PACER: a novel 3D plant cell wall model for the analysis of non-catalytic and enzymatic responses
Biotechnology for Biofuels and Bioproducts volume 15, Article number: 30 (2022)
Substrate accessibility remains a key limitation to the efficient enzymatic deconstruction of lignocellulosic biomass. Limited substrate accessibility is often addressed by increasing enzyme loading, which increases process and product costs. Alternatively, considerable efforts are underway world-wide to identify amorphogenesis-inducing proteins and protein domains that increase the accessibility of carbohydrate-active enzymes to targeted lignocellulose components.
We established a three-dimensional assay, PACER (plant cell wall model for the analysis of non-catalytic and enzymatic responses), that enables analysis of enzyme migration through defined lignocellulose composites. A cellulose/azo-xylan composite was made to demonstrate the PACER concept and then used to test the migration and activity of multiple xylanolytic enzymes. In addition to non-catalytic domains of xylanases, the potential of loosenin-like proteins to boost xylanase migration through cellulose/azo-xylan composites was observed.
The PACER assay is inexpensive and parallelizable, suitable for screening proteins for ability to increase enzyme accessibility to lignocellulose substrates. Using the PACER assay, we visualized the impact of xylan-binding modules and loosenin-like proteins on xylanase mobility and access to targeted substrates. Given the flexibility to use different composite materials, the PACER assay presents a versatile platform to study impacts of lignocellulose components on enzyme access to targeted substrates.
The past 20 years has marked several major breakthroughs in our fundamental understanding of lignocellulose bioconversion [1,2,3]. Some of these breakthroughs are already incorporated in enzyme formulations for the efficient conversion of lignocellulosic biomass to fuels, chemicals and new bio-based materials [4,5,6]. Despite the tremendous achievements by excellent research groups world-wide, currently available enzyme formulations fall short of transformation efficiencies achieved in nature. As a result, the economic feasibility of lignocellulose bioconversion to fuels and chemicals remains a challenge [7,8,9]. In particular, limited accessibility of isolated enzymes to targeted lignocellulose components is acknowledged as a major hurdle to enzymatic deconstruction of biomass [10,11,12,13,14].
Enzyme accessibility to targeted substrates embedded in lignocellulosic fiber (e.g., cellulase accessibility to cellulose) has been correlated to the interior surface area of the fiber (i.e., pore size and pore size distribution) as well as exterior surface area of the fiber (i.e., particle size) [14,15,16,17,18]. In addition to structural factors, the chemical composition and distribution of hemicelluloses and lignin in lignocellulosic substrates impacts enzyme accessibility [19,20,21,22]. Measurements of pore size distribution and exterior surface area of lignocellulose substrates include solute exclusion [23, 24], Simons’ staining [10, 25], water retention , fiber size analysis  and thermoporosimetry . Such methods have been especially beneficial when evaluating the impact of lignocellulose pretreatment and cellulose fiber processing on the performance of cellulolytic enzymes. Besides physicochemical analysis of different lignocellulose preparations, fluorescence microscopy, atomic force microscopy, scanning electron microscopy (SEM) among other imaging techniques are powerful options for monitoring changes to fiber structure and accessibility during enzymatic processing [12, 28,29,30,31]. Such imaging approaches, however, are impractical for screening new amorphogenesis-inducing proteins that boost the enzymatic deconstruction of lignocellulose.
The term amorphogenesis was introduced in 1985 to describe the first step to cellulose deconstruction by hydrolytic enzymes . Non-hydrolytic proteins and protein domains that potentially play a role in amorphogenesis increase the initial accessibility of carbohydrate-active enzymes to lignocellulosic substrates . Reported examples include certain carbohydrate-binding modules (CBMs) , swollenins [34,35,36], loosenins [37, 38], microbial expansin-like proteins [38,39,40,41] and lytic polysaccharide monooxygenases . Since amorphogenesis-inducing proteins often adopt a non-hydrolytic mode of action, we contend functional screens that rely solely on the detection of soluble products risk overlooking those proteins that impact enzyme accessibility and migration through lignocellulose materials. Accordingly, our aim was to establish a versatile and low-cost approach to screen for proteins that impact the accessibility of glycoside hydrolases to targeted lignocellulose components.
