from five n class="Chemical">melojo oak trees that were uprooted from NPF1 site two years after their planpan>tinpan>g. The roots were washed with pan> class="Chemical">water and ethanol and then put into clear plastic bags and conserved at 4°C until its processing. Roots from each tree were vigorously washed with tap water to remove the biggest soil particles attached to them and subsequently rinsed with distilled water. Afterwards, the young cork-free roots of each tree were cut into small pieces (roughly 5 cm of length) and surface sterilized for 1 min in ethanol 96%, 15 min in a solution containing 5% sodium hypochlorite, and 30 seconds in ethanol 96%. After rinsing the roots five times with sterile distilled water and cutting them into 5 mm pieces, 10 fragments were plated on YEM (Yeast Extract Mannitol) and TSA (Tryptic Soy Agar; Bacto, BD) solid media to verify the efficiency of the sterilization. On the other hand, 0.2 g of the remaining root material were soaked in liquid nitrogen and immediately ground for 6 min with the help of sterilized grinding balls (5 mm diameter) by using the grinder MM 031 (Retsch, Germany) at 30 Hz. The obtained root powder was mixed with 500 μL 20 mM phosphate buffer, and after a centrifugation step (2 min, 6 000 x g) 100 μL of each suspension was plated on YEM and TSA media in triplicate. All the plates–including those containing the sterilized roots–were incubated at 30°C for 7 days. The isolation of melojo oak bacterial endophytes was performed separately for each sampled tree.

The identification of those strains isolated from the rhizosphere of holm oak and n class="Chemical">melojo oak trees was performed previously by Fernpan>ández-Gonpan>zález et al. [32] anpan>d Lasa et al., (unpan>published), respectively, while enpan>dospheric strainpan>s were idenpan>tified inpan> this work. Briefly, inpan> the case of the strainpan>s isolated from holm oak rhizosphere, the genpan>omic DNA was obtainpan>ed by suspenpan>dinpan>g bacterial colonpan>ies inpan> 100 μL sterile distilled pan> class="Chemical">water and heating them at 96°C for 10 min in a dry block heater. DNA of strains obtained from melojo oak trees (rhizo- and endosphere) was obtained after cultivating them in TSA and YEM liquid media, respectively, and by using the RealPure genomic DNA extraction kit (Durviz, S.L.U.,Valencia, Spain) and the corresponding manufacturer’s instructions. In all cases, isolated DNA was used as a template in PCR reactions to amplify the almost complete bacterial rrs gene by using the universal primers 9bfm [37] and 1512UR [38]. The specific PCR conditions were as follows: an initial denaturation step at 94°C for 4 min, 25 cycles of denaturation at 94°C for 1 min, primer annealing at 52°C for 1 min and extension at 72°C for 1.5 min, followed by a final step of heating at 72°C for 10 min. PCR products of the expected size were partially sequenced as described by Rivas et al., [39] on an ABI PRISM 3130xl Genetic Analyzer using a BigDye Terminator v3.1 Cycle Sequencing kit (Applied Biosystems Inc., USA) as recommended by the supplier. Obtained sequences were manually edited with the software Sequence Scanner v1.0 (Applied Biosystems, MA, EEUU) and compared against those sequences held in GenBank database through a BLASTn search https://blast.ncbi.nlm.nih.gov.

Among all the isolated strains, three bacterial collections were further analysed: the first, composed of 12 strains affiliated with genus n class="Species">Arthrobacter isolated from the rhizosphere of holm oak trees of which five may be keystonpan>e species inpan> the recovery of burnpan>ed holm oak forests, as demonpan>strated previously by their planpan>t growth promotionpan> ability [32]. 44 isolates belonpan>ginpan>g to genpan>us Pseudomonpan>as were also selected due to the relevanpan>ce of family Pseudomonpan>adaceae as onpan>e of the most potenpan>tially active taxa of pan> class="Species">Q. pyrenaica’s microbiota [35].The plant growth promoting traits and the ability to tolerate tannic acid in vitro of these strains led us to select them (Lasa et al., unpublished). On the other hand, among melojo oak root endophytes, 17 isolates of the genus Luteibacter were selected since it was the most abundantly isolated genus.

Enzyme production of the selected bacterial strains

Since it is impossible to analyse enzyme production by individual bacterial strains directly in their environment (endosphere or rhizosphere), the 73 bacterial strains were cultivated on liquid Malt Extract medium (malt extract, 20 g L-1; 20 mL in 100-mL Erlenmeyer flasks). Malt extract was selected since it contains nutrients of plant origin that are relevant in the rhizosphere and endosphere of plant roots and in the soil including n class="Chemical">cellulose- anpan>d pan> class="Chemical">hemicellulose-derived oligosaccharides [40, 41]. Due to this, it was demonstrated to efficiently induce production of cellulases and hemicellulases in a wide range of bacteria, including Proteobacteria, Bacteroidetes, Actinobacteria but also in fungi [11, 19, 42–44]. Media containing long-chain polysaccharides had to be avoided since these are impossible to separate from bacterial cells and thus not suitable for detection and quantification of the cell wall-associated enzymes [44].

