Effective methods for monitoring eukaryotic gene expression and regulation based on bioluminescence - the emission of light by living organisms - are well established. Typically, the expression of a gene of interest is reported on with high sensitivity and over a wide dynamic range by the emission of light from a variety of engineered luciferase genes from beetles and marine organisms. The luciferase reporter genes are expressed downstream of the target gene or promoter and detected after exogenous addition of luciferin substrates. We describe a novel bioluminescence reporter method for the simultaneous monitoring of two genes expressing engineered firefly luciferase variants that emit readily distinguishable green and red light signals. The key feature is the selectivity of the enzymes for two luciferin substrates that determine each emission color. To validate our method, we performed a complex promoter transactivation experiment side-by-side with the Dual-Luciferase Reporter protocol and obtained essentially identical results. Additional comparative experiments demonstrated that our assay system provided improvements in background, cell normalization, and detectability compared to representative available methods. With access to a luminometer equipped with two optical filters, this method is an excellent choice for genetic reporter assays that can be performed with a single reagent solution.
Effective methods for monitoring gene expression and regulation based on bioluminescence (BL) – the emission of light by living organisms – are well known1,2,3. The expression of a gene of interest is reported on with high sensitivity and over a wide dynamic range by the emission of light from a variety of engineered luciferase (Luc) genes from beetles and marine organisms that are expressed downstream of the target gene after exogenous addition of their respective luciferin substrates. While reporter assays are typically conducted on lysates from cultured human cells, BL detection also enables in vivo cell and animal imaging and biosensor applications as recently reviewed1,2,3. When performing reporter assays, especially when using transiently transfected cells, it is essential to normalize the results because controls are needed to account for cell number, viability, and transfection efficiency4. Normalization has been achieved in dual-reporter assays that monitor control, e.g. cytomegalovirus (CMV) or thymidine kinase (TK) promoters, and test gene activities using two BL signals. Perhaps the most popular format, typified by the Promega Dual-Luciferase® Reporter (DLR®) assay system5, involves two unrelated luciferases that are assayed sequentially without filters using two substrates and a Luc inhibitor. Specifically, the DLR® system uses firefly (Photinus pyralis) and sea pansy (Renilla reniformis) enzymes with their respective substrates firefly luciferin (LH2) plus ATP and coelenterazine. A newer version of the DLR® system called NanoDLR™ 6, uses the NanoLuc and firefly enzymes along with substrates furimazine and 5-fluoroluciferin. The method offers improvements that may provide 2- to 100-fold greater sensitivity6 than DLR®. While several laboratories have conducted studies7,8 with NanoDLR™, we were unable to find comparative data on this new technology. An interesting application of the non homologous enzyme – two substrate sequential format is the use of secreted NanoLuc® 9, and Gaussia enzymes eliminating the need for cell lysis10. Cross reactivity of the enzymes, which share only 22% sequence identity, with the furimazine and coelenterazine substrates, however, limits the ease of performance. This is because in transfection experiments with plasmids under CMV control, a significant signal from NanoLuc®, equivalent to ~25% of the Gaussia response, was observed with the coelenterazine-containing Gaussia assay reagent10. In turn, this necessitated an extensive series of control experiments so that a standard curve could be constructed to determine the contribution of NanoLuc® activity to the signal obtained with the coelenterazine reagent10. The cross-reactivity is ~3-fold higher than expected as estimated from the reported9 ~30-fold greater luminescence of NanoLuc® with furimazine over coelenterazine.
A drawback of using two dissimilar luciferases as is the case with the DLR® systems, especially in the screening of libraries of chemical compounds, is that selective inhibition of the signals may occur leading to misinterpretation of the data11. This problem can be minimized by using a second type of reporter system like the Chroma-Glo™ method12 that employs highly similar (~99%) red- and green-emitting click beetle Lucs CBR and CBG99 with a single substrate (LH2). A similar strategy has been employed with click beetle and railroad worm Lucs (~46% DNA similarity) that use LH2 for dual-color BL imaging13. In the Chroma-Glo™ system, the two signals are produced simultaneously, but with significant spectral overlap that necessitates the use of transmission filters to separate them. It is likely that this assay system has not been widely adopted because of lower signal sensitivity (~10-fold compared to the DLR® method) and requirements for extensive controls needed for cumbersome calculations to determine the intensities of each signal.
