- Open Access
T7Max transcription system
Journal of Biological Engineering volume 17, Article number: 4 (2023)
Efficient cell-free protein expression from linear DNA templates has remained a challenge primarily due to template degradation. In addition, the yields of transcription in cell-free systems lag behind transcriptional efficiency of live cells. Most commonly used in vitro translation systems utilize T7 RNA polymerase, which is also the enzyme included in many commercial kits.
Here we present characterization of a variant of T7 RNA polymerase promoter that acts to significantly increase the yields of gene expression within in vitro systems. We have demonstrated that T7Max increases the yield of translation in many types of commonly used in vitro protein expression systems. We also demonstrated increased protein expression yields from linear templates, allowing the use of T7Max driven expression from linear templates.
The modified promoter, termed T7Max, recruits standard T7 RNA polymerase, so no protein engineering is needed to take advantage of this method. This technique could be used with any T7 RNA polymerase- based in vitro protein expression system.
The T7 promoter for the RNA polymerase of bacteriophage T7 consists of 18 base pairs of sequence (5’ – TAATACGACTCACTATAG – 3’ ) . Previous research identified the relationship between the sequence and transcriptional efficiency, which helped to strengthen the T7 system’s usability [2,3,4].
Due to the T7 system’s versatility, the T7 system can be used both in vivo and in a cell-free translation system (CFTS). For example, bacterial cell-free translation systems commonly use the T7 RNA polymerase alongside the endogenous sigma 70 system . Furthermore, cell-free translation system platforms derived from hosts other than bacteria are also coupled with the T7 transcription, like plant , mammalian , and insect  in vitro translation systems.
We investigated whether translation in a cell free transcription – translation system (TxTl) can be increased by improving the strength of the promoter. It has been shown that increasing plasmid concentration directly correlates with increased translation yields in bacterial TxTl . We reasoned that increasing the promoter strength, with all other components of the translation system being equal, should result in both an increase of protein abundance and an increased protection of the translation yield from the effects of the DNA template degradation by endogenous nucleases in TxTl. As DNA template is degraded by nucleases, the use of stronger promoter ensures higher mRNA abundance despite lower effective DNA template concentration.
Results and discussion
Due to the robustness and high popularity of T7 RNA polymerase, there has been a lot of effort in engineering T7 RNA polymerase promoter sequences [3, 10]. We began by investigating efficiency of several known T7 promoter variants (Table 1 and Table S1) [11, 12]. We constructed double stranded linear DNA templates coding for the broccoli fluorescent RNA aptamer  with each of the tested T7 promoter variants. The templates had no terminators, so all transcriptions were run-off terminated.
Each transcription reaction was analyzed on a urea PAGE gel with the product stained with DFHBI1T, the ligand for the aptamer. The resulting image shows only correctly folded full length aptamer products (Fig. 1a). The gel was then de-stained and stained again using the general nucleic acid stain Sybr Gold. This stain shows all nucleic acid present in the sample, including truncation products of transcription (Fig. 1c). Both DFHBI and Sybr stained gels were quantified, comparing the relative abundance of the full-length aptamer product to the total nucleic acid abundance in the sample (Fig. 1b and d).
We also performed time course fluorescent readout of transcription from all the tested promoters, measuring transcription fluorescence for 6 hours (Fig. 1e, and end point quantification shown on panel 1f). Three promoters showing the highest yields of fluorescent RNA product were chosen for direct comparison in the next steps: T7wt, Uhlenbeck 117 and T7Max.
After experiments shown on Fig. 1, we did not know which promoter (if any) will outperform the WT, so the name T7Max was not yet assigned to any sequence. For clarity, to avoid having the same sequence under two different names, we use label T7Max on all figures.
Next, we proceeded to test full translation efficiency, still using linear dsDNA template.
We constructed eGFP templates with each of the tested promoters, using UTR1 and T500 terminator sequences optimized for bacterial in vitro translation . The translation efficiency was measured by fluorescence of eGFP after an 8 hour reaction (Fig. 2a). We quantified the abundance of eGFP mRNA using RT qPCR (Fig. 2b). While the earlier aptamer transcription data indicated that Uhlenbeck 117 sequence might be the best one, we were surprised to discover that another promoter resulted in higher translation yield. One of the promoters provided a slightly higher protein product amount, and higher end point mRNA abundance. That promoter, with the sequence AATTCTAATACGACTCACTATAGGGA, which we named “T7Max” – is an improved T7 promoter variant.
