The authors would like to acknowledge the following research support: EPSRC [EP/K038648/1] for SJM as a PDRA with PSF; Wellcome Trust sponsored ISSF fellowship for SJM with PSF at Imperial College London; Royal Society research grant [RGS\R1\191186]; Wellcome Trust SEED award [217528/Z/19/Z] for SJM at the University of Kent; and Global Challenges Research Fund (GCRF) Ph.D. scholarship for KC at the University of Kent.

NOTE: See Table 1 and Table 2 for recipes for GYM medium and agar plate and S30A and S30B wash buffers.
1. Preparation of solutions and general guidance
<ol>
	<li>Keep all solutions, cells (post-growth), and cell extracts on ice after preparation, unless an exception is stated.</li>
	<li>Store stocks for 1 M Mg-glutamate, 4 M K-glutamate, 40% (w/v) PEG 6000, 1&#160;g/mL polyvinylsulfonic acid at room temperature, and all other stocks at -80 &#176;C. Minimize the number of freeze-thaw cycles to avoid chemical degradation.</li>
	<li>For the preparation of energy solution stocks (see Table 3) such as 3-PGA (requires pH adjustment), follow the guidance provided in the E. coli TX-TL protocol41. 
	NOTE: All components are fully soluble in ddH2O and stored as aliquots in the -80 &#176;C freezer.</li>
	<li>Defrost individual stocks or energy solutions (described later) on ice. Heat the amino acids stock at 42 &#176;C with vortexing for ~15-30 min to solubilize all amino acids.</li>
	<li>As some amino acids (L-Cys, L-Tyr, L-Leu) precipitate on ice, while minimizing rest time, leave this solution at room temperature and use a vortex to dissolve.</li>
	<li>Add the calculated volumes (Table 3) of stock solutions and water and mix well using a vortex.</li>
	<li>Aliquot the energy solution as 20-100 &#181;L aliquots per tube, or as desired, on ice and store at -80 &#176;C until further use.</li>
</ol>
2. Preparation of S. venezuelae ATCC 10712 cells
<ol>
	<li>Day 1-Media/buffer preparation and overnight pre-culture
	<ol>
		<li>Prepare 1 L of sterile GYM liquid medium in a 2 L baffled flask, as described in Table 1. See the Table of Materials for equipment/chemical/reagent sources.</li>
		<li>Prepare 1 x 50 mL of sterile GYM liquid medium in a 250 mL Erlenmeyer flask, as described in Table 1.</li>
		<li>Prepare 100 mL of 1 M HEPES-KOH pH 7.5, 100 mL of 1 M MgCl2, and 500 mL of 4 M NH4Cl solutions to make 1 L of S30A and 1 L of S30B wash buffers. See Table 2 for the recipes.</li>
		<li>Prepare the overnight pre-culture. Pre-warm the sterile 50 mL of GYM liquid medium in a 250 mL Erlenmeyer flask to 28 &#176;C for 30 min.</li>
		<li>Inoculate a single colony of S. venezuelae ATCC 10712 (or related strain) from a GYM agar plate into prewarmed 50 mL of GYM liquid medium and incubate at 28 &#176;C, 200 rpm for 16 h (overnight pre-culture).</li>
	</ol>
	</li>
	<li>Day 2-Prepare daytime pre-culture and main growth culture.
	<ol>
		<li>Pre-warm 50 mL of sterile GYM liquid medium in a 250 mL Erlenmeyer flask at 28 &#176;C for 30 min.</li>
		<li>Transfer 1 mL of overnight pre-culture into pre-warmed 50 mL of GYM liquid medium and incubate at 28 &#176;C, 200 rpm for 8 h (daytime pre-culture).</li>
		<li>After this growth period, check the OD600 in a spectrophotometer using a 1:10 dilution with sterile GYM medium in a 1 mL (1 cm path length) plastic cuvette. 
		NOTE: The OD600 should have reached at least 3-4. If there is poor growth, it is advisable to repeat steps 2.2.1-2.2.2.</li>
		<li>Sub-culture 0.25 mL of daytime pre-culture into 1 L of liquid GYM medium in 2 L baffled flasks.</li>
		<li>Shake overnight at 28 &#176;C, 200 rpm for 14 h.</li>
	</ol>
	</li>
	<li>Day 3-Harvest cells
	<ol>
		<li>After the previous incubation period (14 h), record the OD600 of the main culture. Dilute the overnight culture 1:10 with fresh GYM medium for OD600 measurement. 
		NOTE: The OD600 should have reached 3.0-4.0 at this stage.</li>
		<li>If OD600&#60;3.0, increase the shaking speed to 250-300 rpm and grow until an OD600 of 3.0 is reached. Grow for no longer than an additional 2 h (16 h in total).</li>
		<li>If OD600&#62;3.0, transfer the cultures to centrifugation containers and rapidly cool on wet ice for 30 min.</li>
		<li>While waiting for the cell culture to cool on ice, prepare 4 mL of fresh 1 M dithiothreitol (DTT), S30A and S30B buffers, as described in Table 1, and keep them on ice. See the Table of Materials for chemical/reagent source.</li>
		<li>Pre-weigh an empty 50 mL centrifuge tube and pre-chill at -20 &#176;C.</li>
		<li>Add 2 mL of 1 M DTT to 1 L of S30A buffer on ice and mix well. 
		NOTE: Add DTT to the S30A and S30B wash buffers only before using them.</li>
		<li>Centrifuge cells at 6,000 &#215; g, 4 &#176;C, 10 min, and carefully discard the supernatant in a quick and single motion. 
		NOTE: If the pellet is disturbed, maximize cell retention with residual GYM medium and continue the protocol.</li>
		<li>Add 500 mL of S30A buffer and resuspend the cells by shaking the centrifugation bottles vigorously until the cell clumps are homogeneously dispersed.</li>
		<li>Centrifuge the cells at 6,000 &#215; g, 4 &#176;C, 6 min, and carefully discard the supernatant. 
		NOTE: Although the cell pellet will be firmer at this point, some cells will remain in suspension (see Figure 1). Treat as described in 2.3.7 and retain as many cells as possible.</li>