We have developed a new dual-color assay format called DART (Dual Analyte Reporter with Two firefly luciferase substrates) that combines several advantages of the current method types, while minimizing the drawbacks of each. BL signals are produced from lysates containing two highly similar (99%) P. pyralis variants upon mixing with a single solution (DSM, dual substrate mix) containing substrates LH2, benzothiophene luciferin (BtLH2)14 (Fig. 1a), ATP, MgSO4, and DTT. A key feature of the two homologous enzyme – two substrate DART method is the selectivity of the Lucs for the substrates that produce very well separated emission spectra.
Results and Discussion
Rationale for construction of pCMV-PLR1 and pCMV-PLG3
Starting with PLG215, a thermostable and pH resistant (to emission color shifting) chimeric Luc that emits with λmax = 559 nm in HEK293T cell lysates, we used random and rational mutagenesis techniques to construct green (PLG3)- and red (PLR1)-emitting Lucs (Supplementary Fig. 1) with enhanced catalytic efficiencies for BtLH2 and LH2 (Table 1 and Fig. 1a), respectively. To construct PLR1, we first introduced two residue changes into PLG2 that we previously found had red-shifted the BL emission, Tyr255Phe16 and Ser284Thr17. Based on the results of several rounds of random mutagenesis, the changes encoding Phe250Thr, Leu291Ile, and Tyr340Phe were introduced into PLG2 to produce a Luc variant gene with a preference for BtLH2. In addition, Val351 was changed to Ile in both PLR1 and PLG3 and Phe465 to Arg for increased thermostability in PLG3.
Bioluminescence properties of PLR1 and PLG3
Using purified proteins, emission maxima of 518 nm and 620 nm were realized with the PLG3-BtLH2 and PLR1-LH2 combinations (Supplementary Table 1 and Supplementary Fig. 2). With DSM, which contains both substrates, lysates of HEK293T cells transfected individually with pCMV-PLG3 or pCMV-PLR1 produced distinct emission profiles with λmax values of 528 nm and 620 nm when assayed alone or mixed together (Fig. 1c,d). The well-separated emission spectra were achieved in large part due to the relative preferences of PLG3 for BtLH2 (1.5-fold) and PLR1 for LH2 (46-fold). With this high degree of signal separation (Fig. 1c), narrow bandpass filters were used to simultaneously measure (Fig. 1b) green and red signals providing very minimal spectral overlap (Fig. 1c).
Detectability of pCMV-PLR1 and pCMV-PLG3 in HEK293T cell lysates
To determine the detectability of PLG3 and PLR1 in the presence of each other, the proteins were expressed individually under the control of the CMV promoter at 37 °C in HEK293T cells. Lysates of equivalent cell count were prepared and mixtures containing both enzymes were assayed with DSM using a microplate luminometer and a single injector. The simultaneously monitored green and red signals could be measured at levels corresponding to 0.2 fmol to 2.0 pmol (Fig. 1b). Under the CMV promoter, the red signal is ~2-fold stronger and contributes only ~0.6% of its intensity to the green luminescence (Fig. 1c). Therefore, optimal results will be obtained using the red signal as the genetic reporter and the green signal as the normalization control.