Escherichia coli has many endogenous DNA nucleases , which make their way into the TxTl extract without losing activity  and thus cause degradation of linear DNA templates in TxTl. Several methods have been proposed for enabling linear template expression, mainly focused on blocking the activity of the RecBCD, one of the more well-characterized nucleases. Among those methods, the most popular are the addition of GamS protein  or small DNA Chi6  – both inhibiting RecBCD nuclease. Bacteria strains deficient in RecBCD were also reported, making TxTl extract without RecBCD nuclease activity [20,21,22].
We used both the Chi6 inhibitors, and the GamS protein inhibitor. We tested expression of eGFP under classic T7 and under T7Max, from the same linear templates described above, using either E. coli extract made in our lab (see Materials and methods for detailed protocol information), or MyTXTL, a commercial E. coli TxTl extract from Arbor Biosciences (Fig. 2c). All reactions were set up with identical DNA template concentrations and in each compared pair (T7 vs T7Max) all other conditions, like concentration of RecBCD inhibitor, were the same. In all cases, the T7Max promoter outperformed the classic T7 promoter, as measured by GFP fluorescence after an 8 hour reaction. In some cases, expression under the T7Max promoter was 5 times larger than expression under the classic T7 promoter (in cases of GamS experiments, Fig. 2c). In addition to fluorescence measurements, we confirmed via a Western Blot one sample for each of the tested conditions (Fig. 2d).
While both T7 and T7Max expression improved in presence of GamS, the use of GamS significantly improves expression of T7Max construct, having less effect on regular T7 promoter expression. In those experiments, in presence of GamS T7Max outperforms T7 threefold, while in absence of GamS and in Chi6 experiments the T7Max advantage was less than two fold. In our experiments, the effectiveness of GamS to suppress RecBCD was less reliable than reported in the original GamS paper. Specifically, we observed significant variability in effectiveness of GamS between different batches of TxTl, this variability was higher than the typical batch to batch variability seen between TxTl preparations. We find no satisfying explanation to why T7Max outperforms T7 significantly better with GamS inhibition of RecBCD compared to no inhibition and to Chi6 system.
After establishing that the T7Max promoter outperforms the classic T7 promoter in expression from linear DNA templates, we moved on to further characterizing the T7Max promoter in translation reactions.
We used two circular DNA plasmids using UTR1 and T500 terminator and eGFP, identical except for the sequence of the promoter. First, we compared the kinetics of eGFP translation in E. coli TxTl (Fig. 3a), and corresponding GFP end point mRNA abundance (Fig. 3c).
The T7Max promoter consistently provided a higher level of fluorescence and a higher copy number of mRNA than the classic T7 promoter. To ensure that the measured protein abundance is not a fluorescence artifact, we analyzed eGFP abundance via Western Blot (Fig. 3b) and then quantified the Western Blot gels (Fig. 3d). The T7Max promoter consistently produced higher protein abundance.
To further characterize performance of the T7Max promoter in cell-free protein expression reactions, we analyzed reactions at different temperatures. In addition to 30°C (the optimal E. c oli TxTl reaction temperature used throughout this paper), we analyzed reactions at 25°C and 37°C (Fig. 4a).
In all cases, T7Max produced more protein product, confirmed by RT qPCR measurements of mRNA abundance (Fig. 4b). The advantage of T7Max was largest at 30°C, the optimal TxTl temperature, however the qPCR data shows significantly higher abundance of mRNA produced from T7Max vs classic T7 at 37°C as well. We speculate that this discrepancy might be due to the generally decreased translation performance at higher temperatures – as indicated by most TxTl protocols suggesting the use of 30C as reaction temperature, instead of 37°C that one might expect from E. coli extract [20, 23, 24]. Our own data presented here (Fig. 4), indicate that increasing TxTl reaction temperature is detrimental to both T7 and T7Max expression, with T7Max being marginally more resistant to increased temperatures (especially comparing 25°C to 30°C reactions).
The analysis of mRNA abundance in a TxTl reaction over time (Fig. 4c) demonstrates that T7Max reactions contain more mRNA than classic T7, with the biggest difference visible at the 2-hour mark . We speculate this might be due to the interplay between mRNA synthesis and degradation.
