Synthetic and Systems Biotechnology

Bacillus subtilis is a core microbial chassis in biomanufacturing, and establishing efficient gene editing technologies is key to engineering this strain. In conventional CRISPR gene editing technologies, the large size of DNA nucleases leads to difficulties in plasmid construction, low transformation efficiency, and cumbersome multi-round editing operations; therefore, developing miniature gene editing tools can effectively address these issues. Although our group previously established a miniature gene editing tool based on IscB in B. subtilis SCK6, IscB relies on the 5'-CAGGAA-3' TAM recognition sequence, and 83.36% of the genes in the SCK6 genome harbor no or only one TAM sequence, indicating a bottleneck of restricted editing for IscB in this strain. The novel miniature DNA nuclease TasR does not require a TAM sequence and can thus compensate for the limitation of IscB; however, the applicability of TasR in B. subtilis remains unknown. Therefore, this study first constructed a single plasmid, pBsuTasR, capable of expressing TasR and its guide RNA (tigRNA), which enabled gene deletion of regular-sized fragments in SCK6 with editing efficiencies of 21.7%- 78.3%. Subsequently, the capacity of TasR to delete a long DNA fragment (169.9 kb) was evaluated, and it was found that under the guidance of a single tigRNA, the deletion efficiency was 21.73%, whereas after optimizing to two tigRNAs, the efficiency increased to 39.13%. Furthermore, the gene integration capability of pBsuTasR was further tested, and TasR was able to integrate the aprN gene into the amyE locus at an efficiency of 13.3% under the guidance of a single tigRNA, and after increasing to two tigRNAs, the integration efficiency increased to 91.3%. In terms of iterative genome editing, this study developed the pBsu-SRP (Scissors-Rock-Paper) iterative editing system, which automatically cures the editing plasmid from the previous round while performing a new round of gene editing, with sequential gene deletion efficiencies of 4.34%-26.08%, and using this system, the editing cycle can be shortened from 4N days by the conventional method to 3N+1 days. Subsequently, the pBsu-SRP system was successfully used to achieve the integration of two and three copies of the mCherry fluorescent reporter gene in SCK6, and it was found that the fluorescence intensity increased with the copy number. Finally, this study also explored the escape of SCK6 from TasR cleavage and found that mutations in the tigRNA sequence are the cause of the escape. In summary, this study constructed a novel miniature genome editing system in B. subtilis using the TAM-independent nuclease TasR as the core component. This system can not only provide an efficient technical tool for genetic manipulation of industrial microorganisms, but also offer new instrumental support for the iterative engineering and functional optimization of chassis cells in biomanufacturing.

With the rapid development of modern biotechnology, DNA vectors have become fundamental tools for inserting, transferring, and expressing specific gene sequences in various fields such as gene cloning, gene expression, gene editing, and gene therapy. However, when dealing with complex structured DNA sequences, traditional vector construction methods face challenges with low connection efficiency. This study proposes a new method for constructing recombinant vectors by employing a strategy of high-temperature treatment followed immediately by placement on ice, effectively reducing the complexity of DNA structures and enhancing the efficiency of PCR product-vector connection, thereby improving the construction efficiency of recombinant vectors. This paper describes the technical details of the method, experimental validation, and applications in gene cloning, gene recombination editing, and the preparation of gene therapy drugs, providing a new efficient tool for molecular biology experiments.

Archaea are promising chassis organisms in biotechnology, and the accurate annotation of their chromosomal replication origins (oriCs) is the key to unlocking their full potential. However, the existing Ori-Finder 2 web server suffers from low accuracy, slow speed, and limited scalability. In this study, we present Ori-Finder-Arch, an updated web server for high-performance oriC prediction in archaea. This pipeline integrates HMMER-based replication initiation protein (RIP) annotation, refined consensus motif recognition, and GC profile-based DNA unwinding element (DUE) detection. On a benchmark set of experimentally validated oriCs, Ori-Finder-Arch achieved a recall of 95.6% and a precision of 86.0%, substantially outperforming Ori-Finder 2 (62.2% and 63.6%, respectively), while running 4.75 times faster and supporting diverse assembly levels. When applied to the available archaeal assemblies, it successfully annotated 17,472 oriCs. Meanwhile, the web server provides interactive visualizations at different levels. In conclusion, Ori-Finder-Arch offers an efficient, accurate, and user-friendly platform for advanced studies of archaeal DNA replication initiation and synthetic biology applications, and is freely available at https://tubic.org/Ori-Finder-Arch/ and https://tubic.tju.edu.cn/Ori-Finder-Arch/.