		<li>Repeat steps 2.3.8-2.3.9.</li>
		<li>Add 2 mL of 1 M DTT to 1 L of S30B buffer on ice and mix well. Add 500 mL of S30B buffer to the cells. Repeat step 2.3.9.</li>
		<li>Resuspend the cell pellet in 10 mL of S30B buffer and transfer to the pre-weighed, pre-chilled 50 mL centrifuge tube. If required, transfer the residual cells with an additional 5-10 mL of S30B buffer. Fill to 50 mL with S30B.</li>
		<li>Centrifuge cells at 6,000 &#215; g, 4 &#176;C, 10 min, and carefully discard the supernatant.</li>
		<li>Repeat step 2.3.13.</li>
		<li>Carefully aspirate the remaining S30B supernatant with a 100-200 &#181;L pipette.</li>
		<li>Weigh the wet cell pellet. 
		NOTE: Typical wet cell pellet weight for 1 L of overnight GYM culture (OD600 = 3.0) is ~4.5 g.</li>
		<li>For every 1 g of wet cells, add 0.9 mL of S30B buffer. Resuspend the cells using either a Pasteur pipette or vortex.</li>
		<li>Centrifuge briefly (~10 s) up to 500 &#215; g to sediment the cells. 
		NOTE: The protocol can be paused at this point, and cells can be frozen on either liquid nitrogen or dry ice and stored at -80&#176;C. For safety, wear appropriate personal protective equipment (PPE) when handling liquid nitrogen, including face shields and gloves.</li>
	</ol>
	</li>
</ol>
3. Cell lysis by sonication to obtain the crude cell extract
NOTE: At this stage, the user can choose to disrupt the cells by sonication either in 1 mL fractions (option 1) or as a larger cell suspension (5 mL) in a 50 mL tube (option 2). Both options have been detailed below to ensure reproducibility, as the final volume of the cell suspension can change due to the loss of cells during previous harvesting and wash steps. A new user should attempt option 2.1 first to establish the protocol.
<ol>
	<li>Cell Lysis by sonicating in 1 mL fractions
	<ol>
		<li>Using a 1 mL pipette tip (cut off the end of the tip to increase the bore size), transfer 1 mL of the cell suspension into 2 mL microcentrifuge tubes. 
		NOTE: If the cells are frozen, rapidly thaw the 50 mL tube containing the pellet in lukewarm water prior to cell lysis. Transfer the tube to wet ice as soon as the pellet has begun to defrost, and chill for 10 min.</li>
		<li>Place each microcentrifuge tube in a beaker of ice water, using a plastic tube rack to hold the tube for sonication. 
		NOTE: Due to the sensitivity of the cell extract to overheating, it is critical to ensure that the tubes do not warm up to prevent protein precipitation and reduced enzymatic activity.</li>
		<li>Use a sonicator probe with a 3 mm diameter tip and clean it with 70% (v/v) ethanol and double-distilled water (ddH2O). Lower the sonicator tip into the cell suspension until it is ~1 cm below the liquid surface.</li>
		<li>Input the following settings into the sonicator: 20 kHz frequency, 65% amplitude, 10 s pulse ON time, 10 s pulses OFF time, 1 min total sonication time.</li>
		<li>Run the sonication protocol. Move the tube up/down and sideways during the first two resting cycles to ensure the cells are evenly sonicated. Record the energy input. 
		NOTE: For safety, wear appropriate hearing protection during sonication. The viscosity will decrease as cells are disrupted, and the pale cream wet cell pellet should turn into a homogenous brown fluid. The recommended energy input is 240 J per mL of wet cells. If the cells are only partially lysed, the suspension will still appear cream-colored with viscous clumps of cells, particularly on the sides of the tube.</li>
		<li>Invert the tube 2-3 times and repeat the sonication for an additional one or two 10 s cycles, mixing frequently until the cells are fully disrupted.</li>
	</ol>
	</li>
	<li>Cell Lysis by sonicating a 5 mL cell suspension
	<ol>
		<li>If the cells are frozen, rapidly thaw the 50 mL tube containing the pellet in lukewarm water with shaking before cell lysis. Transfer the tube to wet ice as soon as the pellet has begun to defrost, and chill for 10 min.</li>
		<li>Briefly spin the tube at 500 x g to sediment the cells.</li>
		<li>Place the 50 mL tube in a beaker of ice water for sonication. 
		NOTE: Due to the sensitivity of the cell extract to overheating, it is critical to ensure that the tubes do not warm up to prevent protein precipitation and reduced enzymatic activity.</li>
		<li>Use a sonicator probe with a 6 mm diameter tip and clean it with 70% (v/v) ethanol and ddH2O (see the visual schematic of 6 mm probe in Figure 1). Lower the sonicator tip into the cell suspension (~5 mL) until it is ~1 cm below the liquid surface.</li>
		<li>Input the following settings into the sonicator: 20 kHz frequency, 65% amplitude, 10 s pulse ON time, 10 s pulses OFF time, 1 min total sonication time per mL of wet cells (5 min in total).</li>
		<li>Run the sonication protocol. Move the tube up/down and sideways during the first two resting cycles to ensure the cells are evenly sonicated. 
		NOTE: For safety, wear appropriate hearing protection during sonication. The viscosity will decrease as the cells are disrupted, and the pale cream wet cell pellet should turn into a homogenous brown fluid. Record the energy input. An optimal energy input of 240 J per mL of wet cells (~1200 J in total from 5 min sonication) is recommended.</li>