Herein, we introduce the PACER assay, a novel 3D Plant cell wall model for the Analysis of non-Catalytic and Enzymatic Responses. The PACER assay was inspired by a three-dimensional human cell culture system  and establishes a versatile new screen for proteins that impact the migration of glycoside hydrolases and other enzymes through model lignocellulosic materials. This technique allows the visualization of enzyme penetration and migration along a constructed cellulose composite, and impacts of non-catalytic proteins and protein modules on enzyme migration. Three lines of investigation were pursued for proof of concept of the PACER assay: (1) comparative analysis of three endo-1,4-β-xylanases to assess the impact of protein size and presence of a CBM on enzyme migration through a formulated cellulose/azo-xylan matrix; (2) evaluation of two loosenins for their potential to increase xylanase migration through the formulated matrix, and (3) characterization of Pm25, an endo-1,4-β-xylanase recently discovered from termite gut metagenome . By simultaneously measuring product release and migration of enzymes through defined cellulosic materials, the PACER assay can uncover determinants of enzyme accessibility not detected through measuring release of soluble products alone.
Results and discussion
Development of the PACER assay
Heteroxylans are a diverse group of branched xylans with a backbone of β-(1 → 4)-linked d-xylopyranosyl (Xylp) residues that can be substituted with α-l-arabinofuranose (Araf), 4-O-methyl-α-d-glucuronic acid (MeGlcpA), acetyl groups, p-coumaric acid and ferulic acid, depending on the botanical source . After cellulose, xylans are the most abundant polysaccharide found in lignocellulosic biomass; accordingly, for proof of concept of the PACER assay, we used azo-coupled xylan from birchwood for the impregnation of filter paper (Fig. 1). To initially evaluate azo-xylan retention on the cellulose filter paper, azo-xylan solutions were prepared at between 2.5 and 10% w/v in either milli-Q water or 0.5 M NaOH, and the absorbance of remaining azo-xylan in solution was measured spectrophotometrically at 590 nm. Best retention was observed after solubilizing azo-xylan in 0.5 M NaOH and retention did not increase at azo-xylan concentrations above 5% w/v. Accordingly, the cellulose/azo-xylan composites were prepared using a 5% azo-xylan (w/v) solution prepared in 0.5 M NaOH; acid hydrolysis of corresponding composites confirmed 7.2 ± 0.5% w/w xylan in the generated materials.
Comparison of the accessibility and activity of three different xylanases
The PACER assay was used to compare three endo-β-1,4-xylanases differentiated by glycoside hydrolase family and occurrence of a family 2 carbohydrate-binding module type B (CBM2b). The enzymes were the glycoside hydrolase family 10 (GH10) xylanase from Cellvibrio mixtus (CmXyn10B; Megazyme), the GH11 xylanase from Neocallimastix patriciarum (NpXyn11A; Megazyme), and the GH11 xylanase from Thermobifida fusca (TfXyn11A)  that comprises a C-terminal carbohydrate-binding module belonging to CBM family 2 (CBM2b) (http://www.cazy.org) (Table 1). Briefly, GH10 endo-xylanases bind two consecutive unsubstituted Xylp residues and can generate terminally substituted xylo-oligosaccharides, whereas GH11 xylanases require three consecutive unsubstituted Xylp residues and can generate internally substituted xylo-oligosaccharides [47, 48].
Following treatment with all three endo-β-1,4-xylanases, the cellulose/azo-xylan composite used in the PACER assay showed a discolouration that progressed over time from the right edge to the left edge of the strip (Fig. 2A, B). This was caused by enzymatic release of azo-coupled oligosaccharides and corresponds to enzyme migration from the outer layer (segment D) towards the inner layers (segment C-A) of the composite when rolled around the mandrel. Overall, NpXyn11A migrated fastest and furthest through the cellulose/azo-xylan composite. The greater migration of NpXyn11A compared to CmXyn10B and TfXyn11A was detected after each time point (Fig. 2A, B), even though CmXyn10B and TfXyn11A released similar levels of soluble product to NpXyn11A after 1 h, and even after 3 h in the case of CmXyn10B (Fig. 2C).