The benzoxazolinate moiety is a key functional group found in a few natural products (NPs), exhibiting diverse bioactivities, including antitumor, antibacterial, and cytotoxic activities. Despite their clinical importance, only a few bacterial strains and NPs have been reported harboring this rare bis-heterocyclic moiety, underscoring a largely unexplored chemical space. Here, we performed large-scale genome mining and identified 277 putative biosynthetic gene clusters (BGCs) across diverse bacterial hosts, including previously unreported bacterial genera and strains. The BGCs were grouped into three compound classes: benzoxazolinate, benzobactin, and ashimides based on sequence similarity network clustering. Bioactivity predictions of the identified BGCs revealed the predominance of antibacterial and cytotoxic potential, highlighting promising candidates for future experimental validation and functional studies. This study also presents a neural network-based bioprospecting model that efficiently detects rare BGCs encoding benzoxazolinate-containing molecules from genomic sequences. Overall, our findings expand the known repertoire of bacterial hosts with the potential to produce benzoxazolinate-containing NPs and provide a comprehensive framework for the discovery and identification of candidate BGCs.

Natural product synthesis by non-ribosomal peptide synthetases (NRPS) is greatly defined by the substrate selectivity of the adenylation (A) domains. Previous assays for specificity determination were mainly performed in vitro and were requiring protein purification. In this work, we developed - based on NRPS engineering - a novel in vivo assay suitable for high-throughput application named ASCR (A domain screening). Using the recently described XUT fusion sites, A domains and their upstream condensation domains were assembled as di-domains to characterized NRPS model system, which allowed detection of defined tripeptide products via mass spectrometry directly after cell culture extraction. We evaluated the assay by screening in total 54 A domains from five known and seven uncharacterized NRPS, covering a broad range organism taxonomy and GC content of the investigated NRPS-encoding genes. Additionally, we applied the assay to elucidate and confirm the structures of novel cyclic pentapeptides derived from three novel NRPS from Photorhabdus temperata K122.

Halophilic chassis has emerged as a promising biomanufacturing platform for industrial polyhydroxyalkanoate (PHA) production. However, challenges still remain in improving the production capacity, scalability and robustness, thereby lowering cost to meet market demands. Here, a high-performing halophilic strain Halomonas LY03 was isolated with over 38% glucose- to-PHA conversion rate and broad non-grain substrate utilization capability. Multidimensional tools, including algorithm-guided high-expression neutral integration site (HENIS) screening toolkit designated SiteSeek, stop codon (TAA)-dependent enhancement of gene expression and recombinase-mediated large-fragment (> 9 kb) genomic integration, were then developed to enable precise, efficient and interference-free genomic integrative expression. Using these tools, various chromosomally engineered strains were rapidly constructed to achieve high-level production of poly-3-hydroxybutyrate (PHB, 151 g L-{superscript 1}) and poly(3-hydroxybutyrate-co-4-hydroxybutyrate) (P34HB, 139 g L-{superscript 1}) under high cell-density fermentation (up to 186 g L-1 cell dry weight) in a 5-L bioreactor. Scalability was demonstrated at 2-m3 and 20-m3 industry-scale fermentations, yielding up to 134 g L-{superscript 1} PHB and 127 g L-{superscript 1} P34HB (6.1 mol% 4HB). Building on the proven robustness, a two-stage continuous fermentation (TCF) process was developed using a twin-bioreactor system at 5-L and 20-m3 scales, where stable and sustained PHA production lasted over 260 h and 160 h, respectively. Techno-economic analysis revealed a substantial cost-reduction space of 48% compared with conventional fed-batch process. This study demonstrates a successful paradigm for engineering a newly isolated strain toward robust, high-titer and cost-competitive PHA production across lab-to-industry scales.