For each bacterial strain, triplicate flasks were inoculated with 200 μL of the corresponding inoculum previously adjusted to an optical density at a wavelength of 600 nm of 0.1, and incubated at 25°C on a rotatory shaker (200 rpm). After seven days, 10 mL of each bacterial culture were harvested and mixed, and the composite cultures were centrifuged for 3 minutes at 11 357 g. Moreover, after seven days all bacteria were at stationary phase of growth. Activity of cell-bound and free fractions of enzymes was determined as described previously [44]. Bacterial cells were washed twice with n class="Chemical">sodium acetate buffer (50 mM, pH 5.0) anpan>d resuspenpan>ded inpan> 20 mL of the same buffer. The culture supernpan>atanpan>t was retainpan>ed as well anpan>d its pH was adjusted by addinpan>g 10 mL of 50 mM pan> class="Chemical">acetate buffer, pH 5.0. Both cell fraction and culture supernatants were used to measure the activity of cell-attached and free enzymes, respectively.

The enzymatic activity of several enzymes that are relevant for nutrient cycling in forest ecosystems were studied in this work. Concretely, we assayed a collection of enzymes involved in the transformation of n class="Disease">organic matter. The measuremenpan>t of enpan>zymatic activity was performed by usinpan>g methylumberiferoll (MUF)-based fluorescenpan>t substrates as described by Baldrianpan> [45] for the followinpan>g enpan>zymes: cellobiohydrolase (exocellulase, EC 3.2.1.91), β-glucosidase (EC 3.2.1.21), α-glucosidase (EC 3.2.1.20), β-xylosidase (EC 3.2.1.37), n class="Chemical">chitinase (EC 3.2.1.14), phosphomonoesterase (acid phosphatase, EC 3.1.3.2). The activities of α-galactosidase (EC 3.2.1.22), β-galactosidase (EC 3.2.1.23), β-glucuronidase (EC 3.2.1.31), β-mannosidase (EC 3.2.1.25), α-arabinosidase (EC 3.2.1.55) and lipase (EC 3.1.1.3) were assessed using 4-methylumbeliyferyl-α-D-galactopyranoside, 4-methylumbeliyferyl-β-D-galactopyranoside, 4-methylumbeliyferyl-β-D-glucuronide, 4-methylumbeliyferyl-β-D-mannopyranoside, 4-methylumbeliyferyl-α-L-arabinopyranoside and 4-methylumbeliyferyl-caprylate substrates, respectively, and the same procedure. In brief, in all cases MUF-labelled substrates dissolved in DMSO at a final concentration of 500 μM were mixed with samples (200 μL), in triplicate, in multiwell plates. Plates were incubated at 40°C and the fluorescence was measured from 5 to 125 minutes on a microplate reader (Infinite, TECAN, Austria), by using an excitation wavelength of 355 nm and an emission wavelength of 460 nm. Three technical replicates were measured, and the quantification of the activities was based on standard curves of 4-methylumbelliferone added to the samples after blank subtraction.

Cell-bound and supernatant fractions were analysed separately and the enzymatic activities were expressed per mL of bacterial culture. Total enzymatic activities were calculated as the sum of the activity in both fractions. The detection limit was 10 nM min-1 mL-1 and lower values were thus considered as a lack of activity.

Statistical analyses

All statistical analyses were performed using R software 3.4.3 version [46]. To check if the enzymatic activity of each bacterial genus follows a normal distribution, the Shapiro test was used by means of the function shapiro.test included in R. As the normality of the data was not met, the non-parametric Mann-Whitney U test was applied to test if there were significant differences among the activity of cell-bound and released enzymes for each bacterial genus, considering all the strains that belonged to the same genus (wilcox.test function of R). Confidence levels > 95% (α = 0.05) were taken into account for all the statistical tests.

Results

Comparison of the activity of cell-associated and released enzymes

73 bacterial strains isolated from the root endosphere of n class="Chemical">melojo oak trees as well as from the rhizosphere of the same host and holm oak trees were studied in this work. Based on the partial sequence of the 16S rRNA gene, these strains showed the highest similarity percentage with genera Luteibacter, Pseudomonas and n class="Species">Arthrobacter, respectively (S2 Table).

The production of enzymes involved in the degradation of n class="Chemical">cellulose, pan> class="Chemical">hemicelluloses and other polysaccharides, as well as in the degradation of compounds based on N and P (chitin and phosphate esters, respectively) was assayed in both cell-wall associated and supernatant fractions (Figs 1–3 and S3 Table). For genus Luteibacter, all studied enzymes were detected in at least one fraction, except for β-glucuronidase, which was not produced in detectable amount in any of the studied fractions (Fig 1 and S4 Table). Overall, the enzyme activity was recorded mostly in the cell-bound fraction: seven enzymes were detected exclusively as attached to cells, and more than 97.6% of total activity of acid phosphatase, β-mannosidase and β-glucosidase recorded for all Luteibacter strains was associated with cells (S4 Table). Acid phosphatase was released into culture liquid by all isolates, however, those strains exhibiting highest activity in the culture liquid still had more than 95% of activity associated with its cells (see S4 Table). It was noticeable that for those enzymes that were synthesized as both cell-bound and free for at least two strains (β-glucosidase, acid phosphatase and lipase), the activity recorded in the cell-attached fraction was significantly higher than that detected in culture liquid (Mann-Whitney U test, p-values < 0.028; S3 Table).