Comparison of DART and Chroma-Glo™ Methods
We first compared the relative intensities and spectral overlap produced by the enzymes in the DART and Chroma-Glo™ systems with their respective reagents. While both methods offer the advantages of using two very similar genes/Lucs (from beetles) and simultaneous detection of green and red signals, the Chroma-Glo™ system requires only a single LH2 substrate and a reagent that produces optimal BL with the click beetle Lucs. In parallel experiments using identically prepared HEK293T cell lysates containing the DART and Chroma-Glo™ Lucs, the BL of individual Lucs was measured with both methods using a set of green and red filters (Fig. 2). While negligible overlap of the red signals was detected (measured through the green filter) with either method (Fig. 2a,b), ~30% spectral overlap of the green signal was monitored through the red filter with the Chroma-Glo™ method, compared to ≤4% overlap with the DART method (Fig. 2a,b). The high degree of spectral overlap of the Luc signals in the Chroma-Glo™ method necessitates the use of a “calculator” and many time- and reagent-consuming controls in order to extract the red and green signals (Fig. 2b)12. With the DART method, however, the very low overlap of both signals through filters (Fig. 2a) renders it unnecessary to mathematically extract each signal over a wide concentration range of the analytes. This is because the spectral overlap is approximately equal to the standard deviation of the signal intensity measurements when equal amounts of the Lucs are present. In practice, using PLG3 as the normalization control at a conservative 5 times the background, red signals can be measured over 3 orders of magnitude without increasing the green signal above the error of the measurement. By increasing the amount of the control plasmid, the dynamic range would remain approximately the same, but higher levels of red signal could be measured as necessary. We also examined the relative intensities of the BL signals emitted by the Lucs used in each method and determined that the intensities of the red- and green-emitting DART Lucs were 130-fold and 70-fold greater than those of the corresponding click beetle enzymes (Fig. 2c). These results likely reflect inherent lower specific activity and possibly reduced expression of the click beetle Lucs.
Validation of DART method
To validate the DART method, we performed a previously described reporter experiment18,19 that employed the widely used DLR® system. In HeLa18 and Cos-719 cells, the transactivation of the myocyte expression factor-3 promoter (MEF3/TATA) by Six4 (a sine oculis protein) and Eya2 (a human homologue of the eyes absent protein) was evaluated. With DART, the activation of MEF3/TATA in HEK293T cells revealed a 2-fold increase in transcription when the transcriptional activating protein Six4 was expressed. This increased to 3.5-fold with the co-expression of the Eya2 protein (Fig. 3a). These results were essentially identical (t-test) when comparing MEF3/TATA alone (P = 0.97), in the presence of Six4 (P = 0.14), and in the presence of Six4/Eya2 (P = 0.22) with those obtained using the DLR® system. Interestingly, DART provided ~18-fold greater S/N for the MEF3/TATA reporter signal even though the corresponding DLR® measurement was ~45-fold higher (Fig. 3b). The greater S/N of the DART method results from the lower background produced by DSM and the use of transmission filters. In Fig. 3c, we show the raw data obtained by simultaneously monitoring the PLG3 normalization control and PLR1 reporter signals used to produce the DART results presented in Fig. 3a. In contrast, the data (Fig. 3a) obtained using the DLR® system were necessarily acquired in a discontinuous manner.
The novel DART format, which features two substrates and two highly similar firefly Luc enzymes, provides a straightforward and robust method for reporter assays of cell lysates. The impressive signal separation eliminates the need to do extensive controls and calculations to manage poor signal overlap. The low cost is mainly attributable to the use of DSM, a simple single assay solution that does not contain expensive additives. The dynamic range of the method spans at least 3 orders of magnitude with exceptionally low background noise. The S/N advantage of DART was mainly achieved by the reduction of the background signal with narrow bandpass filters. While the filters also attenuated the signals by ~80%, the specific activity of the enzymes was sufficiently high to readily enable measurements at the femtomol level. Additional major features of DART are compared to the established reporter formats typified by the Promega DLR® and Chroma-Glo™ methods (Supplementary note).
The stable glow kinetics characterized by signal half-lives of ~3 h could make our method amenable to high throughput screening2,20 and to performing assays without injectors (Supplementary Fig. 3). The DART method, however, does require the use of filters and the BtLH2 substrate is not yet commercially available, but can be obtained from the authors. We are presently investigating the feasibility of extending the principle of the DART method to in vivo imaging applications.