Nicotine accumulates in the gut and drives non-alcoholic steatohepatitis (NASH) via the gut-liver axis, yet no effective clinical intervention is currently available. To address this challenge, the probiotic Escherichia coli Nissle 1917 (EcN) was engineered for in situ nicotine clearance in the gut. Mutational screening of nicotine oxidoreductase 2 (PpNicA2) identified a highly active variant, PpNicA2A107R. Its incorporation into EcN together with an electron transfer protein (CycN) and a newly identified transporter (T3/T7) yielded 80% nicotine-degrading activity. Chromosomal integration of this module generated a stable strain, EcN-N12, which in NASH mouse models depleted intestinal nicotine, rescued hepatic lipid metabolism, alleviated tissue damage, and intercepted the nicotine-mediated gut-liver axis pathological progression. This work thus offers an effective and clinically translatable approach for nicotine-associated diseases.

Circular single-stranded DNA (cssDNA) is a versatile biomolecule with applications spanning genome editing, DNA nanotechnology, synthetic biology, molecular diagnostics, and aptamer development. Compared with linear single-stranded DNA, cssDNA offers enhanced structural stability, resistance to in-cellulo degradation by exonucleases and enables the generation of long, sequence-defined DNA molecules that are difficult to obtain through conventional chemical synthesis methods. Despite its growing utility, widespread adoption of cssDNA has been limited by the lack of accessible, scalable, and cost-effective production methods, with many existing workflows relying on specialised reagents, extensive optimisation, or commercially synthesised DNA. Here, we present a streamlined, end-to-end protocol for the laboratory-scale production of high-purity cssDNA using an M13 phagemid-based system and standard molecular biology laboratory infrastructure. The workflow encompasses bacterial culture, phage amplification, nuclease treatment, phage precipitation, anion-exchange purification, and quality control, with practical optimisations to improve yield, reproducibility, and scalability. Using this approach, yields range from 120-195 {micro}g of purified cssDNA from 300 mL of culture supernatant. The protocol provides detailed guidance on critical process parameters, troubleshooting, and quality assessment, enabling reliable production of cssDNA suitable for a wide range of downstream molecular biology and genome engineering applications.

Poly(ethylene terephthalate) (PET) is one of the most widely produced plastics, and enzymatic depolymerization offers a promising route to closed-loop recycling under mild conditions. However, most known bacterial PET hydrolases belong to a conserved canonical-fold cutinase family, leaving much of alpha/beta-hydrolase diversity unexplored. Here, we mapped bacterial cutinase sequence space by combining bioinformatics-guided sequence selection with high-throughput secretion screening in Bacillus subtilis. A library of 1,120 genes encoding 954 unique bacterial cutinases, spanning canonical- and minimal-fold families, was screened for activity on Impranil DLN and semicrystalline PET. We identified 156 secreted cutinases with polyester activity, broadly distributed across sequence space, but only ten showed detectable PET hydrolysis, all from the canonical-fold family. These PET hydrolases were active at 40-50{degrees}C, preferred alkaline pH, and showed moderate thermostability. Our results demonstrate that PET activity is rare among bacterial cutinases and provide a scalable workflow for discovering diverse enzyme starting points.