Fig 1

Activity of cell-associated and freely-released enzymes from genus Luteibacter.

Box and whiskers were represented in the style of Tukey. Hinges correspond to the 1st and 3th quartiles and medians of the activity of each enzyme recorded for all strains are represented by horizontal lines. Red points correspond to those data beyond 1.5 x Inter Quartile Range. An ‘*’ indicates significant differences between the activity of those enzymes detected in both fractions calculated with the non-parametric Mann-Whitney U test at a confidence level of 95%. Abbreviations of enzymes: bG: β-glucosidase; Pho: acid phosphatase; bX: β-xylosidase; bGal: β-galactosidase; CBH: cellobiohydrolase; aG: α-glucosidase; ChTN: chitinase; Lip: lipase; bGlu: β-glucuronidase; aA: α-arabinosidase; bM: β-mannosidase; aGal: α-galactosidase. All the data were log-transformed for graphical clarity by fitting the same scale.

Fig 3

Activity of cell-associated and freely-released enzymes from genus Arthrobacter.

Box and whiskers were represented in the style of Tukey. Hinges correspond to the 1st and 3th quartiles and medians of the activity of each enzyme recorded for all strains are represented by horizontal lines. Red points correspond to those data beyond 1.5 x Inter Quartile Range. No significant differences were detected between both fractions according to the non-parametric Mann-Whitney U test at a confidence level of 95%. Abbreviations of enzymes: bG: β-glucosidase; Pho: acid phosphatase; bX: β-xylosidase; bGal: β-galactosidase; CBH: cellobiohydrolase; aG: α-glucosidase; ChTN: chitinase; Lip: lipase; bGlu: β-glucuronidase; aA: α-arabinosidase; bM: β-mannosidase; aGal: α-galactosidase. All the data were log-transformed for graphical clarity by fitting the same scale.

Box and whiskers were represented in the style of Tukey. Hinges correspond to the 1st and 3th quartiles and medians of the activity of each enzyme recorded for all strains are represented by horizontal lines. Red points correspond to those data beyond 1.5 x Inter Quartile Range. An ‘*’ indicates significant differences between the activity of those enzymes detected in both fractions calculated with the non-parametric Mann-Whitney U test at a confidence level of 95%. Abbreviations of enzymes: bG: β-glucosidase; Pho: acid phosphatase; bX: β-xylosidase; bGal: β-galactosidase; CBH: cellobiohydrolase; aG: α-glucosidase; ChTN: n class="Chemical">chitinase; Lip: lipase; bGlu: β-glucuronpan>idase; aA: α-arabinpan>osidase; bM: β-manpan>nosidase; aGal: α-galactosidase. All the data were log-tranpan>sformed for graphical clarity by fittinpan>g the same scale.

Box and whiskers were represented in the style of Tukey. Hinges correspond to the 1st and 3th quartiles and medians of the activity of each enzyme recorded for all strains are represented by horizontal lines. Red points correspond to those data beyond 1.5 x Inter Quartile Range. An ‘*’ indicates significant differences between the activity of those enzymes detected in both fractions calculated with the non-parametric Mann-Whitney U test at a confidence level of 95%. Abbreviations of enzymes: bG: β-glucosidase; Pho: acid phosphatase; bX: β-xylosidase; bGal: β-galactosidase; CBH: cellobiohydrolase; aG: α-glucosidase; ChTN: n class="Chemical">chitinase; Lip: lipase; bGlu: β-glucuronpan>idase; aA: α-arabinpan>osidase; bM: β-manpan>nosidase; aGal: α-galactosidase. All the data were log-tranpan>sformed for graphical clarity by fittinpan>g the same scale.

Box and whiskers were represented in the style of Tukey. Hinges correspond to the 1st and 3th quartiles and medians of the activity of each enzyme recorded for all strains are represented by horizontal lines. Red points correspond to those data beyond 1.5 x Inter Quartile Range. No significant differences were detected between both fractions according to the non-parametric Mann-Whitney U test at a confidence level of 95%. Abbreviations of enzymes: bG: β-glucosidase; Pho: acid phosphatase; bX: β-xylosidase; bGal: β-galactosidase; CBH: cellobiohydrolase; aG: α-glucosidase; ChTN: n class="Chemical">chitinase; Lip: lipase; bGlu: β-glucuronpan>idase; aA: α-arabinpan>osidase; bM: β-manpan>nosidase; aGal: α-galactosidase. All the data were log-tranpan>sformed for graphical clarity by fittinpan>g the same scale.

