A recombinant xylose reductase enzyme with biotechnological potential for xylitol production

Heterologous Expression of a Neurospora crassa Catalase Reprograms the Cellulase System and Enhances β-Glucosidase Production in Trichoderma reesei

Efficient saccharification of lignocellulose, the most abundant renewable carbon reservoir resource, is of great industrial importance. Trichoderma reesei is a premier cellulase producer, but its fermentation efficiency is often constrained by dual challenges: dissolved oxygen limitation and intrinsic oxidative stress. To address this, we engineered T. reesei to heterologously express a robust catalase gene (cat-3) from Neurospora crassa. The recombinant strain Tr-cNcat3 exhibited a 7.4-fold increase in extracellular catalase activity. Tr-cNcat3 showed an increase in total extracellular protein, resulting in markedly enhanced filter paper activity (FPA) and β-glucosidase activity compared to the control. Strikingly, this intervention specifically triggered a significantly higher expression of β-glucosidase, a known bottleneck in T. reesei’s cellulase system, particularly on bagasse and straw as the carbon source. Moreover, the ability of the supernatant to degrade cellulose substrates was improved. Our results reveal that overexpression of cat-3 in T. reesei could modify the cellulase cocktail by triggering a higher level of β-glucosidase. This study provides a novel and effective genetic engineering strategy to unlock the full industrial potential of T. reesei for cost-effective lignocellulosic biorefining.

Enhanced Trehalose Production Through Integrated Chassis and Expression Engineering in Bacillus subtilis

Trehalose is a functional disaccharide widely used in the food, pharmaceutical, and cosmetic industries. It is industrially produced via a dual-enzyme process involving maltoligosaccharide trehalose synthase (MTSase) and maltoligosaccharide trehalose hydrolase (MTHase), with Escherichia coli (E. coli) serving as the expression host. Bacillus subtilis (B. subtilis) is an ideal host for industrial trehalose production due to its generally recognized as safe (GRAS) status and low phage susceptibility. However, engineered B. subtilis strains often exhibit slow growth, low heterologous protein expression, and high fermentation costs, thereby limiting their industrial application. To address these challenges, this study employed a synergistic strategy that combined chassis modification, expression element optimization, and knockout of substrate-competition pathways. First, a tryptophan-independent strain was constructed by reverting the trpC2 mutation to shorten the growth cycle. Next, knockout of flgD, yueB, and integration of E. coli-derived glutamate dehydrogenase (gdhA) significantly enhanced biomass accumulation. Expression of MTSase and MTHase was markedly improved through tandem strong promoters (PHpaII-P36) and ribosome-binding site (RBS) optimization (RBS1), achieving a 10.87-fold and 4.22-fold increase in enzyme activity, respectively. Finally, disruption of the amyE gene reduced non-specific substrate degradation. Using maltodextrin as substrate, the final trehalose conversion rate reached 76%. This study constructed B. subtilis chassis cells that highly express MTHase and MTSase respectively, laying a foundation for subsequent industrial trehalose production.

A highly efficient thermostable xylanase from Thermomyces dupontii J22: purification, properties and its application in xylan film modification

Xylitol Biomanufacturing: Production Technologies, Industrial Applications and Future Opportunities

Xylitol is a five-carbon sugar alcohol widely used in the food, pharmaceutical, oral healthcare, and personal care industries because of its low caloric value, low glycaemic index, and non-cariogenic properties. Industrial production is mainly based on catalytic hydrogenation of xylose, which provides high conversion efficiency but requires intensive energy input, costly catalysts, and complex purification processes. Microbial fermentation has emerged as a sustainable alternative for producing xylitol from renewable lignocellulosic biomass. This review summarizes recent advances in xylitol production, with a particular focus on microbial biomanufacturing. Key developments in lignocellulosic biomass utilization, metabolic engineering, cofactor balancing, oxygen regulation, and fermentation optimization are discussed. Chemical and biological production routes are critically compared in terms of efficiency, sustainability, and industrial applicability. Recent progress in downstream purification and biorefinery integration is also highlighted. Despite substantial advances, challenges including inhibitor toxicity, limited microbial robustness, low fermentation productivity, and high purification costs continue to hinder large-scale commercialization. Future research should focus on feedstock valorization, systems metabolic engineering, process intensification, and sustainable separation technologies to improve the economic and environmental sustainability of bio-based xylitol production.

Scalable catalyst production process for oleate hydratase whole-cell biocatalysis.

The sustainable production of hydroxy fatty acids, such as 10-hydroxystearic acid (10-HSA), by biocatalysis is a promising alternative to petrochemical and castor oil-derived products. However, industrial implementation still requires an efficient and scalable process for biocatalyst production by fermentation, which precedes the biotransformation to 10-HSA. In general, industrial biocatalysis is commonly performed using whole cells, which are cheaper than purified enzymes. Still, the fermentation process itself is a major cost contributor requiring a high-yielding and scalable process. Here, we established and scaled a lactose-induced fed-batch process to produce an Escherichia coli BL21 (DE3) based whole-cell biocatalyst containing an oleate hydratase from Stenotrophomonas nitritireducens. The two-phased process employs an initial growth phase on glucose, followed by an induced feed phase using glycerol and lactose. When comparing two different growth rates during enzyme expression, a higher growth rate was found beneficial, resulting in a higher biomass concentration of 69.2 ± 0.5 g L-1 and a yield increase of 80 % while maintaining biocatalyst activity at >85 % conversion. This highlights the importance of process design variables, such as growth rate settings, for a high-yielding and economic process. Feasibility of the process was demonstrated by scaling into a 150 L bioreactor, achieving a biomass concentration of 60.6 ± 0.4 g L-1 with a yield of 0.44 gC,Biomass gC -1 and 91.5 ± 1.4 % conversion. Supplemented with an initial test of suitable unit operations for technical biomass separation, this work provides a fermentation route for a whole-cell oleate hydratase biocatalyst, paving the way for further scaling toward industrial 10-HSA production.

Periplasmic Engineering Enhances Terminal Hydroxylation for Efficient Caffeic Acid Biosynthesis in Escherichia coli.

Caffeic acid (CA) is a valuable phenylpropanoid with applications in food, pharmaceutical, and chemical industries. Microbial production of CA is often limited by the terminal hydroxylation catalyzed by 4-hydroxyphenylacetate 3-monooxygenase (HpaBC). Here, we constructed a de novo CA biosynthetic pathway in Escherichia coli and enhanced production through systematic metabolic and spatial engineering. Optimization of l-tyrosine supply and HpaBC expression increased CA production to 61.0 mg/L. However, further enhancement of glucose uptake and precursor supply was insufficient, indicating that hydroxylation remained a major limitation. To address this, HpaBC was relocated to the periplasm via the Tat pathway, increasing CA production 4.9-fold to 299.1 mg/L with reduced byproduct formation. Further lpp+14 mediated periplasmic remodeling and fermentation optimization increased shake-flask production to 463.7 mg/L. Finally, fed-batch fermentation achieved 5.1 g/L CA in a 3 L bioreactor. This study highlights periplasmic engineering as an effective strategy for improving oxidation-dependent phenylpropanoid biosynthesis.