Building high-performance microbial cell factories requires dynamic coordination of resource allocation among cellular growth, target-product biosynthesis, and endogenous host metabolism. However, existing polyploid engineering strategies rely primarily on static manipulation of chromosome copy number. Although increasing gene dosage can enhance biosynthetic capacity, static designs cannot readily accommodate the changing metabolic demands encountered during fermentation. Here, we developed a metabolite-responsive dynamic polyploid engineering strategy that couples chromosome ploidy to the cellular metabolic state. We first constructed a high-performance L-threonine biosensor and used it to sense intracellular L-threonine levels and regulate ftsZ expression, a key cell-division gene, thereby establishing a dynamic polyploid system that requires neither exogenous inducers nor antibiotics. This system enabled engineered cells to progressively transition from polyploid to haploid during fermentation, accompanied by stage-specific remodeling of cellular physiology and metabolism. Physiological characterization revealed a marked increase in cell size and alterations in cell-envelope properties during the polyploid phase, followed by a gradual decrease in chromosome copy number as fermentation progressed. Transcriptomic and metabolomic analyses further demonstrated that dynamic ploidy transitions induced global metabolic network rewiring, remodeling the tricarboxylic acid cycle and amino acid metabolism while redirecting carbon flux toward the biosynthesis of aspartate-family amino acids. Ultimately, dynamic polyploid engineering substantially enhanced L-threonine production, enabling the engineered strain to achieve an L-threonine titer of 183.1 g/L and a yield of 0.67 g/g glucose in 5-L fed-batch fermentation without antibiotics or exogenous inducers. These findings show that dynamic regulation of chromosome ploidy can couple gene-dosage control with remodeling of cellular physiology and metabolic networks, providing a new engineering strategy to overcome the limitations of static polyploid designs and build high-performance microbial cell factories.

We present a robust and versatile in vitro transcription (IVT) assay based on an optimized Broccoli RNA aptamer sequence. When paired with the fluorophore DFHBI-1T, this system enables real-time monitoring of multi-round transcription over several hours. To facilitate streamlined promoter analysis, we developed the pIVT3 plasmid backbone. The system was validated using both the single-subunit T7 RNA polymerase and the multi-subunit Escherichia coli RNA polymerase; notably, the activity of the E. coli enzyme remained strictly dependent on the presence of a {sigma} factor and a cognate promoter. To optimize the signal-to-noise ratio, we incorporated two rrnBT1 terminators upstream of the promoter of interest. This modification effectively eliminated background transcription for weak promoters (PlivJ) and prevented interference from read-through transcription in strong synthetic promoters (Ptrc*). Furthermore, we demonstrated the assays utility for drug discovery by characterizing the time- and dose-dependent inhibitory kinetics of rifampicin. Collectively, these results establish the Broccoli-based IVT system as a highly adaptable platform for quantifying promoter strength and screening small-molecule inhibitors of bacterial transcription. Graphical Abstract O_FIG O_LINKSMALLFIG WIDTH=200 HEIGHT=141 SRC="FIGDIR/small/744185v1_ufig1.gif" ALT="Figure 1"> View larger version (42K): org.highwire.dtl.DTLVardef@1e0c991org.highwire.dtl.DTLVardef@d154aeorg.highwire.dtl.DTLVardef@10e95fcorg.highwire.dtl.DTLVardef@98ea80_HPS_FORMAT_FIGEXP M_FIG C_FIG

Methane is a potent greenhouse gas, nearly half of which is consumed anaerobically by anaerobic methanotrophic archaea (ANME) through methyl-coenzyme M reductase (Mcr). However, ANME cannot be grown as pure cultures, and obtaining active ANME Mcr in vitro remains extremely challenging, preventing previous efforts to engineer this key enzyme. Here, we used directed evolution in the methanogen Methanosarcina acetivorans to enhance ANME-1 Mcr (McrANME-1) activity for methane and carbon dioxide capture by selecting McrANME-1 variants with improved growth during methane-dependent cultivation. As a result, we discovered two beneficial substitutions in the catalytic -subunit of McrANME-1, S60P and I154V, that increased biofilm growth as well as acetate production and methane capture. AlphaFold structural predictions suggest possible mechanistic explanations for these beneficial substitutions. These findings demonstrate that Mcr can be engineered to enhance methane and carbon dioxide capture, establishing a foundation for biological greenhouse gas mitigation and carbon utilization technologies.