The enzyme deployment strategy of Pseudomonas strains was not as definite as that of Luteibacter strains. On the one hand, five out of 12 enzymes were exclusively detected in the supernatant of Pseudomonas cultures (namely α-arabinosidase, β-galactosidase, n class="Chemical">chitinase, α-galactosidase anpan>d β-glucuronpan>idase, Fig 2 anpan>d S3 Table). β-Manpan>nosidase, exocellulase, β-xylosidase anpan>d α-glucosidase were synpan>thesized inpan> both fractionpan>s by just few strainpan>s, while the activity detected inpan> the cell-associated fractionpan> was conpan>siderable low (at most, 57.4% of the total activity of β-xylosidase inpan> cell-bounpan>d fractionpan> of strainpan> p24; see S5 Table). Onpan> the other hanpan>d, signpan>ificanpan>t differenpan>ces betweenpan> the activity of cell-associated anpan>d free enpan>zymes were observed onpan>ly for acid phosphatase anpan>d lipase, beinpan>g the titres of both enpan>zymes higher inpan> the cell-bounpan>d fractionpan> (S3 Table).

Fig 2

Activity of cell-associated and freely-released enzymes from genus Pseudomonas.

Box and whiskers were represented in the style of Tukey. Hinges correspond to the 1st and 3th quartiles and medians of the activity of each enzyme recorded for all strains are represented by horizontal lines. Red points correspond to those data beyond 1.5 x Inter Quartile Range. An ‘*’ indicates significant differences between the activity of those enzymes detected in both fractions calculated with the non-parametric Mann-Whitney U test at a confidence level of 95%. Abbreviations of enzymes: bG: β-glucosidase; Pho: acid phosphatase; bX: β-xylosidase; bGal: β-galactosidase; CBH: cellobiohydrolase; aG: α-glucosidase; ChTN: chitinase; Lip: lipase; bGlu: β-glucuronidase; aA: α-arabinosidase; bM: β-mannosidase; aGal: α-galactosidase. All the data were log-transformed for graphical clarity by fitting the same scale.

β-Mannosidase and exocellulase were not recorded at detectable levels in any of the n class="Species">Arthrobacter isolates tested. Although α-glucosidase, α-galactosidase anpan>d β-glucuronpan>idase were produced exclusively as free-diffusible enpan>zymes, less thanpan> 6.5% of the total activity of phosphatase anpan>d n class="Chemical">chitinase recorded for this genus was found in the culture liquid (S6 Table). α-Arabinosidase was the only enzyme which was found specifically in association with cells (S6 Table).

Enzyme production potential of bacterial isolates

None of the Luteibacter isolates was able to produce β-glucuronidase and only 6 isolates were able to produce n class="Chemical">chitinase, however all the remainpan>inpan>g enpan>zymes were expressed by more thanpan> 94% isolates (Fig 4A). The enpan>zyme productionpan> ability of those strainpan>s isolated from the root enpan>dosphere of pan> class="Species">Q. pyrenaica was noteworthy. Even for the least active strain L14 75% of assayed enzymes were detected. As shown in Fig 4B, 16 out of 17 isolates synthesized at least 10 enzymes, which resulted in an expression of roughly 86% of the tested enzymes on average. By contrast, the mean production of the isolates belonging to genus Pseudomonas did not exceed 33% of the enzymes assayed. Only a few strains contributed to a wide variety of enzymes, thus, just eight out 44 isolates were able to produce more than one third of the enzymes tested here (Fig 4B). Indeed, only five isolates (p20, p23, p34, p49, p54) were able to synthesize all the assayed enzymes, exhibiting the wider and more diverse range of enzymes produced (Fig 5). Nevertheless, these strains showed moderately low activity of all enzymes except for lipase, acid phosphatase, and β-glucosidase in some cases (S5 Table). On the other hand, any isolate belonging to Arthrobacter bacterial collection had the ability to produce all the enzymes, and those three isolates expressing more than a half of the assayed enzymes, produced seven enzymes at most (Fig 4B).

Fig 4

Relationship of the number of enzymatic activities and bacterial strains.

(a) Percentage of Luteibacter, Pseudomonas and Arthrobacter strains exhibiting different enzymatic activities. (b) Enzymatic specialization of Luteibacter, Pseudomonas and Arthrobacter strains. The degree of specialization of each genus was measured as the total amount of strains producing different number of enzymes in liquid cultures. Abbreviations of enzymes: aA: α-arabinosidase; aG: α-glucosidase; aGal: α-galactosidase; CBH: cellobiohydrolase; bG: β-glucosidase; bGal: β-galactosidase; bM: β-mannosidase; ChTN: chitinase; Pho: acid phosphatase; bGlu: β-glucuronidase; bX: β-xylosidase; Lip: lipase.

Fig 5

Enzymatic profiles of Luteibacter Pseudomonas and Arthrobacter strains.

Data represent means of the total activity of three replicates and were log-transformed to fit the same scale. The clustering was constructed by using UPGMA algorithm based on Euclidean distances. Bacterial genera are colour-coded. Abbreviations of enzymes: Pho: acid phosphatase; Lip: lipase; ChTN: chitinase; bGlu: β-glucuronidase; bG: β-glucosidase; aA: α-arabinosidase; CBH: cellobiohydrolase; bX: β-xylosidase; bM: β-mannosidase; aGal: α-galactosidase; aG: α-glucosidase; bGal: β-galactosidase.