This comparative analysis underscores the problem with equating soluble product release and enzyme accessibility to the corresponding substrate. Given that enzyme loadings used herein were based on units of activity, we reasoned that the different positions targeted by GH10 and GH11 would have negligible impact on enzyme migration through the constructed composites. Instead, the presence of a CBM, size of the catalytic domain, and number of Xylp binding sites, likely impacted the diffusion of TfXyn11A, NpXyn11A and CmXyn10B. TfXyn11A (32 kDa) contains a C-terminal CBM2b that binds both cellulose and insoluble xylan . As a type B CBM, CBM2b of TfXyn11A is expected to primarily target the enzyme to the substrate (i.e., display a so-called targeting function) rather than promote fiber disruption [49, 50]. Accordingly, TfXyn11A migration through the cellulose/azo-xylan composite could be limited by dissociation from the substrate. Since neither CmXyn10B (42 kDa) or NpXyn11A (26 kDa) comprise a CBM, the difference in their molecular weight likely drove the varying migration of these enzymes. It is also conceivable that the extended substrate binding surface formed by the higher number of Xylp binding sub-sites expected in NpXyn11A compared to CmXyn10B increased NpXyn11A accessibility to the xylan substrate within the cellulose/azo-xylan composite. Future mutagenesis studies of NpXyn11A, for example, could apply the PACER assay to directly evaluate the impact of an extended substrate binding site on substrate accessibility.
Impact of loosenin-like proteins on NpXyn11A migration
NpXyn11A demonstrated greatest migration through the cellulose/azo-xylan composites and so was selected to investigate the potential of two loosenin-like proteins (PcaLOOL2 and PcaLOOL12 from Phanerochaete carnosa) for ability to boost enzyme accessibility to the xylan substrate . Briefly, loosenins and loosenin-like proteins are microbial expansin-related proteins that comprise the N-terminal D1 domain characteristic of microbial and plant expansins [37, 52]. Similar to other microbial expansin-related proteins, loosenins reportedly weaken filter paper, disrupt cotton fibers, and boost cellulase action on lignocellulosic substrates by a non-lytic mechanism [37, 38].
Using the PACER assay, we observed the potential of PcaLOOL2 and PcaLOOL12 to increase NpXyn11A migration through the constructed cellulose/azo-xylan composite. After 3 h of incubation, NpXyn11A migration through the composites was more advanced in those pretreated with either PcaLOOL2 or PcaLOOL12 compared to composites pretreated with bovine serum albumin (BSA) (Fig. 3A, B). Moreover, the increased migration of NpXyn11A through composites pretreated with PcaLOOL2 coincided with an increase in absorbance measurements of the resulting reaction solutions (Fig. 3C). Notably, the particular boosting effect of PcaLOOL2 on NpXyn11A activity was not observed using azo-xylan in solution (Additional file 1: Fig. S1), and consistent with the predicted loosening effect of loosenin-like proteins, control reactions lacking NpXyn11A showed low release of azo-xylan from composites treated with PcaLOOL2 and PcaLOOL12 alone (Additional file 1: Fig. S2).
PACER for the characterization of a novel GH10 endo-β-1,4-xylanase and its mutants
Having demonstrated the potential of the PACER assay to uncover performance differences between well characterized xylanases, we then evaluated the potential of the assay to characterize a recently discovered multimodular xylanase. Briefly, the earlier metagenomic analysis of the fungus-growing termite, Pseudacanthotermes militaris, revealed a putative xylan utilization locus linked to the genus Bacteroides . One of its open reading frames encodes a multimodular GH10, designated P. militaris 25 (Pm25). This enzyme is characterized by a discontinuous organization that includes the insertion of two tandem CBM4 domains (CBM4-1 and CBM4-2) within the catalytic GH10 xylanase domain (Table 1) .