Understanding transporter kinetics is essential for deciphering metabolite exchanges in biosystems, particularly for cells subject to substrate gradients. Nevertheless, the prediction of transporter kinetic parameters, maximum rate per gram protein (Vmax) and Michaelis-Menten constant (Km), has not yet been tackled. Here, we developed the first compound-protein interaction machine learning model of transporter Vmax and Km, MMTKPred, which achieved R2=0.553, RMSE=1.155 mmol/hr/g Protein and R2=0.330, RMSE=0.935 mM for log10-scaled Vmax and Km prediction, respectively. Moreover, we demonstrated MMTKPred's predictive power across biosystem scales, from capturing transporter kinetics modulated by point mutations and substrate changes at the molecular level, to enabling substrate-sensitive metabolic modelling of non-model yeasts at the cellular level, and rationalizing inter-species substrate competition in co-cultures. Collectively, MMTKPred effectively models metabolite transport spanning from molecular to multi-species scales, thereby offering a computational tool for rational microbial cell factory optimization.

Current cytosine base editors (CBEs) are limited to unidirectional C to T conversions, restricting their applications. Retrons, bacterial genetic elements, encode a reverse transcriptase that generates multicopy single-stranded DNA (msDNA) by reverse transcribing specific non-coding RNA (ncRNA). This msDNA mimics Okazaki fragments during DNA replication, making retrons promising for gene editing. Here, we developed a retron-based cytosine base editor (RCBE) by fusing cytosine deaminase with reverse transcriptase (RT-CDA) within the retron system. RCBE first transcribes ncRNA, allowing RT-CDA to deaminate cytosine on the ncRNA. The modified ncRNA is then reverse transcribed into msDNA, where RT-CDA induces further cytosine deamination. This mutant msDNA introduces specific mutations into target gene sequences, enabling both C to T and G to A conversions. Using RCBE, we demonstrated accelerated molecular evolution of the rpoB gene in Escherichia coli. High-throughput sequencing confirmed that RCBE achieves a mutation rate of up to 0.2% in regions with high GC content. Our findings establish RCBE as a versatile tool, particularly suitable for directed evolution in GC-rich regions, with broad potential applications across various bacterial and eukaryotic hosts.

NicA2 is a flavin-bound amine dehydrogenase from Pseudomonas putida S16 that converts nicotine to the pharmacologically inactive N-methylmyosmine. In animal models of nicotine addiction, injection of NicA2 can decrease nicotine-seeking behavior 10-fold. Accordingly, NicA2-related enzymes have been investigated as smoking-cessation therapeutics. However, efficient catalysis by NicA2 in Pseudomonas putida relies on electron transfer to CycN, a cytochrome c, and not directly to O2. Impractically high amounts of NicA2 are thus necessary to achieve a pharmacological effect in the absence of CycN. Directed evolution has improved the ambient-O2 value of kcat from 0.007 s-1 to 1 s-1 for NicA2, but further improvements have been challenging. Here, we identify a strain of Peribacillus frigoritolerans NIC8 which encodes two flavin amine oxidoreductases, Ncox and Pnox. In the presence of oxygen, Ncox and Pnox act on nicotine and pseudooxynicotine respectively with apparent kcat values of 7.7 s-1 and 3.9 s-1. Transient kinetics establishes bimolecular rate constants of 51100 M-1s-1 and 81000 M-1s-1 for the half-reactions between Ncox and O2 and between Pnox and O2 respectively, consistent with Ncox and Pnox being bona-fide oxidases. Transcriptomics shows enhanced expression of Ncox and Pnox under nicotine-dependent growth as well as supporting the identification of downstream enzymes. Phylogenetic analysis suggests that Ncox and Pnox arose out of repurposing of homologous enzymes found in Bacillus species. The enzymes we describe may be useful for the development of nicotine addiction therapeutics and for bioconversion of nicotine in waste streams.