(a) Percentage of Luteibacter, Pseudomonas and n class="Species">Arthrobacter strainpan>s exhibitinpan>g differenpan>t enpan>zymatic activities. (b) Enpan>zymatic specializationpan> of Luteibacter, Pseudomonpan>as anpan>d pan> class="Species">Arthrobacter strains. The degree of specialization of each genus was measured as the total amount of strains producing different number of enzymes in liquid cultures. Abbreviations of enzymes: aA: α-arabinosidase; aG: α-glucosidase; aGal: α-galactosidase; CBH: cellobiohydrolase; bG: β-glucosidase; bGal: β-galactosidase; bM: β-mannosidase; ChTN: chitinase; Pho: acid phosphatase; bGlu: β-glucuronidase; bX: β-xylosidase; Lip: lipase.

Data represent means of the total activity of three replicates and were log-transformed to fit the same scale. The clustering was constructed by using UPGMA algorithm based on Euclidean distances. Bacterial genera are colour-coded. Abbreviations of enzymes: Pho: acid phosphatase; Lip: lipase; ChTN: n class="Chemical">chitinase; bGlu: β-glucuronpan>idase; bG: β-glucosidase; aA: α-arabinpan>osidase; CBH: cellobiohydrolase; bX: β-xylosidase; bM: β-manpan>nosidase; aGal: α-galactosidase; aG: α-glucosidase; bGal: β-galactosidase.

Although six Luteibacter strains were able to produce n class="Chemical">chitinase, its activity was close to the detectionpan> limit inpan> all cases. Inpan> this senpan>se, a low meanpan> activity was also recorded for α-arabinpan>osidase, yet it was commonpan>ly founpan>d amonpan>g the isolates belonpan>ginpan>g to this genpan>us (S4 Table). With the exceptionpan> of the abovemenpan>tionpan>ed enpan>zyme, other enpan>zymes inpan>volved inpan> the decompositionpan> of pan> class="Chemical">hemicellulose and also cellulose-degrading cellobiohydrolase were rather common and active in Luteibacter collection, specially β-galactosidase and β-mannosidase (S4 Table). Lipase, acid phosphatase and β-glucosidase exhibited the highest activities, as was observed for Pseudomonas collection. However, the latter was more rare among Pseudomonas isolates, being produced by approximately 50% of all of them. α-arabinosidase, exocellulase, β-galactosidase, β-mannosidase, chitinase, β-glucuronidase and β-xylosidase were expressed by less than 20% of Pseudomonas isolates (Fig 4A) and, besides, their activity was scarcely detected for most of the producing isolates. A lack of activity was reported for exocellulase and β-mannosidase among all the strains affiliated with genus Arthrobacter. Overall, typically low activity levels were detected for most of the enzymes and strains, even for acid phosphatase. Strikingly, the activity of this enzyme was on average around 88.5 and 64 times lower than that recorded for Luteibacter and Pseudomonas isolates, respectively. Again, lipase was the enzyme which on average exhibited the higher activity. It should be noted that this enzyme was the most widespread among the 73 strains studied; indeed, it was synthesized by all of them (Fig 4A).

Discussion

Many attempts have been made in the past to gain more insights into the functionality of microorganisms in forest ecosystems, especially regarding fungal communities [47-49]. However, few efforts have been channelled towards nutrient cycles driven by cell-bound enzymes of soil bacteria. In this study, the role of 73 bacterial isolates in different ecosystem processes is reported by assessing the activity of cell-associated and free-diffusible enzymes involved in C, N and P cycles. The bulk of Luteibacter’s total activity (nearly 96.5% on average) was recorded in cell-bound fraction, and although the mean percentage of activity associated to cell-walls in Pseudomonas and n class="Species">Arthrobacter collectionpan>s was lower (19.6 anpan>d 44.1%, S5 anpan>d S6 Tables, respectively), it was far from negligible. These results conpan>firmed our mainpan> hypothesis, inpan>dicatinpan>g the potenpan>tial ability of the tested planpan>t-associated bacteria to synpan>thesize cell-associated enpan>zymes. Although the productionpan> of cell-bounpan>d associated enpan>zymes was mostly observed inpan> the case of those strainpan>s isolated from pan> class="Chemical">melojo oak root endosphere (genus Luteibacter), we cannot conclude whether this pattern is explained by the endophytic origin of these strains or if it is a phenomenon associated to some specific genera. Differences in terms of extracellular enzymatic profiles have been previously observed for different species belonging even to the same genus, namely Sphingomonas and Burkholderia [10], so diverse enzyme deployment strategies could be expected among different bacterial genera. In order to address if the different location of extracellular enzymes is owing to the taxonomical diversity, further experiments including more number of endospheric and rhizospheric taxonomically diverse bacterial genera should be performed. In addition, since the resolution of the 16S rRNA gene sequence at intrageneric level is low [50]–especially for genus Pseudomonas–the correlation between enzyme deployment strategy and the taxonomy at species level is difficult to unravel. Thus, here we demonstrated that by ignoring the cell-wall associated enzymatic fraction, the total contribution of certain bacteria to organic matter decomposition could be underestimated.