		<li>If some cells remain intact, follow the guidance from step 3.1.5.</li>
		<li>Transfer the cell extracts into 2 mL microcentrifuge tubes.</li>
	</ol>
	</li>
</ol>
4. Cell extract clarification and run-off reaction
<ol>
	<li>Centrifuge the lysed cells at 16,000 &#215; g for 10 min at 4 &#176;C to remove the cell debris. Transfer the supernatant into 1.5 mL microcentrifuge tubes as 1 mL aliquots.</li>
	<li>Perform the run-off reaction for the cell extracts. Incubate the 1.5 mL tubes containing the cell extracts at 30 &#176;C for 60 min on a heat block or incubator without shaking.</li>
	<li>Centrifuge the cell extracts at 16,000 &#215; g for 10 min at 4 &#176;C. Pool the supernatants into a 15 mL centrifuge tube. Mix the supernatant by inverting the tube five times until homogenous, then keep it on ice. Invert gently to avoid the formation of air bubbles.</li>
	<li>Dilute 10 &#181;L of the cell extract 100-fold with S30B buffer and measure the total protein concentration using a Bradford assay with three technical repeats (see Supplemental Material S2 for Bradford assay guidance).</li>
	<li>If the protein concentration is 20-25 mg/mL, transfer the cell extracts as 100 &#181;L aliquots into new 1.5 mL tubes, flash-freeze in liquid nitrogen, and store at -80 &#176;C. 
	NOTE: For safety, wear appropriate PPE when handling liquid nitrogen, including face shields and gloves.</li>
	<li>If the protein concentration is &#60;20 mg/mL, repeat the crude extract preparation steps to ensure high-quality cell extract and TX-TL yields are comparable to the previously published work5.</li>
</ol>
5. Preparation of plasmid DNA template
<ol>
	<li>Purify the pTU1-A-SP44-mScarlet-I plasmid (pUC19 origin) from a freshly transformed E. coli plasmid strain (DH10&#946;, JM109) grown in 50 mL of LB culture (with 100 mg/mL carbenicillin) using an appropriate plasmid DNA purification kit as per manufacturer&#39;s instructions.</li>
	<li>Elute the plasmid in 2 x 300 &#181;L of nuclease-free water and combine the fractions.</li>
	<li>Add 0.1 volumes (66 &#956;L) of 3 M sodium acetate (pH 5.2).</li>
	<li>Add 0.7 volumes (462 &#956;L) of isopropanol.</li>
	<li>Incubate the DNA at -20 &#176;C for 30 min.</li>
	<li>Centrifuge at 16,000 &#215; g for 30 min at 4 &#176;C and discard the supernatant.</li>
	<li>Add 2 mL of 70% (v/v) ethanol to the DNA pellet.</li>
	<li>Invert the tube 3-4 times to resuspend the plasmid DNA pellet.</li>
	<li>Centrifuge at 16,000 &#215; g for 5 min at 4 &#176;C and discard the supernatant.</li>
	<li>Repeat steps 5.7-5.9 and remove all visible liquid.</li>
	<li>Air-dry the DNA pellet for 10-30 min or dry for 5 min with a vacuum centrifuge.</li>
	<li>Resuspend the dried pellet with 600 &#181;L of nuclease-free ddH2O.</li>
	<li>Measure the DNA concentration and purity using a spectrophotometer.</li>
	<li>Prepare 50-100 &#181;L aliquots and store at -20 &#176;C. 
	&#8203;NOTE: A high DNA concentration in the range of 500-1000 ng/&#181;L is recommended due to the tight volume constraints of cell-free reactions. Dilute the plasmid DNA stock to 80 nM; 168 ng/&#181;L pTU1-A-SP44-mScarlet-I plasmid is equivalent to 80 nM.</li>
</ol>
6. Preparation of the Streptomyces Master Mix (SMM) solution
<ol>
	<li>Amino acid solution
	<ol>
		<li>Use the amino acid sampler kit to avoid manual errors and reduce preparation time, following the manufacturer&#39;s instructions provided online.</li>
		<li>Dilute the 20x amino acid stock solution using ddH2O to a final concentration of 6 mM (5 mM L-Leu).</li>
		<li>Further dilute to 2.4 mM (2 mM L-Leu) within the 2.4x SMM solution (see Table 3). 
		&#8203;NOTE: The final concentration in the TX-TL reaction is 1 mM 19x amino acids and 0.83 mM L-Leu.</li>
	</ol>
	</li>
	<li>Energy solution and additives
	<ol>
		<li>Prepare the other components in the 2.4x SMM solution by following the recipe described in Table 3.</li>
		<li>Alternatively, prepare a 2.4x Minimal Energy Solution (MES), following the recipe described in Table 3.</li>
	</ol>
	</li>
</ol>
7. Setting up a standard S. venezuelae TX-TL reaction
<ol>
	<li>Thaw the cell extract, SMM (or MES) solution, and plasmid DNA on ice. Pre-chill a 384-well plate at -20 &#176;C.</li>
	<li>Set up TX-TL reactions where 25% of the volume is plasmid DNA, 33.33% is cell extract, and 41.67% is SMM solution; keep them on ice to avoid start time bias. 
	NOTE: A standard TX-TL template has been provided (Table 4) to calculate the volume of reagents needed based on the number of reactions. The standard volume for a 33 &#181;L reaction is as follows: 11 &#181;L of cell extract, 13.75 &#181;L of SMM, and 8.25 &#181;L of plasmid DNA.</li>
	<li>Gently vortex the mixture for ~5 s at a low-speed setting to ensure the solution is homogenous. Avoid foaming/bubble formation.</li>
	<li>Transfer 10 &#181;L aliquots into three wells of a 384-well plate as a technical triplicate without introducing air bubbles. Seal the plate with a transparent cover and spin at 400 &#215; g for 5 s.</li>
	<li>Incubate the reaction at 28 &#176;C either in an incubator (for end-point readings) or a plate-reader without shaking. 
	NOTE: Reactions typically require 3-4 h to reach completion. See Supplemental Material S2 for guidance on a plate reader and mScarlet-I standard measurements.</li>
</ol>