Natural product (NPs) and their derivatives are a major source of small-molecule drugs, and the building blocks of these NPs are often amino acids. These include both proteinogenic and nonproteinogenic amino acids (NPAAs), the latter of which expand the structural diversity of NPs. Homologation, or the addition of a methylene group to the amino acid side chain, is one modification that generates NPAAs. If the natural homologation pathway can be characterized and engineered, it could be used to diversify NPs. In this study, we investigated the terminal enzyme of this pathway, HphB, to determine its substrate scope. HphB was tested with various substrates that differed in backbone and/or side chain structures relative to its natural substrate. The results showed that HphB exhibits high promiscuity toward substrates with different side chains while maintaining strict specificity for the substrate backbone. Comparative analysis with two homologous enzymes from primary metabolic pathways revealed that HphB displays markedly higher substrate promiscuity. Bioinformatics analysis and structural modeling suggest that this promiscuity arises from the absence of a "lid" over the active site, resulting in increased solvent exposure of the substrate side chain. This study highlights the unique substrate flexibility of HphB and is a step toward engineering the homologation pathway to generate amino acid derivatives.

BackgroundMicrobial chain-elongation by Clostridium kluyveri using the products (acetate and ethanol) derived from the electrocatalytic CO2 reduction reaction (CO2RR) represents a unique sustainable strategy for producing C4-C6 chemicals from CO2. However, direct integration of electrocatalytic effluents with anaerobic bioprocesses is often impeded by the physiological incompatibility between electrocatalytic product streams and microbial metabolism. Specifically, CO2RR effluents commonly contain formate, which cannot be utilized by C. kluyveri for chain elongation and therefore reduces the overall carbon efficiency of CO2 conversion to C4-C6 chemicals. Moreover, both formate and the elevated phosphate concentrations typical of electrochemical reaction solutions may inhibit microbial growth. ResultsWe show that formate at concentrations of up to 50 mM did not inhibit the growth of or the chain elongation by C. kluyveri. Based on this finding, we developed a modular two-step bioprocess. In the first step, the acetogen Clostridium ljungdahlii converts formate in CO2RR product mixtures into acetate, thereby generating additional substrates for second-step C. kluyveri-driven chain elongation, thus increasing the CO2RR carbon-conversion efficiency to C- C6 chemicals. To address the issue of C. ljungdahliis inhibition by high phosphate concentrations in electrocatalytic solutions, we explored the use of C. ljungdahlii biofilms for the first, i.e. the formate-conversion, step. C. ljungdahlii biofilms exhibit tolerance to concentrated electrolytes, enabling the conversion of up to 50 mM formate in CO2RR solutions. ConclusionsThe demonstrated two-step process constitutes the basis for the development of a robust and carbon-efficient biological process for the scalable upgrading of C1-C2 CO2RR products into higher-value C4-C6 chemicals.

The Clustered Regularly Interspaced Short Palindromic Repeats (CRISPR) and associated nuclease gene (Cas), originating from the bacteria acquired immune system, have revolutionized gene editing technology. In this regard, type II (Cas9) been extensively studied and widely applied CRISPR system so far. The mechanism for precise manipulation of genomic sequences is guided by small RNA called CRISPR RNA (crRNA). In this study we devised and optimized CRISPR-Cas9 screening system based on Cas9 gene detection, targeting a conserved part of recognition domain (REC) consisting of arginine rich bridge helix (BH). We used hemi-nested PCR approach for screening sensitivity and reproducibility. The recombinant E. coli DH5 alpha containing the pRGEB32 vector (DH5 alpha/pRGEB32) with the Cas9 gene was used for system optimization. Subsequently, the screening system was applied and validated on different environmental bacterial strains including Alcaligenes faecalis and Pseudomonas stutzeri, isolated from sewerage samples. The optimized hemi-nested PCR resulted in amplification of targeted region in environmental bacterial strains and results were reproduced successfully. Furthermore, nucleotides and amino acid sequence, motif and domain analysis of PCR products, confirmed the targeted Cas9 REC-BH domain. Presently, no rapid and cost effective CRISPR-Cas screening system is available except expensive whole genome sequencing approach. Our investigation aimed to device rapid and cost effective screening system for identification of new variants of Cas9 proteins in environmental bacterial species. In this context, the developed Cas9 gene-based CRISPR-Cas screening system (C9CSS) may be a potential rapid screening tool to identify new Cas9 orthologs in different bacterial genomes with improved functions.