Due to the location of the enzymes in the cell surface the degradation products are likely to remain in the vicinity of the producer cells, which could result in a reduction of the diffusional losses of the nutrients. By lessening the diffusion of hydrolysis products, the ‘cheating’ behaviour of those microorganisms which can intercept these products without producing extracellular enzymes could be mitigated or reduced [51]. As a result, the attachment of hydrolytic enzymes to cell walls could make its biosynthesis a more energetically cost-efficient process, and could represent an efficient nutritional strategy. Besides the nutritional implications of cell-bound enzymes for bacteria, activities associated with cell-walls result in a localized effect upon plant hosts. In the case of plant biomass degrading enzymes expressed by endophytes, the cell-bound location can restrain a generalized degradative process of host’s roots, thereby avoiding a boundless hydrolysis of plant tissues but allowing these bacteria a localized penetration into the host [52].

It is difficult to say how large is the fraction of cell-associated enzymes among other groups of bacteria or among microorganisms in general due to an almost total lack of data. The fact that high activity of free enzymes was detected in cultures of certain cellulolytic bacteria [11, 53] and n class="Disease">soil Actinobacteria [19] inpan>dicates that the free fractionpan> of enpan>zymes canpan> be relatively large. Inpan> the case of the highly active soil pan> class="Chemical">cellulose decomposer Paenibacillus, that efficiently degrades crystalline cellulose [53], it can be anticipated that its endocellulases attacking the crystalline domains of cellulose fibrils need to be freely mobile in order to access their substrate. In the screening of forest soil bacteria, Actinobacteria showed high enzyme production in culture while the values of Proteobacteria were low [10] which might indicate either low production, or association of enzymes with cells that was not tested in that case. For filamentous fungi that are able to cover decomposed substrates with their mycelia and thus ensure efficient capture of reaction products liberated by free enzymes, high activities of enzymes are typically found as free in their cultures [43]. There is, however, some evidence that some share of the total activity is still associated with mycelia [54]. In the case of yeasts, the majority of enzyme activity is associated with cells [44]. Due to their unicellularity, cell-association of enzymes may give them the same advantages as seen for bacteria. The question about the share of cell-bound activity in fungi, remains, however, undisclosed.

The activity of those enzymes involved in the breakdown of n class="Chemical">polysaccharides was almost exclusively detected as cell-associated inpan> strainpan>s affiliated with genpan>us Luteibacter; onpan>ly three isolates expressed free β-manpan>nosidase anpan>d β-glucosidase anpan>d the activity of these enpan>zymes was residual inpan> culture liquid. These observationpan>s were not unpan>expected sinpan>ce polysaccharases are oftenpan> founpan>d as cell-associated enpan>zymes [29]. Microbes have evolved several mechanpan>isms to binpan>d pan> class="Chemical">polysaccharides, such as carbohydrate binding modules included in cellulases and hemicellulases, and protruding structures like type IV pili. The latter mediate the adherence to cellulose in Fibrobacter and Ruminococcus species [55, 56], and it has been reported more recently in a cellulolytic Luteibacter strain isolated from the litter of a Quercus petrea forest [11]. Besides type IV pili, these authors also described the presence of glycoside hydrolases containing carbohydrate binding modules in the proteome of that Luteibacter strain. Taking into consideration our results and the adaptations to retain substrates in their proximity, we can speculate that the genus Luteibacter may have developed different strategies to improve nutrient acquisition, for instance by reducing the nutrient sharing with other bacteria. Moreover, the presence of decomposition products released by free enzymes could attract other bacteria, as occurred with root wounds [57]. Therefore, cell-associated enzymes could represent an adaptation developed by endophytic strains here studied belonging to genus Luteibacter to avoid such attraction of competitors to the root entry point. Notwithstanding the above, the importance of cell-wall attached enzymes of strains affiliated with this genus remains unclear and needs to be further explored to gain more insight about their physiology and ecology.

In addition to n class="Chemical">polysaccharide hydrolases, other hydrolases like lipase anpan>d acid phosphatase were synpan>thesized as cell-attached inpan> conpan>siderable proportionpan>s inpan> all the Luteibacter, Pseudomonpan>as anpan>d pan> class="Species">Arthrobacter collections. The production of these enzymes bound to cell-walls seems to be a widely distributed trait, since it has been previously observed in phylogenetically divergent microorganisms such as bacterial genera Burkholderia (class β-Proteobacteria) [58] and Clostridium (phylum Firmicutes) [59], and even in forest yeasts [44].

The location of the enzymes relative to parent cells could not always be certain but variable. Pseudomonas and n class="Species">Arthrobacter isolates did not show a productionpan> patternpan> as Luteibacter did. The activity of some enpan>zymes was conpan>siderably high inpan> cell-bounpan>d fractionpan> for Pseudomonpan>as anpan>d pan> class="Species">Arthrobacter isolates, representing more than 62 and 71% of the total activity, respectively (S5 and S6 Tables). However, freely-released enzymes ranged from 29.5 to 100% of the total activity in genus Pseudomonas whereas some enzymes were produced exclusively as free and other even not detected among Arthrobacter isolates. Although it has been already demonstrated that cell-associated enzymes accounted for the main part of total enzymatic activity in aquatic ecosystems, the contribution of free-diffusible enzymes is generally regarded as highly variable [27]. Many studies agree that the contribution of secreted enzymes relies on environmental factors even on different substrates [60, 61] and it should be pointed out that the location of hydrolytic enzymes varies across the time, life stage and from enzyme to enzyme [29] as observed here. Although free-enzymes suppose the diffusion and dilution of hydrolysis products from parent cells, other microbes could take advantage of this situation. The so-called ‘cheaters’ could grasp that soluble products, therefore, the expression of cell-free enzymes may exert a beneficial effect at community level. Thus, we suggest that some Pseudomonas and Arthrobacter isolates may have a syntrophic relationship with other microbial members in Quercus spp. rhizosphere, however we cannot define the specific role of those enzymes just with the results obtained in this work.