The authors declare that they have no competing financial interests.

In this manuscript, a high-yield S. venezuelae TX-TL protocol has been described with detailed steps that are straightforward to conduct for both experienced and new users of TX-TL systems. Several features from existing Streptomyces45 and E. coli TX-TL41 protocols have been removed to establish a minimal, yet high-yield protocol for S. venezuelae TX-TL5,26. The workflow recommend...

Cell-free transcription-translation (TX-TL) systems provide an ideal prototyping platform for synthetic biology to implement rapid design-build-test-learn cycles, the conceptual engineering framework for synthetic biology1. In addition, there is growing interest in TX-TL systems for high-value recombinant protein production in an open-reaction environment2, for example, to incorporate non-standard amino acids in antibody-drug conjugates3. Specifically, TX-TL requires a cell extract, plasmid or linear DNA, and an energy solution to catalyze protein synthesis in batch or semicontinuous reactions. While Escherichia coli TX-TL is the dominant cell-free system, a number of emerging non-model TX-TL systems have attracted attention for different applications4,5,6,7,8. Key advantages of TX-TL include flexible scalability (nanoliter to liter scale)9,10, strong reproducibility, and automated workflows8,11,12. In particular, automation of TX-TL permits the accelerated characterization of genetic parts and regulatory elements8,12,13.
In terms of reaction setup, TX-TL requires both primary and secondary energy sources, as well as amino acids, cofactors, additives, and a template DNA sequence. Nucleotide triphosphates (NTPs) provide the primary energy source to drive initial mRNA (ATP, GTP, CTP, and UTP) and protein synthesis (only ATP and GTP). To increase TX-TL yields, NTPs are regenerated through the catabolism of a secondary energy source, such as maltose14, maltodextrin15, glucose14, 3-phosphoglycerate (3-PGA)16, phosphoenolpyruvate17, and L-glutamate18. This inherent metabolic activity is surprisingly versatile, yet poorly studied, especially in emerging TX-TL systems. Each energy source has distinct properties and advantages in terms of ATP yield, chemical stability, and cost, which is an important consideration for scaled-up TX-TL reactions. So far, current protocols for E. coli TX-TL have reached up to 4.0 mg/mL (~157 &#181;M) for the model green fluorescent protein (GFP), using a blend of 3-PGA (30 mM), maltodextrin (60 mM), and D-ribose (30 mM) as the secondary energy source19.
Recently, there has been a rising interest in studying secondary metabolite biosynthetic pathways in TX-TL systems20,21,22. Specifically, Actinobacteria are a major source of secondary metabolites, including antibiotics and agricultural chemicals23,24. Their genomes are enriched with so-called biosynthetic gene clusters (BGCs), which encode enzymatic pathways for secondary metabolite biosynthesis. For the study of Actinobacteria genetic parts and biosynthetic pathways, a range of Streptomyces-based TX-TL systems have recently been developed5,6,25,26. These specialized Streptomyces TX-TL systems are potentially beneficial for the following reasons: [1] provision of a native protein folding environment for enzymes from Streptomyces spp.26; [2] access to an optimal tRNA pool for high G+C (%) gene expression; [3] active primary metabolism, which potentially can be hijacked for the supply of biosynthetic precursors; and [4] provision of enzymes, precursors, or cofactors from secondary metabolism present in the native cell extract.&#160;Hence, a high-yield S.venezuelae TX-TL toolkit has recently been established to harness these unique capabilities5.
Streptomyces venezuelae is an emerging host for synthetic biology with a rich history in industrial biotechnology5,27,28,29 and as a model system for studying cell division and genetic regulation in Actinobacteria30,31,32.&#160;The main type strain, S. venezuelae ATCC 10712, has a relatively large genome of 8.22 Mb with 72.5% G+C content (%) (Accession number: CP029197), which encodes 7377 coding sequences, 21 rRNAs, 67 tRNAs, and 30 biosynthetic gene clusters27. In synthetic biology, S. venezuelae ATCC 10712 is an attractive chassis for the heterologous expression of biosynthetic pathways. Unlike most other Streptomyces stains, it provides several key advantages, including a rapid doubling time (~40 min), an extensive range of genetic and experimental tools5,28, lack of mycelial clumping, and sporulation in liquid media28,33. Several studies have also demonstrated the use of S. venezuelae for heterologous production of a diverse array of secondary metabolites, including polyketides, ribosomal and nonribosomal peptides34,35,36,37,38. These combined features make this strain an attractive microbial host for synthetic biology and metabolic engineering applications. While S. venezuelae is not the dominant Streptomyces model for heterologous gene expression, with further developments, it is primed for broader use within natural product&#160;discovery.
This manuscript presents a detailed protocol (Figure 1) for a high-yield S. venezuelae TX-TL system, which has been updated from the original previously-published protocol26. In this work, the energy solution and reaction conditions have been optimized to increase protein yield up to 260 &#956;g/mL for the mScarlet-I reporter protein in a 4 h, 10 &#956;L batch reaction, using a standard plasmid, pTU1-A-SP44-mScarlet-I. This plasmid has been specifically designed to enable various methods of detecting protein expression. The protocol is also streamlined, while the energy system has been optimized to reduce the complexity and cost of setting up cell-free reactions without compromising the yield. Along with the optimized TX-TL system, a library of genetic parts has been developed for fine-tuning gene expression and as fluorescent tools for monitoring TX-TL in real time, thereby creating a versatile platform for prototyping gene expression and natural product biosynthetic pathways from Streptomyces spp. and related Actinobacteria.