To assess the impact of this unusual multidomain organization on enzyme migration, Pm25 and three constructs with modular deletions or point mutations were characterized using the PACER assay. Variant M1 (Pm25 E546A) harbors a point mutation in domain GH10b, reducing its activity on glucuronoxylan and arabinoxylan by two to three orders of magnitude . Variant M5 (Pm25 Y213A + Y378A) carries two point mutations inactivating CBM4-1 and CBM4-2. Lastly, both CBM4 domains are deleted in M6 (Pm25∆CBMs) . Given the particularly low activity of M1 on azo-xylan in solution (Table 1), the wild-type Pm25 and all variants were compared using the PACER assay on a molar basis.
The low residual activity of the M1 variant was insufficient to promote detectable M1 migration through the cellulose/azo-xylan composite (Fig. 4A, B). More interesting, despite achieving similar levels of azo-xylan hydrolysis in solution (Additional file 1: Fig. S3), differences in wild-type Pm25, M5 and M6 performance after 3 h were clearly observed when using the PACER assay (Fig. 4A, B). The PACER assay also showed a clear correlation between activity and mobility, suggesting little to no passive diffusion of the enzyme through the system. The deletion of CBM4-1 and CBM4-2 leading to M6 significantly increased xylanase migration through the cellulose/azo-xylan composite, indicating that molecular weight outweighs the proximity effect gained by CBM4-1 and CBM4-2, at least at high substrate concentration . Given the high apparent substrate concentration, the substantially lower migration of M5 compared to wild-type Pm25 was more surprising. Wu et al.  previously reported the lower activity of M5 compared to wild-type Pm25 on insoluble wheat bran; however, herein, differences in M5 and wild-type Pm25 migration were observed despite displaying similar levels of activity on azo-xylan (Fig. 4C). It is conceivable that active forms of CBM4-1 and/or CBM4-2 of Pm25 could impart both proximity and disruption effects to the wild-type Pm25 by extending the number of Xylp binding sub-sites of the catalytic domain.
The three-dimensional PACER assay was established to accelerate the discovery of non-catalytic proteins and protein domains that increase enzyme access to lignocellulosic substrates. Using a cellulose/azo-xylan composite to demonstrate the PACER concept, we could readily visualize the impact of xylan-binding modules and loosenin-like proteins on xylanase mobility and accessibility to the targeted substrate. The low cost, small scale, and option to create different composite materials, contribute to the advantages of the PACER assay. By using labeled proteins, composites could in future be constructed using defined and native lignocellulose components, and then visualized by tracking the labeled protein.
Substrates and chemicals
VWR® quantitative filter paper grade 454 (Cat.# 516-0857) was supplied by VWR (Radnor, PA, USA). Azo-xylan (birchwood powder; Cat.# S-AXBP) was obtained from Megazyme (Bray, Ireland). All other chemicals were reagent grade.
Enzymes and non-catalytic proteins
CmXyn10B (recombinant endo-β-1,4-xylanase from Cellvibrio mixtus; Cat.# E-XYNBCM) and NpXyn11A (recombinant endo-β-1,4-xylanase from Neocallimastix patriciarum; Cat.# E-XYLNP) were obtained from Megazyme. TfXyn11A (recombinant endo-β-1,4-xylanase from Thermobifida fusca) was kindly provided by T.V. Vuong . All xylanases were purchased or recombinantly prepared as mono-component enzymes; protein purity was determined by SDS-PAGE (Additional file 1: Fig. S4). Bovine serum albumin (BSA) was obtained from Sigma-Aldrich (St. Louis, MO, USA; CAS# 9048-46-8).