Traditionally, the enzyme location with respect to the producer cell has been overlooked when studying extracellular enzymes of soil microorganisms. Notwithstanding, it has allowed us to assess the contribution of bacteria that produced only cell-bound enzymes otherwise would not have been measured, especially in the case of those isolated affiliated with genus Luteibacter. By studying both locations and taking into account a historically almost ignored enzyme location for many soil bacteria (cell-bound attached fraction), the potential involvement of each genus in nutrient turnover was determined. Overall, Pseudomonas and n class="Species">Arthrobacter isolates showed a moderated ranpan>ge of enpan>zymes produced anpan>d relatively low levels of enpan>zymatic activity, which inpan>dicates that most of the isolates of these genpan>era have the potenpan>tial to conpan>tribute to a limited soil processes to a greater or lesser extenpan>t.

Effective n class="Chemical">cellulose degradationpan> typically relies onpan> exocellulase (cellobiohydrolase) anpan>d β-glucosidase, which yields pan> class="Chemical">glucose from cellobiose (a product of cellulose hydrolysis). Pseudomonas p23 and all Luteibacter isolates exhibited high activity not only of β-glucosidase, but also of exocellulose, which catalyzes the rate-limiting step of cellulose deconstruction, suggesting these strains are truly involved in the decomposition of this polymer. Berlemont and Martiny [62] reported in a genome-based approach that both genes encoding exocellulases and β-glucosidases were distributed in 24% of all bacterial genomes, and the majority of the lineages (56%) encoded only genes for β-glucosidases in terms of cellulose hydrolysis. Our results are partially in accordance with these observations: the expression of both exocellulase and β-glucosidase was moderately common among isolates (31.5%), however the proportion of strains exhibiting exclusively β-glucosidase activity only reached half of the predicted value, probably because gene content does not necessarily mean gene expression. Those isolates producing only β-glucosidase could be considered opportunistic bacteria since they could be taking advantage of the cellobiose generated by exocellulase producing microorganisms. Therefore, our results suggest that Luteibacter and several Pseudomonas isolates may be cellulolytic bacteria, either as truly decomposers or as opportunistics. Actinobacteria are generally considered as an important phylum in cellulose degradation in forest soils [4, 63], and although only few lineages are able to degrade this polymer, cellobiose utilization is rather common in this phylum. Indeed, only 20% of actinobacterial genomes do not contain genes encoding any enzyme involved in cellulose degradation [62]. In spite of the fact that the cellulolytic capability of some strains affiliated with genus Arthrobacter have already been described [64], our isolates did not produce exocellulase and only three isolates exhibited very low β-glucosidase activity. It is possible that many strains harbouring exocellulase and β-glucosidase genes do not express them or that Arthrobacter isolates studied here represent an exception in cellulose degradation.

Although the genus Luteibacter is not well characterized yet and some authors have previously reported that strains isolated from a terrestrial lichen are not even able to produce β-glucosidase [65], recently it has been described as cellulolytic [11]. These authors reported its ability to degrade also n class="Chemical">hemicellulose anpan>d detected differenpan>t pan> class="Chemical">hemicellulose-degrading proteins in its proteome. As shown in S4 Table, Luteibacter isolates resulted active producers of hemicellulose degrading enzymes, specially β-mannosidase and β-galactosidase, thereby agreeing with the observations of López-Mondéjar et al. [11]. It is worth noting the diversified enzymatic competence exhibited by Luteibacter isolates which indicates these endophytes are not specialized decomposers and have evolved a diverse enzymatic system. This set of different but complementary enzymes could act synergistically and contribute altogether to a more efficient hydrolysis of plant cell wall compounds. Extracellular enzymes involved in plant cell wall degradation (e.g. cellulases, hemicellulases, xylanases, pectinases, polygalacturonases, amylases) are commonly synthesized by endophytic bacteria to penetrate in plant tissues [66, 67]. Other bacterial taxa isolated from root endosphere of cotton or even mangrove trees have the ability to produce a wide variety of enzymes which aid these endophytes in penetrating plant roots [57, 68]. Therefore, it would not be striking that the expression of cellulases and hemicellulases observed for Luteibacter was related to its endophytic origin; nevertheless additional confirmatory experiments should be performed to clarify the concrete role of these enzymes for those strains.