In this work, the recommended standard plasmid (pTU1-A-SP44-mScarlet-I) can be used to establish the S. venezuelae TX-TL workflow in a new laboratory and is available on AddGene (see Supplemental Table S1). pTU1-A-SP44-mScarlet-I provides the user with the flexibility to study other open-reading frames (ORFs). The mScarlet-I ORF is codon-optimized for S. venezuelae gene expression. The SP44 promoter is a strong constitutive promoter that is highly active in both E. coli and Streptomyces spp.39. The plasmid has two unique restriction enzyme sites (NdeI, BamHI) to allow the sub-cloning of new ORFs in-frame with a joint C-terminal FLAG-tag and fluorescein arsenical hairpin (FlAsH) binder tag system. Alternatively, both tags can be removed with the inclusion of a stop codon after sub-cloning a new gene. With this base vector, the high-yield expression of a range of proteins has been demonstrated, namely proteins from the oxytetracycline biosynthesis pathway and an uncharacterized nonribosomal peptide synthetase (NRPS) from Streptomyces rimosus (Figure 2). In terms of mRNA detection, the pTU1-A-SP44-mScarlet-I standard plasmid contains a dBroccoli aptamer (in the 3&#39;-untranslated region) for detection with the 3,5-difluoro-4-hydroxybenzylidene imidazolinone (DFHBI) probe. For increased flexibility, a toolset of EcoFlex40-compatible MoClo parts has also been made available on AddGene, including an EcoFlex-compatible Streptomyces shuttle vector (pSF1C-A-RFP/pSF2C-A-RFP) and a range of pTU1-A-SP44 variant plasmids expressing superfolder green fluorescence protein (sfGFP), mScarlet-I, mVenus-I, and &#946;-glucuronidase (GUS). In particular, the pSF1C-A plasmid is derived from pAV-gapdh28 and is cured of BsaI/BsmBI sites for MoClo assembly. pSF1C-A-RFP/pSF2C-A-RFP is equivalent to pTU1-A-RFP/pTU2-A-RFP from EcoFlex40 but contains additional functionality for conjugation and chromosomal integration in Streptomyces spp. using the phiC31 integrase system28.
The first stage of the protocol involves the growth of the S. venezuelae ATCC 10712 or a closely related strain, cell harvest at mid-exponential phase, cell wash steps, and equilibration in S30A and S30B buffers. This stage requires three days, and the time for cell growth can be used to prepare the remaining components as described below. The harvested cells are then lysed by sonication, clarified, and undergo a run-off reaction. At this final stage of preparation, the cell extracts can be prepared for long-term storage at -80 &#176;C to minimize loss of activity. For the assembly of TX-TL reactions using this protocol, a Streptomyces Master Mix (SMM) is presented, with the option of a Minimal Energy Solution format (MES) that gives comparable yields. Further, it is recommended to streak a fresh culture of S. venezuelae ATCC 10712 from a -80 &#176;C glycerol stock onto a GYM agar plate and incubate at 28 &#176;C for at least 48-72 h until single colonies are visible. Only fresh cultures should be used for the following steps.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>2.5 L UltraYield Flask</td>
			<td>Thomson</td>
			<td>931136-B</td>
			<td></td>
		</tr>
		<tr>
			<td>3-PGA (&#62;93%)</td>
			<td>Sigma</td>
			<td>P8877</td>
			<td></td>
		</tr>
		<tr>
			<td>384 Well Black/Clear Bottom Plate</td>
			<td>ThermoFisher</td>
			<td>10692202</td>
			<td></td>
		</tr>
		<tr>
			<td>Ammonium chloride (98%)</td>
			<td>Fluorochem</td>
			<td>44722</td>
			<td></td>
		</tr>
		<tr>
			<td>ATP, CTP, UTP, GTP (100 mM solution, &#62;99%)</td>
			<td>ThermoFisher</td>
			<td>R0481</td>
			<td></td>
		</tr>
		<tr>
			<td>Carbenicillin (contact supplier for purity)</td>
			<td>Melford</td>
			<td>C46000-25.0</td>
			<td></td>
		</tr>
		<tr>
			<td>D-(+)-glucose (contact supplier for purity)</td>
			<td>Melford</td>
			<td>G32040</td>
			<td></td>
		</tr>
		<tr>
			<td>DFHBI (&#8805;98% - HPLC)</td>
			<td>Sigma</td>
			<td>SML1627</td>
			<td></td>
		</tr>
		<tr>
			<td>DTT (contact supplier for purity)</td>
			<td>Melford</td>
			<td>MB1015</td>
			<td></td>
		</tr>
		<tr>
			<td>FlAsH-EDT2 (contact supplier for purity)</td>
			<td>Santa Cruz Biotech</td>
			<td>sc-363644</td>
			<td></td>
		</tr>
		<tr>
			<td>Glucose-6-phosphate (&#62;98%)</td>
			<td>Sigma</td>
			<td>G7879</td>
			<td></td>
		</tr>
		<tr>
			<td>HEPES Free Acid (contact supplier for purity)</td>
			<td>Melford</td>
			<td>B2001</td>
			<td></td>
		</tr>
		<tr>
			<td>L-glutamic acid hemimagnesium salt tetrahydrate (&#62;98%)</td>
			<td>Sigma</td>
			<td>49605</td>
			<td></td>
		</tr>
		<tr>
			<td>Magnesium chloride (98%)</td>
			<td>Fluorochem</td>
			<td>494356</td>
			<td></td>
		</tr>
		<tr>
			<td>Malt extract</td>
			<td>Sigma</td>
			<td>70167-500G</td>
			<td></td>
		</tr>
		<tr>
			<td>PEG-6000</td>
			<td>Sigma</td>
			<td>807491</td>
			<td></td>
		</tr>
		<tr>
			<td>Pierce 96-well Microdialysis Plate, 10K MWCO</td>
			<td>ThermoFisher</td>
			<td>88260</td>
			<td></td>
		</tr>
		<tr>
			<td>Poly(vinyl sulfate) potassium salt</td>
			<td>Sigma</td>
			<td>271969</td>
			<td></td>
		</tr>
		<tr>
			<td>Potassium glutamate (&#62;99%)</td>
			<td>Sigma</td>
			<td>G1149</td>
			<td></td>
		</tr>
		<tr>
			<td>RTS amino acid sampler</td>
			<td>5 Prime</td>
			<td>2401530</td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium chloride (99%)</td>
			<td>Fluorochem</td>
			<td>94554</td>
			<td></td>
		</tr>
		<tr>
			<td>Supelclean LC-18 SPE C-18 SPE column (1 g)</td>
			<td>Sigma</td>
			<td>505471</td>
			<td></td>
		</tr>
		<tr>
			<td>Yeast Extract</td>
			<td>Melford</td>
			<td>Y1333</td>
			<td></td>
		</tr>
		<tr>
			<td>Equipment</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Platereader</td>
			<td>BMG</td>
			<td>Omega</td>
			<td></td>
		</tr>
	</tbody>
</table>