PcaLOOL2 (loosenin-like protein 2 from Phanerochaete carnosa, GenBank code EKM55357.1) and PcaLOOL12 (loosenin-like protein 12 from Phanerochaete carnosa, GenBank code EKM51974.1) were recombinantly expressed in Pichia pastoris SMD1168H. Briefly, codon optimized genes encoding PcaLOOL2 or PcaLOOL12 were obtained as subcloned in pPICZαA plasmids with a C-terminal 6 × His tag (GenScript, Piscataway, NJ, USA). Transformants were grown in shake flasks in buffered glycerol-complex medium (BMGY; 100 mM potassium phosphate buffer (pH 6.0), 2% (w/v) peptone, 1% (w/v) yeast extract, 1.34% (w/v) yeast nitrogen base, 4 × 10–5% (w/v) biotin, 1% (v/v) glycerol) at 30 °C and 100 rpm until an OD600 of ~ 6 and then induced in buffered methanol-complex medium (BMMY; BMGY containing 0.5% (v/v) methanol instead of glycerol). Secreted recombinant proteins were purified from culture supernatants by FPLC using a GE Healthcare HisTrap™ FF Crude prepacked column (Thermo Fisher Scientific; Cat.# 11723219).
Pm25 (Xyn10C, endo-β-1,4-xylanase from the termite Pseudacanthotermes militaris gut metagenome, GenBank code CCO21036.1) and variants M6 (Pm25∆CBMs), M5 (Pm25 Y213A Y378A) and M1 (Pm25 E546A) were recombinantly expressed in E. coli Rosetta™ (DE3) pLysS as previously described .
Enzyme activity determination
The activity of endo-β-1,4-xylanases on azo-xylan was determined according to the protocol provided by Megazyme with minor alterations. In brief, a 1% solution of azo-xylan was prepared in milli-Q H2O, 0.25 mL was transferred into a 15-mL Falcon™ conical centrifuge tube and pre-equilibrated in a ThermoMixer C set at 40 °C. Enzymes were diluted in 100 mM sodium acetate buffer (pH 5.0), 0.25 mL buffered enzyme preparation were added to the azo-xylan solution and thoroughly mixed. Tubes were incubated at 40 °C for 10 min, after which reactions were terminated by addition of 1.75 mL 96% (v/v) ethanol with vigorous stirring. Tubes were incubated at room temperature for 10 min and again thoroughly mixed. In the case of reaction blanks, ethanol was added prior to enzyme addition. Supernatants were recovered by centrifugation (3000 rpm for 10 min) and absorbance was analyzed spectrophotometrically at 590 nm. Activities were calculated with the Megazyme Mega-Calc™ using Aspergillus niger endo-β-xylanase as a reference.
Preparation of cellulose/azo-xylan composites and confirmation of xylan content
Azo-xylan was dissolved in slightly heated 0.5 M NaOH to produce a 5% (w/v) solution and then stirred at room temperature for 1 h before transferring 6 mL of the solution to the bottom of a glass petri dish (Ø 190 mm). A pre-dried filter paper (VWR® quantitative filter paper grade 454; Ø 185 mm) was then submerged in the solution and covered with an additional 5 mL of the azo-xylan preparation. An even pressure was then applied by gently pressing the submerged filter paper with a second petri dish that had a slightly smaller diameter. After applying pressure to both sides of the filter paper, the paper was left to incubate in the azo-xylan solution for two more minutes before being placed between paper towels to remove excessive liquid. The resulting cellulose/azo-xylan composite was then dried for 10 min at 60 °C, washed in ~ 125 mL ice-cold 0.5 M acetic acid for 2 min, rinsed and washed in milli-Q H2O for 10 min, and then dried over night at 60 °C. The cellulose/azo-xylan composite was then cut into 4.9–5.2 mm × 80 mm strips using a guillotine paper trimmer. The weight percent of azo-xylan retained in the filter paper was verified by acid hydrolysis of cellulose/azo-xylan composites (n = 2). Briefly, for the acid hydrolysis, 10–11 mg of composite (two composites were analyzed in duplicate, n = 4) was prehydrolyzed with 72% H2SO4 (0.45 mL) at 30 °C for 1 h and then hydrolyzed with 1 M H2SO4 (10.9 mL) at 100 °C for 3 h. Samples were diluted 50 times and analyzed by high performance anion exchange chromatography (HPAEC) on a Dionex Ultimate 6000 system (Thermo Scientific, Sunnyvale, CA, USA) equipped with a CarboPac PA-1 column (2 mm × 250 mm ID) in combination with a CarboPac PA-1 guard column (2 mm × 50 mm ID) and PAD detector. Elution of monosaccharides (0.25 mL min−1) was performed with a multi-step-gradient using the following eluents: A: 0.1 M NaOH, B: 1 M NaOAc in 0.1 M NaOH, C: 0.2 M NaOH, and D: milli-Q water. Gradient was as follows: 0–20 min 16% A and 84% D; 20–25 min 45%A, 5%B, and 50%D; 15 min with 60%A and 40% B; 25–37 min 100% C (flow rate up to 0.35 mL min−1 over the first 2 min), and 37–49 min 16%A, 84%D (flow rate decreased to 0.25 mL min−1 over the first 2 min). The system was controlled using Chromeleon 7.2.9 software (Thermo Scientific, Sunnyvale, CA, USA).