We also investigated the influence of the T7 RNA polymerase concentration on translation performance (Fig. 4d). Comparing the T7Max promoter with the classic T7 promoter demonstrates that the T7Max promoter produces higher protein yield at higher T7 RNA polymerase concentrations. However, as the T7 RNA polymerase concentration decreases , the difference between the T7Max and classic T7 templates starts to even out. We speculate this is because at lower RNA polymerase concentrations, the polymerase concentration becomes the rate limiting factor. While T7Max provides more efficient translation, if there is not enough polymerase to bind to all DNA templates, the promoter strength becomes less significant.
To thoroughly characterize the difference in T7Max performance vs classic T7 performance, we expressed several different types of proteins differing in open reading frame size from 1650bp to 30bp (Fig. 5).
We expressed luciferases: firefly (Fig. 5a), Renilla (Fig. 5d) and Nanoluc  (Fig. 5f). We expressed viral coat protein RNA binding proteins PP7  (Fig. 5g) and MS2  (Fig. 5h). We expressed the protein OphA from Omphalotus olearius Jack-o'-Lantern mushroom (Fig. 5b). We expressed the DNA restriction enzyme EcoRI (Fig. 5c), and the kanamycin resistance protein (Fig. 5e). We also expressed the extremely small fluorescent protein aptamer, FlAsH aptamer, which binds an arsenic ligand  (Fig. 5i). Thus, we covered a wide range of protein sizes, and many possible mRNA folds.
In all cases, in addition to measuring the protein abundance after an 8 hour TxTl reaction, we performed RT qPCR analysis of mRNA abundance. In all cases, T7Max templates produced more protein and higher end point mRNA abundance (shown as lower Cq values) than classic T7 templates.
Cell-free translation systems are key components of most synthetic minimal cell designs . We tested the T7Max promoter in the cytoplasm of a synthetic cell: encapsulating E. c oli TxTl in POPC / cholesterol liposomes . We prepared samples of synthetic cells with phospholipid membranes, dyed red with Rhodamine-PE dye, and bacterial TxTl with eGFP -encoding plasmid under the control of either the classic T7 promoter or our T7Max promoter (Fig. 6). Imaging of the diluted samples clearly showed individual synthetic cell liposomes expressing GFP in the lumen (Fig. 6a and b). To increase the number of samples analyzed in each field of view, we also imaged undiluted samples, at higher concentrations of lipids (Fig. 6c and d). We quantified fluorescence from these images, measuring total fluorescence in the GFP channel to estimate protein production and then normalizing that value to total fluorescence in the red channel ( normalizing to the number of liposomes in each field of view). Synthetic cells expressing GFP under the T7Max promoter showed higher protein production than synthetic cells containing the classic T7 promoted GFP.
Next, we asked how will T7Max compare to classic T7 in other in vitro translation systems. Other in vitro translation systems are used for different applications [30, 31], including the PURE system composed of E. coli translation machinery purified individually , wheat germ extract , Leishmania tarentolae extract , insect Spodoptera frugiperda Sf21 cell line extract , and rabbit reticulocyte extract . All of those extracts are commercially available and were used according to the manufacturer’s protocols.
We created templates for eGFP expression in each of those cell-free systems, with the only difference between templates being the T7 RNA polymerase promoter: either T7Max or classic T7.
Because the absolute yields (measured as GFP fluorescence) were different in each extract, we normalized the results: the classic T7 promoter is assigned value 100, and the T7Max template fluorescence is proportionally scaled for each sample. For example, the raw fluorescence value for classic T7 promoter E. coli in this case was 9384, while T7Max value was 15671; normalizing T7 to 100 gives T7Max value of 167 (Fig. 7a). In all tested cases, the yield of protein synthesis was higher from a template using the T7Max promoter than from the template using the classic T7 promoter.
Finally, we looked to other applications for T7Max. Robust, sensitive, and transportable disease detection systems are in great need, and many rely on the amplification of nucleic acids . Apta-NASBA is an isothermal exponential disease detection reaction, dependent on the productivity of T7 RNA polymerase . In Apta-NASBA, primers introduce the T7 RNA polymerase promoter and result in a fluorescent read out via an RNA aptamer.