a high-yield streptomyces transcription-translation toolkit for synthetic biology and natural product applications

Streptomyces spp. are a major source of clinical antibiotics and industrial chemicals. Streptomyces venezuelae ATCC 10712 is a fast-growing strain and a natural producer of chloramphenicol, jadomycin, and pikromycin, which makes it an attractive candidate&#160;as a next-generation synthetic biology chassis. Therefore, genetic tools that accelerate the development of S. venezuelae ATCC 10712, as well as other Streptomyces spp. models, are highly desirable for natural product engineering and discovery. To this end, a dedicated S. venezuelae ATCC 10712 cell-free system is provided in this protocol to enable high-yield heterologous expression of high G+C (%) genes. This protocol is suitable for small-scale (10-100 &#956;L) batch reactions in either 96-well or 384-well plate format, while reactions are potentially scalable. The cell-free system is robust and can achieve high yields (~5-10 &#956;M) for a range of recombinant proteins in a minimal setup. This work also incorporates a broad plasmid toolset for real-time measurement of mRNA and protein synthesis, as well as in-gel fluorescence staining of tagged proteins. This protocol can also be integrated with high-throughput&#160;gene expression characterization workflows or the study of enzyme pathways from high G+C (%) genes present in Actinomycetes genomes.

This detailed protocol is provided as an example to help the user establish a Streptomyces TX-TL system based on the S. venezuelae ATCC 10712 model strain (Figure 1). The user may seek to study other Streptomyces strains; however, the growth/harvesting stages of other strains with longer doubling times or distinct&#160;growth preferences will need to be custom-optimized to achieve peak results. For the representative result, the mScarlet-I fluorescent protein from ...

Watch this Scientific Journal Video about A High-Yield Streptomyces Transcription-Translation Toolkit for Synthetic Biology and Natural Product Applications at JoVE.com

A High-Yield Streptomyces Transcription-Translation Toolkit for Synthetic Biology and Natural Product Applications

This protocol details an enhanced method for synthesizing high yields of recombinant proteins from a Streptomyces venezuelae cell-free transcription-translation (TX-TL) system.

A High-Yield Streptomyces Transcription-Translation Toolkit for Synthetic Biology and Natural Product Applications

Streptomyces spp. are a major source of clinical antibiotics and industrial chemicals. Streptomyces venezuelae ATCC 10712 is a fast-growing strain and a ...

a-high-yield-streptomyces-transcription-translation-toolkit-for

Microsoft Bing

Research

JoVE Journal

Bioengineering

3.9K Views.  South Kensington Campus. This protocol details an enhanced method for synthesizing high yields of recombinant proteins from a Streptomyces venezuelae cell-free transcription-translation (TX-TL) system. 

Video: A High-Yield Streptomyces Transcription-Translation Toolkit for Synthetic Biology and Natural Product Applications

A Toolkit to Enable Hydrocarbon Conversion in Aqueous Environments

This work puts forward a toolkit that enables the conversion of alkanes by Escherichia coli and presents a proof of principle of its applicability. The toolkit consists of multiple standard interchangeable parts (BioBricks)9 addressing the conversion of alkanes, regulation of gene expression and survival in toxic hydrocarbon-rich environments.
A three-step pathway for alkane degradation was implemented in E. coli to enable the conversion of medium- and long-chain alkanes to their respective alkanols, alkanals and ultimately alkanoic-acids. The latter were metabolized via the native &beta;-oxidation pathway. To facilitate the oxidation of medium-chain alkanes (C5-C13) and cycloalkanes (C5-C8), four genes (alkB2, rubA3, rubA4and rubB) of the alkane hydroxylase system from Gordonia sp. TF68,21 were transformed into E. coli. For the conversion of long-chain alkanes (C15-C36), theladA gene from Geobacillus thermodenitrificans was implemented. For the required further steps of the degradation process, ADH and ALDH (originating from G. thermodenitrificans) were introduced10,11. The activity was measured by resting cell assays. For each oxidative step, enzyme activity was observed.
To optimize the process efficiency, the expression was only induced under low glucose conditions: a substrate-regulated promoter, pCaiF, was used. pCaiF is present in E. coli K12 and regulates the expression of the genes involved in the degradation of non-glucose carbon sources.
The last part of the toolkit - targeting survival - was implemented using solvent tolerance genes, PhPFD&alpha; and &beta;, both from Pyrococcus horikoshii OT3. Organic solvents can induce cell stress and decreased survivability by negatively affecting protein folding. As chaperones, PhPFD&alpha; and &beta; improve the protein folding process e.g. under the presence of alkanes. The expression of these genes led to an improved hydrocarbon tolerance shown by an increased growth rate (up to 50%) in the presences of 10% n-hexane in the culture medium were observed.
Summarizing, the results indicate that the toolkit enables E. coli to convert and tolerate hydrocarbons in aqueous environments. As such, it represents an initial step towards a sustainable solution for oil-remediation using a synthetic biology approach.

A sustainable auto regulating bacterial system for the remediation of oil pollutions was designed using standard interchangeable DNA parts (BioBricks). An engineered E. coli strain was used to degrade alkanes via &beta;-oxidation in toxic aqueous environments. The respective enzymes from different species showed alkane degradation activity. Additionally, an increased tolerance to n-hexane was achieved by introducing genes from alkane-tolerant bacteria.

This work puts forward a toolkit that enables the conversion of alkanes by Escherichia coli and presents a proof of principle of its applicability. The ...

A Novel Stretching Platform for Applications in Cell and Tissue Mechanobiology

Tools that allow the application of mechanical forces to cells and tissues or that can quantify the mechanical properties of biological tissues have contributed dramatically to the understanding of basic mechanobiology. These techniques have been extensively used to demonstrate how the onset and progression of various diseases are heavily influenced by mechanical cues. This article presents a multi-functional biaxial stretching (BAXS) platform that can either mechanically stimulate single cells or quantify the mechanical stiffness of tissues. The BAXS platform consists of four voice coil motors that can be controlled independently. Single cells can be cultured on a flexible substrate that can be attached to the motors allowing one to expose the cells to complex, dynamic, and spatially varying strain fields. Conversely, by incorporating a force load cell, one can also quantify the mechanical properties of primary tissues as they are exposed to deformation cycles. In both cases, a proper set of clamps must be designed and mounted to the BAXS platform motors in order to firmly hold the flexible substrate or the tissue of interest. The BAXS platform can be mounted on an inverted microscope to perform simultaneous transmitted light and/or fluorescence imaging to examine the structural or biochemical response of the sample during stretching experiments. This article provides experimental details of the design and usage of the BAXS platform and presents results for single cell and whole tissue studies. The BAXS platform was used to measure the deformation of nuclei in single mouse myoblast cells in response to substrate strain and to measure the stiffness of isolated mouse aortas. The BAXS platform is a versatile tool that can be combined with various optical microscopies in order to provide novel mechanobiological insights at the sub-cellular, cellular and whole tissue levels.