Cellulose/azo-xylan composites were soaked in 50 mM sodium acetate buffer (pH 5.0) for 3 min and then each strip was rolled tightly around a metal mandrel (Ø 6.0 mm, height 15.1 mm) before securing the outer end of the strip with a custom-made plastic clip . The resulting mandrels were then placed in a 24-well round bottom microplate and fixed in an upright position using a pipette tip (Agilent Technologies, Santa Clara, CA, USA; Cat.# 202061-300) (Fig. 1).
To compare the migration of three different endo-β-1,4-xylanases, mandrels were incubated in a total reaction volume of 3 mL containing 0.01 mg/ mL CmXyn10B, 0.005 mg/ mL NpXyn11A or 0.009 mg/ mL TfXyn11A in 50 mM sodium acetate buffer (pH 5.0). For all three enzymes, this corresponded to 71 mU/ mL. As a reference, mandrels were incubated in buffer only. Incubations were performed for 1—6 h on a ThermoMixer C set at 40 °C and 300 rpm.
The impact of loosenin-like proteins on the migration of endo-β-1,4-xylanases through cellulose/azo-xylan composites was investigated by submerging each strip (4.9–5.2 mm × 80 mm) in 0.5 mL of 50 mM sodium acetate buffer (pH 5.0) alone or containing 0.1 mg/ mL PcaLOOL2, PcaLOOL12, or BSA. After 24 h, each composite strip was rolled on a mandrel and incubated in 3 mL of 50 mM sodium acetate buffer (pH 5.0) alone or containing 0.005 mg/ mL (71 mU/ mL) NpXyn11A. Incubations were performed for 0.5–6 h on a ThermoMixer C set at 40 °C and 300 rpm.
The PACER assay was also used to further characterize a novel GH10 endo-β-1,4-xylanase and its mutants. Here, mandrels were incubated in 3 mL of 50 mM sodium acetate buffer (pH 5.0) containing 0.03 mg/ mL wild-type Pm25, 0.03 mg/ mL of the M5 mutant (Pm25 Y213A Y378A), 0.017 mg/ mL of the M6 mutant (Pm25∆CBMs) or 0.03 mg/ mL of the M1 mutant (Pm25 E546A). As a reference, mandrels were incubated in buffer only. Incubations were performed for 0.5–20 h on a ThermoMixer C set at 40 °C and 300 rpm.
After each incubation, the mandrel was transferred to ice-cold milli-Q H2O for 3 min. Composites were then unrolled, washed three times in their corresponding reaction solution to release soluble products to the reaction supernatant, placed on a petri dish and dried over night at 60 °C. Absorbance of the reaction solution was analyzed spectrophotometrically at 590 nm.