The pulp and paper industry produces large volumes of condensed kraft lignin, which is challenging to convert to single chemical products. For this purpose, tandem chemical depolymerization and bioconversion to a single atom-efficient product is a potentially promising strategy. In this study, we conducted copper-catalyzed oxidative depolymerization using pine-derived kraft lignin to generate multiple bioavailable aromatic monomers at a yield of 4.5 weight% (wt%; g monomers per g lignin) from both C--O and C--C bond cleavage, followed by counter-current extraction with a 52 wt% monomer recovery. This resulted in an oxidized lignin product containing vanillin, vanillate, 4-hydroxybenzaldehyde, 4-hydroxybenzoate, 5-formylvanillin, 5-carboxyvanillin, 5-carboxyvanillate, acetovanillone, and vanillyl glyoxylate. Based on this stream composition, we engineered the industrially relevant soil bacterium Pseudomonas putida KT2440 to catabolize the latter five compounds via overexpression of ten heterologous genes (acvABCDEFSYK-6, vceABSYK-6, ligW2SYK-6, and mdlCPP). We combined these engineered pathways with previously reported strategies for muconate production from G- and H-type monomers to generate P. putida KMM428, which utilized 93.6 {+/-} 0.2 mol% of the quantified aromatic monomers in a depolymerized kraft lignin mixture, and produced muconate at a yield of 99 {+/-} 3 mol%, on a quantified monomer basis. Together, this work increases the theoretical carbon conversion efficiency of this process by 37.6 {+/-} 0.1 mol% through incorporation of three {beta}-5 cleavage products, in addition to traditional G-type monomers.

DNA assembly is a cornerstone of synthetic biology, enabling the construction of bespoke genetic systems for applications ranging from metabolic engineering to DNA nanotechnology. Conventional Gibson Assembly (GA), the most widely used method, relies on 5' exonucleolytic resection and elevated temperatures ([~]50 {degrees}C), which together prevent the retention of 5' modifications and restrict compatibility with temperature-sensitive functionalities. Here, we report a DNA assembly strategy, 3 exonuclease-mediated low-temperature DNA assembly (3LTDA), which generates complementary 5' overhangs while preserving 5' end integrity. This approach enables the efficient assembly of blunt-ended, 5'-functionalised DNA fragments into both linear and circular constructs at ambient temperature (21 {degrees}C), with some assembly observed at temperatures as low as 4{degrees}C. We systematically optimise reaction conditions and demonstrate that this method supports efficient plasmid re-circularisation and multi-fragment assembly, including the construction of a [~]12.5 kbp plasmid from multiple DNA components. Comparative analysis across several DNA substrates shows that, under their respective optimal conditions, this approach matches or exceeds GA performance, improving assembly efficiency by up to 12.8%. Sequence analysis confirms high fidelity with no detectable base-pairing errors across assembled junctions. Crucially, this method preserves chemically functionalised 5' termini, enabling downstream conjugation and biochemical functionality. Retention of azide and biotin modifications was verified through fluorescence imaging, bead-based co-localisation, and enzymatic activity in ELISA-based assays. This is in contrast to GA-assembled controls, which showed complete loss of functionality under comparable conditions. We further assembled 5 kbp dsDNA using 3LTDA from four independent segments, three with different fluorescence reporters, and the fourth containing a biotin group for microparticle conjugation, each on the 5 end. Under fluorescence illumination, bead-bound DNA with all three fluorescence markers were detected. Conventional GA assembled constructs, on the other hand, failed to retain the reporter groups and the fluorescent images did not show the presence of any fluorescent markers. In addition to enhanced performance, the method could also reduce reagent cost and eliminate the need for elevated temperatures, simplifying workflows and expanding the applicability of multi-functionalised DNA constructs. Collectively, this work establishes 3LTDA as a robust, low-temperature alternative to conventional GA, with advantages for applications requiring precise chemical modification, temperature-sensitive components, or deployment outside conventional laboratory environments.