We present in this article a novel stretching platform that can be used to investigate single cell responses to complex anisotropic biaxial mechanical deformation and quantify the mechanical properties of biological tissues.

Tools that allow the application of mechanical forces to cells and tissues or that can quantify the mechanical properties of biological tissues have ...

Light-mediated Formation and Patterning of Hydrogels for Cell Culture Applications

Click chemistries have been investigated for use in numerous biomaterials applications, including drug delivery, tissue engineering, and cell culture. In particular, light-mediated click reactions, such as photoinitiated thiol&#8722;ene and thiol&#8722;yne reactions, afford spatiotemporal control over material properties and allow the design of systems with a high degree of user-directed property control. Fabrication and modification of hydrogel-based biomaterials using the precision afforded by light and the versatility offered by these thiol&#8722;X photoclick chemistries are of growing interest, particularly for the culture of cells within well-defined, biomimetic microenvironments. Here, we describe methods for the photoencapsulation of cells and subsequent photopatterning of biochemical cues within hydrogel matrices using versatile and modular building blocks polymerized by a thiol&#8722;ene photoclick reaction. Specifically, an approach is presented for constructing hydrogels from allyloxycarbonyl (Alloc)-functionalized peptide crosslinks and pendant peptide moieties and thiol-functionalized poly(ethylene glycol) (PEG) that rapidly polymerize in the presence of lithium acylphosphinate photoinitiator and cytocompatible doses of long wavelength ultraviolet (UV) light. Facile techniques to visualize photopatterning and quantify the concentration of peptides added are described. Additionally, methods are established for encapsulating cells, specifically human mesenchymal stem cells, and determining their viability and activity. While the formation and initial patterning of thiol-alloc hydrogels are shown here, these techniques broadly may be applied to a number of other light and radical-initiated material systems (e.g., thiol-norbornene, thiol-acrylate) to generate patterned substrates.

We describe a sequential process for light-mediated formation and subsequent biochemical patterning of synthetic hydrogel matrices for three-dimensional cell culture applications. The construction and modification of hydrogels with cytocompatible photoclick chemistry is demonstrated. Additionally, facile techniques to quantify and observe patterns and determine cell viability within these hydrogels are presented.

Click chemistries have been investigated for use in numerous biomaterials applications, including drug delivery, tissue engineering, and cell culture. In ...

Using Synthetic Biology to Engineer Living Cells That Interface with Programmable Materials

We have developed an abiotic-biotic interface that allows engineered cells to control the material properties of a functionalized surface. This system is made by creating two modules: a synthetically engineered strain of E. coli cells and a functionalized material interface. Within this paper, we detail a protocol for genetically engineering selected behaviors within a strain of E. coli using molecular cloning strategies. Once developed, this strain produces elevated levels of biotin when exposed to a chemical inducer. Additionally, we detail protocols for creating two different functionalized surfaces, each of which is able to respond to cell-synthesized biotin. Taken together, we present a methodology for creating a linked, abiotic-biotic system that allows engineered cells to control material composition and assembly on nonliving substrates.

This paper presents a series of protocols for developing engineered cells and functionalized surfaces that enable synthetically engineered E. coli to control and manipulate programmable material surfaces.

We have developed an abiotic-biotic interface that allows engineered cells to control the material properties of a functionalized surface. This system is ...

Synthesis of Multi-walled Carbon Nanotubes Modified with Silver Nanoparticles and Evaluation of Their Antibacterial Activities and Cytotoxic Properties

In this study, multi-walled carbon nanotubes (MWCNTs) were treated with an aqueous sulfuric acid solution to form an oxygen-based functional group. Silver MWCNTs were prepared by the reductive deposition of silver from an aqueous solution of AgNO3 on the oxidized MWCNTs. Given the unique color of the CNTs, it was not possible to apply them to the minimum inhibitory concentration or mitochondrial toxicity assays to evaluate the toxicity and antibacterial properties, since they would interfere with the assays. The inhibition zone and minimum bactericidal concentration for the Ag-MWCNTs were measured and Live/Dead and Trypan Blue assays were used to measure the toxicity and antibacterial properties without interfering with the color of the CNTs.

In this study, antimicrobial nanomaterials were synthesized by acidic oxidation of multiwalled carbon nanotubes and subsequent reductive deposition of silver nanoparticles. Antimicrobial activity and cytotoxicity tests were performed with the as-prepared nanomaterials.

In this study, multi-walled carbon nanotubes (MWCNTs) were treated with an aqueous sulfuric acid solution to form an oxygen-based functional group. Silver ...

Formulating and Characterizing Lipid Nanoparticles for Gene Delivery using a Microfluidic Mixing Platform

Lipid-based drug carriers have been used for clinically and commercially available delivery systems due to their small size, biocompatibility, and high encapsulation efficiency. Use of lipid nanoparticles (LNPs) to encapsulate nucleic acids is advantageous to protect the RNA or DNA from degradation, while also promoting cellular uptake. LNPs often contain multiple lipid components including an ionizable lipid, helper lipid, cholesterol, and polyethylene glycol (PEG) conjugated lipid. LNPs can readily encapsulate nucleic acids due to the ionizable lipid presence, which at low pH is cationic and allows for complexation with negatively charged RNA or DNA. Here LNPs are formed by encapsulating messenger RNA (mRNA) or plasmid DNA (pDNA) using rapid mixing of the lipid components in an organic phase and the nucleic acid component in an aqueous phase. This mixing is performed using a precise microfluidic mixing platform, allowing for nanoparticle self-assembly while maintaining laminar flow. The hydrodynamic size and polydispersity are measured using dynamic light scattering (DLS). The effective surface charge on the LNP is determined by measuring the zeta potential. The encapsulation efficiency is characterized using a fluorescent dye to quantify entrapped nucleic acid. Representative results demonstrate the reproducibility of this method and the influence that different formulation and process parameters have on the developed LNPs.

Lipid nanoparticles are developed using a microfluidic mixing platform approach for mRNA and DNA encapsulation.

Lipid-based drug carriers have been used for clinically and commercially available delivery systems due to their small size, biocompatibility, and high ...