We designed Apta-NASBA primers to detect the aggR gene associated with enteroaggregative E. Coli, using T7Max, which contains features known to be of value in NASBA primers, such as no pyrimidine residues early in the transcript [11, 14], as well as a second set of primers using the canonical T7 RNAP promoter. All other reaction components were kept identical. Reactions where T7Max was incorporated created a 14X signal compared to a negative control (a reaction lacking template) vs 1.24X when incorporating classic T7 after 100 minutes (Fig. 7b). Such increase in signal can allow for a more sensitive detection reaction.
While T7Max consistently outperforms T7 promoter in expression from both linear and circular plasmids, as indicated by both protein activity or abundance (Western blot or activity assays), we observed significant increase in translation yields in the case of linear DNA templates with RecBCD nuclease inhibitor protein GamS. The T7Max shows remarkable improvement in translation yields under those single specific conditions. In expression from circular plasmids, T7Max consistently outperforms T7 (both in protein abundance and in qPCR measurements) by 20% to 100%; in GamS experiments T7Max outperforms T7 by more than 300%. The T7 advantage in expression from plasmids remains consistent for all proteins tested in this work, including data from all species of TxTl system we tested.
Cell free expression platforms find increasingly versatile applications in many areas of bioengineering, synthetic biology, and metabolic engineering [39,40,41]. Additionally, the focus for engineering synthetic minimal cells is on reconstituting in vitro translation reactions , most often with the use of a bacterial translation system and T7 RNA polymerase [42, 43]. Here we demonstrated a simple technique to enable a significant increase in translation yield via a change of the T7 promoter sequence.
This system utilizes all existing elements of T7 RNA polymerase-driven transcription without changes and only requires replacement of the promoter sequence in the construct.
We have demonstrated versatile utility of the T7Max promoter in multiple different cell-free protein expression systems and for proteins over a wide range of sizes and types, as well as significantly increased yields of protein synthesis from linear DNA templates.
While the sequence of the T7Max promoter has been known , the performance of this variant has not been characterized in details beyond the original transcription yield comparisons; this is the first comprehensive characterization of its use for in vitro transcription and translation. Our hope is this technology will enable further improvements in both transcription and in vitro protein expression to result in better biomedical, biotechnological, and synthetic cell engineering applications [44, 45].
Materials and methods
Construction of Tx Templates for Screen of Different Promoters
A series of T7 promoters described previously [1, 2, 11, 12], see Table 1 for sequences, were placed upstream of the broccoli coding sequence via primer extension. Sense strand primers with promoter sequences, the first 23 nucleotides of the broccoli coding sequence, and the anti-sense primers coding for broccoli (49 nucleotides) were synthesized (Integrated DNA Technologies) and brought to 10 μ M in Millipore water (GenPure Pro UV-TOC/UF). Bulldog Bio BioReady Taq DNA Polymerase (BSA12L010) was used according to manufacturer’s instructions with NEB dNTPs (N0446S). 9μL of PCR master mix reagents and anti-sense primer were combined with 1 μL of the promoter primer to give a primer-extension reaction of 1X Bulldog Reaction Buffer, 1 μM of both primers, 1 mM dNTPs, BioReady rTaq (0.05 U/μL). The reaction was denatured for 5 seconds at 95°C, annealed for 5 minutes at 60°C, and then extended for 30 min at 72°C (Bio-Rad T100 thermocycler). These reactions were generated in triplicate for each promoter tested, which served as a 10X stock of template in a transcription reaction.
The sequences used in transcription screening in this work differed from the original Uhlenbeck paper sequences testing the strength of various promoter variants. The relative order of promoter strength in our experiments is different than the earlier reported relative transcription yields. We speculate this might be due to the use of different sequences of the transcript. In our experiments, the transcript contained G quadruplex in Broccoli aptamer sequence. It is possible that there is, yet to be explored, variability in promoter strength vs transcribed sequence. Similarly, the promoter best in transcription experiments did not produce the absolute strongest translation result – providing more evidence to speculate about possible transcript sequence dependency.