The production of acid phosphatase was common for all isolates studied here. According to Bergkemper and colleagues [69], phylogenetically diverse bacteria were commonly involved in n class="Disease">P turnover inpan> temperate forest soils, amonpan>g which order Xhanpan>tomonpan>adales (to which genpan>us Luteibacter belonpan>gs) dominpan>ated the expressionpan> of acid phosphatase. Lladó et al. [10] also reported high activity levels of this enpan>zyme for isolates belonpan>ginpan>g to differenpan>t phyla inpan> a conpan>iferous forest, while several Pseudomonpan>as species are well-knpan>ownpan> for their role inpan> the release of pan> class="Chemical">phosphate in a wide variety of agricultural soils. Arthrobacter nanjingensis is another example of a bacterium isolated from forest environment which also showed acid phosphatase activity [70], thereby highlighting the theoretical important role of these taxa in P turnover.

Conclusions

So far, enzymes bound to cells have rarely been studied in detail in soil bacteria. As reported here, the activity of enzymes attached to cells involved in n class="Disease">organic matter decompositionpan> canpan> suppose a substanpan>tial part of their total extracellular enpan>zymatic activity; inpan>deed, for some strainpan>s they canpan> be detected exclusively bounpan>d to cells. Our results suggested that measurinpan>g onpan>ly freely diffusible enpan>zymes, the total enpan>zymatic potenpan>tial of manpan>y root-associated bacteria could be unpan>derestimated. Henpan>ce, here we suggest takinpan>g heed of cell-bounpan>d fractionpan> for further anpan>alyses so that the inpan>volvemenpan>t of bacteria inpan> nutrienpan>t cyclinpan>g processes mediated by extracellular enpan>zymes could be described inpan> a more reliable way. By studyinpan>g both fractionpan>s, we have beenpan> able to describe the potenpan>tial of Luteibacter isolates as cellulolytic anpan>d hemicellulolytic bacteria, whereas the potenpan>tial conpan>tributionpan> of genpan>era Pseudomonpan>as anpan>d pan> class="Species">Arthrobacter to plant biomass decomposition processes was moderate and subtle, respectively. In short, our results reflected different ecological significance of both three genera in terms of C, N and P cycling, and pointed out the importance of measured cell-bound enzymes.

Position and main characteristics of the experimental areas.

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Identification of the strains studied based on their partial 16S rRNA gene sequence.

The identity of the closest hit for each strain is indicated, and in some cases, several hits are reported for those strains which showed the same similarity percentage with different species.

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Activity of cell-wall bound and freely-released enzymes produced by genera Luteibacter, Pseudomonas and Arthrobacter isolated from the root endosphere or the rhizosphere of Quercus spp. trees.

Data represent means and standard deviations of activities of those enzymes produced by two or more strains. A ‘-’ indicates values below detection limit. An ‘*’ indicates values that were recorded just for one strain, the one which is shown in parentheses. Abbreviations of enzymes: bG: β-glucosidase; Pho: acid phosphatase; Lip: lipase; bM: β-mannosidase; aA: α-arabinosidase; bX: β-xylosidase; bGal: β-galactosidase; CBH: cellobiohydrolase; aG: α-glucosidase; ChTN: n class="Chemical">chitinase; aGal: α-galactosidase; bGlu: β-glucuronpan>idase. For each bacterial genpan>us, signpan>ificanpan>t differenpan>ces betweenpan> the activity of those enpan>zymes detected inpan> both fractionpan>s were calculated by usinpan>g the nonpan>-parametric Manpan>n-Whitnpan>ey U test at a conpan>fidenpan>ce level of 95%.

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Activity of cell-bound and freely-released enzymes, and total enzymatic activity of strains of genus Luteibacter.

Data represent means and standard deviations of the total activity of three replicates. Abbreviations of enzymes: bG: β-glucosidase; Pho: acid phosphatase; Lip: lipase; bM: β-mannosidase; aA: α-arabinosidase; bX: β-xylosidase; bGal: β-galactosidase; CBH: cellobiohydrolase; aG: α-glucosidase; ChTN: n class="Chemical">chitinase; aGal: α-galactosidase; bGlu: β-glucuronidase. A ‘-’ indicates values below detection limit

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Activity of cell-bound and freely-released enzymes, and total enzymatic activity of strains of genus Pseudomonas.

Data represent means and standard deviations of the total activity of three replicates. Abbreviations of enzymes: bG: β-glucosidase; Pho: acid phosphatase; Lip: lipase; bM: β-mannosidase; aA: α-arabinosidase; bX: β-xylosidase; bGal: β-galactosidase; CBH: cellobiohydrolase; aG: α-glucosidase; ChTN: n class="Chemical">chitinase; aGal: α-galactosidase; bGlu: β-glucuronidase. A ‘-’ indicates values below detection limit.

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Activity of cell-bound and freely-released enzymes, and total enzymatic activity of strains of genus Arthrobacter.

Data represent means and standard deviations of the total activity of three replicates. Abbreviations of enzymes: bG: β-glucosidase; Pho: acid phosphatase; Lip: lipase; bM: β-mannosidase; aA: α-arabinosidase; bX: β-xylosidase; bGal: β-galactosidase; CBH: cellobiohydrolase; aG: α-glucosidase; ChTN: n class="Chemical">chitinase; aGal: α-galactosidase; bGlu: β-glucuronidase. A ‘-’ indicates values below detection limit.

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