Open-source Toolkit: Benchtop Carbon Fiber Microelectrode Array for Nerve Recording

Conventional peripheral nerve probes are primarily fabricated in a cleanroom, requiring the use of multiple expensive and highly specialized tools. This paper presents a cleanroom "light" fabrication process of carbon fiber neural electrode arrays that can be learned quickly by an inexperienced cleanroom user. This carbon fiber electrode array fabrication process requires just one cleanroom tool, a Parylene C deposition machine, that can be learned quickly or outsourced to a commercial processing facility at marginal cost. This fabrication process also includes hand-populating printed circuit boards, insulation, and tip optimization. 
The three different tip optimizations explored here (Nd:YAG laser, blowtorch, and UV laser) result in a range of tip geometries and 1 kHz impedances, with blowtorched fibers resulting in the lowest impedance. While previous experiments have proven laser and blowtorch electrode efficacy, this paper also shows that UV laser-cut fibers can record neural signals in vivo. Existing carbon fiber arrays either do not have individuated electrodes in favor of bundles or require cleanroom fabricated guides for population and insulation. The proposed arrays use only tools that can be used at a benchtop for fiber population. This carbon fiber electrode array fabrication process allows for quick customization of bulk array fabrication at a reduced price compared to commercially available probes.

Here, we describe fabrication methodology for customizable carbon fiber electrode arrays for recording in vivo in nerve and brain.

Conventional peripheral nerve probes are primarily fabricated in a cleanroom, requiring the use of multiple expensive and highly specialized tools. This ...

Fabrication of Size-Controlled and Emulsion-Free Chitosan-Genipin Microgels for Tissue Engineering Applications

Chitosan microgels are of significant interest in tissue engineering due to their wide range of applications, low cost, and immunogenicity. However, chitosan microgels are commonly fabricated using emulsion methods that require organic solvent rinses, which are toxic and harmful to the environment. The present protocol presents a rapid, non-cytotoxic, non-emulsion-based method for fabricating chitosan-genipin microgels without the need for organic solvent rinses. The microgels described herein can be fabricated with precise size control. They exhibit sustained release of biomolecules, making them highly relevant for tissue engineering, biomaterials, and regenerative medicine. Chitosan is crosslinked with genipin to form a hydrogel network, then passed through a syringe filter to produce the microgels. The microgels can be filtered to create a range of sizes, and they show pH-dependent swelling and degrade over time enzymatically. These microgels have been employed in a rat growth plate injury model and were demonstrated to promote increased cartilage tissue repair and to show complete degradation at 28 days in vivo. Due to their low cost, high convenience, and ease of fabrication with cytocompatible materials, these chitosan microgels present an exciting and unique technology in tissue engineering.

The present protocol describes a non-emulsion-based method for the fabrication of chitosan-genipin microgels. The size of these microgels can be precisely controlled, and they can display pH-dependent swelling, degrade in vivo,&#160;and be loaded with therapeutic molecules that release over time in a sustained manner, making them highly relevant for tissue engineering applications.

Chitosan microgels are of significant interest in tissue engineering due to their wide range of applications, low cost, and immunogenicity. However, ...

Cell-Free Expression of Membrane Proteins in Giant Unilamellar Vesicles

Reconstitution of the Bacterial Glutamate Receptor Channel by Encapsulation of a Cell-Free Expression System

Cell-free expression (CFE) systems are powerful tools in synthetic biology that allow biomimicry of cellular functions like biosensing and energy regeneration in synthetic cells. Reconstruction of a wide range of cellular processes, however, requires successful reconstitution of membrane proteins into the membrane of synthetic cells. While the expression of soluble proteins is usually successful in common CFE systems, the reconstitution of membrane proteins in lipid bilayers of synthetic cells has proven to be challenging. Here, a method for reconstitution of a model membrane protein, bacterial glutamate receptor (GluR0), in giant unilamellar vesicles (GUVs) as model synthetic cells based on encapsulation and incubation of the CFE reaction inside synthetic cells is demonstrated. Utilizing this platform, the effect of substituting the N-terminal signal peptide of GluR0 with proteorhodopsin signal peptide on successful cotranslational translocation of GluR0 into membranes of hybrid GUVs is demonstrated. This method provides a robust procedure that will allow cell-free reconstitution of various membrane proteins in synthetic cells.

Author Spotlight: Membrane Protein Reconstitution in Synthetic Cells

This protocol describes the inverted emulsion method used to encapsulate a cell-free expression (CFE) system within a giant unilamellar vesicle (GUV) for the investigation of the synthesis and incorporation of a model membrane protein into the lipid bilayer.

Cell-free expression (CFE) systems are powerful tools in synthetic biology that allow biomimicry of cellular functions like biosensing and energy ...

Versatile Biomolecular Condensates from Amphiphilic DNA Nanostars or C-Stars

Synthetic Condensates and Cell-Like Architectures from Amphiphilic DNA Nanostructures

Synthetic droplets and condensates are becoming increasingly common constituents of advanced biomimetic systems and synthetic cells, where they can be used to establish compartmentalization and sustain life-like responses. Synthetic DNA nanostructures have demonstrated significant potential as condensate-forming building blocks owing to their programmable shape, chemical functionalization, and self-assembly behavior. We have recently demonstrated that amphiphilic DNA "nanostars", obtained by labeling DNA junctions with hydrophobic moieties, constitute a particularly robust and versatile solution. The resulting amphiphilic DNA condensates can be programmed to display complex, multi-compartment internal architectures, structurally respond to various external stimuli, synthesize macromolecules, capture and release payloads, undergo morphological transformations, and interact with live cells. Here, we demonstrate protocols for preparing amphiphilic DNA condensates starting from constituent DNA oligonucleotides. We will address (i) single-component systems forming uniform condensates, (ii) two-component systems forming core-shell condensates, and (iii) systems in which the condensates are modified to support in vitro transcription of RNA nanostructures.

Author Spotlight: Developing Synthetic Cells from Programmable Amphiphilic DNA Nanostructures

We present a protocol for preparing synthetic biomolecular condensates consisting of amphiphilic DNA nanostars starting from their constituent DNA oligonucleotides. Condensates are produced from either a single nanostar component or two components and are modified to sustain in vitro transcription of RNA from an embedded DNA template.

Synthetic droplets and condensates are becoming increasingly common constituents of advanced biomimetic systems and synthetic cells, where they can be ...