The templates were then used as -is in a transcription assay. All reagents, tubes, and plates were pre-chilled on ice. A master mix of transcription reagents was prepared on ice, and 9 μL of the master mix and 1 μL of the 10X templates were combined in a 200 μ L PCR tube, flicked, spun down, and then transferred to a cold, clear bottom 384-well plate. The transcriptions (1X template, 1X Homemade NEB Buffer, 8 mM GTP, 4 mM A/C/UTP, 0.005X phosphatase 25 ng/μ L, 1 μ M T7 RNAP, 100 μ M DFHBI-1T, RNAse inhibitor 0.4 U/μ L) were incubated for 6 hours at 37°C in a SpectraMax Gemini XS microplate fluorimeter and data collected every 5 minutes (excitation: 488 nm, emission: 507 nm, PMT Medium). An endpoint measurement was taken and the transcriptions stored at -80°C.
The fluorescent data was correlated by resolving the transcriptions in a denaturing polyacrylamide gel. An 8M urea, 10% (19:1) PAGE was prerun for 30 minutes at 100V in a Mini PROTEAN tank (Bio-Rad) electrophoresis chamber using 1X TBE (89 mM Tris, 89 mM boric acid, 2 mM EDTA, pH 8.0). Transcriptions were diluted 1:1 with 2x TBE Loading Buffer (8 M urea, 89 mM Tris, 89 mM boric acid, 2 mM EDTA, pH 8.0) and the entire 20 μL sample was resolved for 1 hour at 125V. The gel was then equilibrated in 50 mL 1X folding buffer (1 mM MgCl2, 50 mM KCl, 10 mM Tris, pH 8.0) for 45 minutes. The buffer was then decanted, exchanged with 50 mL 1X folding buffer supplemented with 10 μ M DFHBI-1T, and incubated for 15 minutes at room temperature . The broccoli band was imaged on an Aplegen Omega Lum G using a SYBR Safe filter. The buffer was decanted as before and replaced with 1X Folding Buffer supplemented with 1X SYBR Gold (Thermo Scientific, S11494). After a 15 minute incubation at room temperature , the total RNA was imaged using the aforementioned filter.
Low range ssRNA Ladder (New England BioLabs, Cat no N0364S) and 10 pmol of broccoli were run alongside the transcriptions as controls. The RNA produced for both stain s was quantified using GelQuant.NET.
Construction of T7Max Plasmids
Double stranded T7Max promoter insert was formed from a pair of annealed 5’-phosphorylated primers. Primers were designed with 4 bp 5’ overhangs just upstream of a restriction enzyme digestion site, the forward primer containing the AgeI restriction site and the reverse primer containing the BglII restriction site, using Geneious 7.1.9 (https://www.geneious.com/) and purchased from IDT. For the promoter insert primers, the forward primer sequence was 5’-/5Phos/GATCTAATTCTAATACGACTCACTATAGGGAAATAATTTTGTTTAACTTTAAGAA-3’ and the reverse primer sequence was 5’-/5Phos/CCGGTATATCTCCTTCTTAAAGTTAAACAAAATTATTTCCCTATAGTGAGTCGTA-3’. The T7 promoter sequence was excised from the original plasmid backbone, UTR1-T7RNAP-T500 (Catalog No. 67739, Addgene), via restriction digestion with AgeI and BglII. The T7Max promoter was cloned into backbones containing the genes for eGFP, fluorescein arsenical hairpin (FlAsH) peptide, and Omphalotin A (OphA) by following NEB’s restriction digest protocol (NEB #R0744), 5’ dephosphorylation protocol (NEB #M0289) and T4 DNA ligase protocol (NEB #M0202). Ligated constructs were transformed into the E. c oli strain BL21(DE3) and plated on LB agar plates containing 100 μg/ml carbenicillin. Colony constructs were verified by sequencing.