Dried composites were scanned at 600 × 600 dpi using Canon image RUNNER Advance C5250i system. The image processing was done with Fiji software [54, 55]. The scanned RGB images were converted to Hue Saturation Brightness (HSB) color space. The strips were segmented from the background pixels in the saturation channel using “Threshold tool” by choosing pixels with minimum intensity value of 80 and maximum value of 255. The saturation channel was chosen for the analysis because it contained most of the tone loss due to the enzymatic reaction in comparison to the other channels. From Fiji function “Analyze particles” the minimum particle size was set as 1000 pixels to remove wrongly selected pixels from the background. Fiji function “save XY coordinates” was used to extract the x and y coordinates of each pixel, as well as their intensity value in each strip. The data were stored as CSV files and imported to R studio  for further processing. X coordinates of the pixels were converted into percentages relative to full length of the strip and the split into four segments corresponding to turns of cellulose/azo-xylan composites around the mandrel. Mean intensity values of each segment with the standard error of the mean from at least four replicated strips per treatment were plotted. Processing, analysis and plotting of the data were done using Tidyverse 1.2.1, ggplot2 3.2.1, dplyr 0.8.3 R packages [56,57,58,59]. Code for extracting pixel information using Fiji and processing the data in R is deposited in GitHub and available through the link https://github.com/mipavici/PACERassay.
Assay for in-solution hydrolysis of azo-xylan
Xylanase reactions using azo-xylan were optimized to ensure absorbance values were within the linear range of the assay. Final reactions contained 0.06% azo-xylan in 50 mM sodium acetate buffer (pH 5.0). For activity assays using NpXyn11A, 0.001 mg/ mL NpXyn11A were used and incubations were performed at 40 °C and 300 rpm for 10 min. NpXyn11A activity on azo-xylan were also measured after pre-incubation of the azo-xylan solution with 0.003 mg/ mL PcaLOOL2, PcaLOOL12 or BSA in a ThermoMixer C set at 25 °C and 300 rpm for 24 h. For activity assays using Pm25 and corresponding variants, 0.03 mg/ mL Pm25, 0.03 mg/ mL Pm25 Y213A Y378A (aka M5), 0.017 mg/ mL Pm25∆CBMs (aka M6) or 0.03 mg/ mL Pm25 E546A (aka M1) were used and reactions were incubated in a ThermoMixer C set at 40 °C and 300 rpm for 3, 6 and 20 h.
In all cases, reactions were terminated using 1 mL 96% (v/v) ethanol with vigorous stirring. In the case of reaction blanks, ethanol was added prior to enzyme addition. Supernatants were recovered by centrifugation (15,000 rpm for 10 min) and absorbance was analyzed spectrophotometrically at 590 nm.
Availability of data and materials
All data generated or analyzed during this study are reported in this manuscript and its Additional file 1.
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We thank Kuisma Littunen and Kim Kataja who assisted with substrate preparation and Nelly Monties who assisted with enzyme production. We also thank Professor A. McGuigan (University of Toronto) for helpful discussions.
We thank the following granting agencies for their financial support: the European Research Council (ERC) (Consolidator Grant no. BHIVE – 648925) (MM, EJ, VL and ERM); Jenny and Antti Wihuri Foundation (Centre for Young Synbio Scientists) (TK); Academy of Finland Postdoctoral Researcher Grant No. 331853 (TP); The French national research agency (anr) Grant No. ANR-18-CES43-DECO (TE and CD).
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Figure S1. Impact of loosenin-like proteins on NpXyn11A hydrolysis of azo-xylan in solution. Figure S2. Impact of loosenin-like proteins on cellulose/azo-xylan composites. Figure S3. In-solution hydrolysis of azo-xylan by Pm25 and its mutants. Figure S4. SDS-PAGE analysis of CmXyn10B (lane 2), NpXyn11A (lane 3) and TfXyn11A (lane 4). Figure S5. Replicate cellulose/azo-xylan composites after treatment for 1-h with (A) NpXyn11A or (B) TfXyn11A.
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Monschein, M., Jurak, E., Paasela, T. et al. PACER: a novel 3D plant cell wall model for the analysis of non-catalytic and enzymatic responses. Biotechnol Biofuels 15, 30 (2022). https://doi.org/10.1186/s13068-022-02128-8
- Assay development
- Enzyme accessibility