C-terminus 6xHis-tagged proteins were expressed in vitro with transcription-translationally active E. c oli cell-free extract using the protocol described before . Constructs were expressed for 8 hours at 30°C using a Bio-Rad T100 thermo cycler running software version 1.201. Samples were mixed 1:1 with 2X SDS loading buffer (100 mM Tris HCl, 2.5% SDS, 20% Glycerol, 4% Beta -mercaptoethanol, 0.1% Bromophenol Blue). Mixtures of loading buffer and sample were boiled at 95°C for 5 minutes in a Bio-Rad T100 thermo cycler. Boiled samples were fractionated on a 37.5:1 Acrylamide:Bis-Acrylamide SDS-Page gel and then transferred to a 0.2 μ m nitrocellulose membrane using a Mini-PROTEAN tank (Bio-Rad) according to the manufacturer’s protocol. Gels were run for 60 minutes at 100V in 800 mL of 1X SDS running buffer (25mM Tris, 192mM Glycine, 3.5mM SDS). Gels were transferred for 60 minutes at 100V in 1L of 1X transfer buffer (25mM Tris, 192mM Glycine). Electrical current was provided by Bio-Rad Power Pac 3000. Membrane was incubated with 5% nonfat milk in TBST (20mM Tris, pH 7.4, 150mM NaCl, 0.05% tween) for 60 minutes on a horizontal rocker (Benchmark) before mouse IgG1 anti-his primary antibodies (1:5000), purchased from Biolegend, were added to the solution. The 5% nonfat milk TBST and mouse IgG1 mixture incubated with the membrane for 60 minutes on a horizontal rocker. After incubation with primary antibodies, the membrane was rinsed three times with TBST followed by three 10 min washes in TBST. The membrane was next added to 5% nonfat milk in TBST containing horseradish peroxidase-conjugate goat anti-mouse IgG1 secondary antibodies (Biolegend 405306) diluted at 1:5000 and incubated on a horizontal rocker for 60 minutes. After incubation with secondary antibodies, the membrane was rinsed three times with TBST followed by three 10 minute washes in TBST. Blots were developed with SuperSignal (Thermo Scientific) immunoblotting detection system according to manufacturer’s protocols. Blots were imaged using the ChemiDoc MP Imaging System (Bio-Rad) running Image Lab version 5.2.1.
Measuring promoter-dependent protein expression using cell-free TXTL
To prepare the E. coli cell extract and TXTL master mix, we followed the protocol outlined by Sun et al. . For extract preparation we used BL21(DE3) Rosetta strain of E coli, with the salt mix used as 130mM potassium glutamate, 10 mM ammonium acetate and 10 mM magnesium glutamate. All TxTl data showed on single figure were obtained using the same batch of TxTl extract, to avoid batch to batch variability between extract preparations. All bacterial TxTl experiments described in this paper were done using TxTl mix prepared this way, except the controls with commercially available MyTxTl (Arbor Biosciences).
The TxTl was prepared from a strain that contains genomic copy of T7 RNA polymerase under acUV5 promoter. We did not induce T7 expression growing the cells for TxTl prep, therefore we assume there was no basal T7 RNA polymerase in the TxTl prep. We added T7 RNA polymerase to the reactions from 25μ stock in 50% glycerol, purified according to the previously described protocol .
The eGFP, fluorescein arsenical hairpin (FlAsH) peptide, or Omphalotin A (OphA) genes with C-terminal His-tags were cloned into the UTR1-T7RNAP-T500 plasmid backbone (Catalog No. 67739, Addgene). The T7 Max promoter was further cloned into these plasmids for downstream experiments. The linear version of the eGFP plasmid was created through restriction enzyme digestion of the circular plasmid with BamHI. To measure the differences in protein expression between the two promoters, 10nM of templates with each promoter type were added to TXTL reactions and incubated at 30oC for 8 hours (T100 Thermal Cycler, Bio-Rad). Post-incubation, protein expression was determined through measurement of fluorescence (eGFP and FlAsH) or Western Blot (OphA). eGFP fluorescence was standardized to 1μ M fluorescein.
FlAsH peptide expression was determined through the addition of 5 μ M FlAsH dye and 20mM 2-(N-morpholino) ethanesulfonic acid (MES) buffer and were standardized to samples without the peptide. The excitation and emission spectra of FlAsH intersects with that of Chai Green Dye 20X (Catalog No. R01200, Chai Bio) in the subsequent quantitative polymerase chain reaction experiments, so 10 μL of the peptide’s TXTL reactions were saved for transcript quantification prior to determining expression levels.
Relative comparison of transcripts with Reverse Transcription-quantitative Polymerase Chain Reaction (RT-qPCR)
Template DNA in 10 μ L of the TXTL reaction was degraded by adding 0.5 μ L of TURBO DNase (2U/μ L, Catalog No. AM2238, Invitrogen). The mixture was incubated at 37oC for 30 minutes. The enzyme and the expressed proteins were inactivated by adding 15mM EDTA (Catalog No. E9884, Sigma-Aldrich) at 75oC for 10 minutes (T100 Thermal Cycler, Bio-Rad). The denatured proteins were pelleted through centrifugation at 3,200g for 2 minutes.
Forward and reverse primers (Integrated DNA Technologies), for each protein sample were created for downstream reverse transcription and qPCR experiments. The primers were designed based on our GFP sequences, using the IDT Oligo analyzer tool to match the melting temperatures of primer pair. Each primer pair was compatible for transcripts produced from the old promoter and T7 Max. For eGFP, the forward primer was 5’-AAGTTCATCTGCACCACC-3’ and the reverse primer was 5’-TTGAAGTCGATGCCCTTC-3’. For the FlAsH peptide, the forward primer was 5’-TATACCGGTATGTGGGACTG-3’ and the reverse primer was 5’-GATGGTGATGATGGTGATGG-3’. For OphA, the forward primer was 5’-ACGACAATGGCAAGTCCA-3’ and the reverse primer was 5’-GGAAATCCGATGCCTCGT-3’.
To prepare the reverse transcription reaction, 2 μL of the DNase-treated sample was mixed with 2 μL of 10 μM reverse primer, 4 μL of 5X Protoscript II Reverse Transcriptase Buffer, 1 μL of Protoscript II Reverse Transcriptase (200U/μL, Catalog No. M0368, New England BioLabs Inc.), 2 μL of 0.1M dithiothreitol (DTT), 1 μL of 10mM dNTP, 0.2 μL of RNase Inhibitor (Catalog No. M0314, New England BioLabs Inc.), and 8 μL of nuclease-free water. The reverse transcription reaction was incubated at 42oC for 1 hour and the reverse transcriptase was inactivated at 65 oC for 20 minutes.
The quantitative PCR reaction mix was prepared by mixing 2 μL of complementary DNA from the reverse transcription with 2 μL of 10 μM forward and reverse primers, 11.25 μL OneTaq Hot Start 2X Master Mix with Standard Buffer (Catalog No. M0484, New England BioLabs Inc.), 1.25 μL Chai Green Dye 20X (Catalog No. R01200, Chai Bio), and 7.5 μL of nuclease-free water. The qPCR was completed using Open qPCR (Chai Biotechnologies) with the following thermocycling program: 1 cycle of 30 second denaturation at 95oC, 30 cycles of 15 second denaturation at 95oC, 15 second annealing at 50oC, 1 minute extension at 68oC, and 1 cycle of 5-minute final extension at 68oC. The amplification curves plotted through the Open qPCR software to determine Cq values and averages across 3 replicates of each promoter type were calculated separately.
For experiments involving the kinetic determination of protein expression and transcript comparison, 50 μ L of TXTL reactions with 10 nM DNA templates were incubated at 30oC for 8 hours. Every 2 hours, including at the start of the incubation, 10 μ L samples were removed to measure protein expression and quantify transcription.
In any qPCR reaction, the lower Cq value indicates higher abundance of the analyzed sequence. While sometimes qPCR data is presented as relative RNA abundance after performing calibration curves, often the Cq values are presented directly. The latter approach is chosen in this work, to avoid any possible error introduced by the calibration curves and to show the data in the least processed form.
Promoter comparison using different extracts
To compare T7Max performance, we used commercially available PURE system (NEB), wheat germ extract (Promega), Leishmania tarentolae extract (Jena Bioscience), insect Spodoptera frugiperda Sf21 cell line extract (Promega), and rabbit reticulocyte extract (Promega). All of those extracts were used according to the manufacturer’s protocols.
To maintain directly comparable values, all translations were performed in uncoupled mode: the mRNA template was transcribed separately. To preserve the original transcription yields, the transcription reaction was not purified, concentrated, or altered in any way before adding equal volume aliquots of each T7 and T7Max transcription to the corresponding translation reactions.
The GFP template for E coli and PURE reactions was the same, PCR product from the T7 and T7Max GFP plasmids used in other experiments in this paper. We did not codon-optimize GFP for eukaryotic translation, because in those experiments we wished only to compare yield of GFP between T7 and T7Max. With both sequences in each comparison pair being non-codon optimized, the difference in expression can still be directly compared even though the absolute yields are lower than the yields from a codon-optimized gene. Wheat germ extract expression cassette was designed with UTR sequences based on Promega pF3 WG (BYDV) Flexi vector. Leishmania tarentolae extract expression cassette was designed with UTR sequences based on Jena pLEXSY_invitro-2 vector. Spodoptera frugiperda Sf21 cell line extract expression cassette was designed with UTR sequences based on Promega pF25K ICE T7 Flexi vector. All expression cassette sequences are in Table S1.
For the reported normalized fluorescence values, each three WT T7 expression values were averaged, and error was calculated. Then, this expression value was assigned arbitrary value of 100, and error was scaled accordingly. For example if the raw averaged value was 400 with error value of 40, after normalizing raw value of 400 to 100 the error would be normalized by the same factor, in this case divided by 4, to produce error bar with value 10.
Apta-NASBA reactions were performed as previously described, with 10nM input RNA . Primers used for the Apta-NASBA reaction were: Broccoli aptamer coding primer (broccoli is in italics) 5’-GAGCCCACACTCTACTCGACAGATACGAATATCTGGACCCGACCGTCTCCAGCGATACATTAAGACGCCTAAAG-3’ classic T7 primer (promoter is in italics) 5’-TAATACGACTCACTATAGCGTCAGCATCAGCTACAATTATTCC-3’ T7Max primer (promoter is in italics) 5'-AATTCTAATACGACTCACTATAGGGAGACGTCAGCATCAGCTACAATTATTCC-3’
Availability of materials
We deposited plasmids with T7 max promoter used in this work on Addgene, https://www.addgene.org/browse/article/28223150/. Maps of plasmids are available in Supporting Figure S3, S4, and S5.
Availability of data and materials
Please contact the authors for all data sets and plasmids. No data was generated that is suitable for public open source data repositories.
T7 RNA polymerase
Nucleic acid sequence-based amplification
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We thank Richard Murray for providing a sample of the GamS protein. We thank Vincent Noireaux for advice on T7 RNAP expression and on using Chi6 inhibitor system. We thank Michael Freeman for the gift of OphA protein from Omphalotus olearius Jack-o’-Lantern mushroom.
This work was supported by NIH award 5R01MH114031-02 RNA Scaffolds for Cell Specific Multiplexed Neural Observation, NASA award 80NSSC18K1139 Center for the Origin of Life - Translation, Evolution And Mutualism, John Templeton Foundation award 61184 Exploring the Informational Transitions Bridging Inorganic Chemistry and Minimal Life, NSF award 1840301 RoL:FELS:RAISE Building and Modeling Synthetic Bacterial Cells, and NSF award 1935372 Collaborative Research: Booting up a Mirror Cell.
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Additional file 1: Figure S1.
The original uncropped gels for data presented on Fig. 1. Sybr stained gel.
Additional file 2: Figure S2.
The original uncropped gels for data presented on Fig. 1. DFHBI stained gel.
Additional file 3: Figure S3.
Map of plasmid used in the TxTl experiments, pCI-T7Max-UTR1-deGFP-8xHis-T500.
Additional file 4: Figure S4.
Map of plasmid used in the TxTl experiments, pCI-T7Max-UTR1-NTerminus8xHis-T500.
Additional file 5: Figure S5.
Map of plasmid used in the TxTl experiments, pCI-T7Max-UTR1-CTerminus8xHis-T500.
Additional file 6: Figure S6.
The full uncropped Western Blot image of GFP expression comparison between T7 and T7Max. p1686 is T7 and p2008 is T7Max promoter.
Additional file 7: Figure S7.
Western blots used to quantify protein expression for different proteins using T7 vs T7Max promoter. The ladder is BLUEstain Protein Ladder (Goldbio).
Additional file 8: Figure S8.
GFP fluorescence data for expression of proteins in different cell-free extracts, before normalizing T7 value to 100 (as shown on Fig. 7).
Additional file 9: Table S1.
Complete sequences used in the promoter testing experiments. The aptamer transcription templates had no terminators, so all transcriptions were run-off terminated. Promoter sequence is underlined, the aptamer sequence is in italics and protein coding sequence is in bold.
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Deich, C., Cash, B., Sato, W. et al. T7Max transcription system. J Biol Eng 17, 4 (2023). https://doi.org/10.1186/s13036-023-00323-1
- in vitro transcription
- in vitro translation
- synthetic cells
- cell-free protein expression