Materials and Methods
The following materials were obtained from the sources indicated: Mg-ATP (bacterial source) and ATP (disodium salt hydrate) from Sigma-Aldrich (St. Louis, MO); and DLR Assay System, pRL-CMV, expressing Renilla luciferase driven by a CMV promoter, and passive lysis buffer (PLB) from Promega (Madison, WI). Firefly luciferin potassium salt, Chroma-Glo™ reagent, the pF4Ag plasmid (non-commercial expression vector driven by a CMV promoter), pCBG99-Basic and pCBR-Basic vectors, and pGL4.54 (containing luc2 driven by the TK promoter) were generous gifts from Promega (Madison, WI). The pMEF3/TATA-Luc + plasmid, containing six MEF3 sites and a TATA sequence preceding the luc+ gene in the Promega pGL3 Basic vector; the pcDNA3.1-Flag-Eya2 plasmid expressing Eya2; and pcDNA3.1-Six4 expressing Six4 were kind gifts from the Pascal and Casey labs18,21. Benzothiophene luciferin was prepared as previously described14 and is available upon request. DSM was prepared by diluting stock solutions of the reagents to the final concentrations indicated in 50 mM Tricine, pH 7.8: 0.48 mM ATP, 1.8 mM MgSO4, 18 mM DTT, 0.12 mM LH2 and 0.24 mM BtLH2.
Construction of pCMV-PLR1 and pCMV-PLG3
Site-directed mutagenesis to construct pCMV-PLR1 was performed by introducing the Tyr255Phe and Ser284Thr changes and reverting Val351 to Ile (Supplementary Fig. 1) with the QuikChange® Lightning Site-Directed Mutagenesis kit (Agilent, Santa Clara, CA) using human codon optimized PLG2 in the pGEX-6P-2 plasmid15 as the template. The PLR1 cDNA was then sublconed into the pF4Ag plasmid, which contains a CMV promoter. Plasmid pCMV-PLG3 was constructed by screening an in-house library of approximately 75 P. pyralis variants and identifying the Phe250Thr mutation, which produced the optimal combination of ~2-fold improved substrate specificity (kcat/Km) towards BtLH2 and blue-shifted emission spectra (λmax = 517 nm). Two rounds of PCR-based random mutagenesis with the GeneMorph® II EZClone Domain Mutagenesis Kit (initially with the P. pyralis F250T variant in the pGEX-6P-2 plasmid), in which ~4,500 colonies were screened, sequentially identified the Tyr340Phe and Leu291Ile mutations that together improved the BtLH2 selectivity an additional 6-fold with a modest 5 nm red shift in emission. The screening process involved visualization of BL in XL-10 Gold cells initially with LH2 to identify dim colonies. Selected colonies were streaked in duplicate and screened with either BtLH2 or LH2 to identify those that were brighter with BtLH2 than LH2. The three mutations Phe250Thr, Leu291Ile, and Tyr340Phe were then introduced into the human codon optimized PLG2 cDNA in the pGEX-6P-2 plasmid15 followed by reverting Val351 to Ile and changing Phe465 to Arg (Supplementary Fig. 1) to match the thermostability of PLG3 at 37 °C to that of PLR1 (~24 h half-life). The PLG3 cDNA was then subcloned into the pF4Ag plasmid, which contains a CMV promoter. While the latter mutations improved the overall thermostability and narrowed the emission spectrum bandwidth, they were also responsible for reducing the substrate specificity for BtLH2 by ~2-fold. The sequences of luciferase genes in the pGEX-6P-2 and pF4Ag vectors were verified by DNA sequencing at the W. M. Keck Biotechnology Laboratory (Yale University, New Haven, CT). The constructs in the pF4Ag plasmid are referred to as pCMV-PLG3 and pCMV-PLR1 throughout the manuscript. The pCMV-CBG99 and pCMV-CBR constructs were prepared by replacing the PLG3 and PLR1 cDNA sequences with that of CBG99 and CBR, respectively, in the pF4Ag plasmid. Methods for protein expression in the pGEX-6P-2 vector and purification using the Glutathione Sepharose® 4B affinity chromatography were previously reported22.
Steady-State Kinetic Constants
Values of Km and Vmax for LH2 and Bt-LH2 with purified PLR1 and PLG3 were determined from BL activity assays in which measurements of maximal light intensities (bursts) were taken as estimates of initial velocities. The equipment used to make these measurements has been previously described23. Data were collected from 0.525 ml reactions in 50 mM Tricine buffer, pH 7.8, containing 0.6 μg of Luc enzyme in 20 mM Tris-HCl (pH 7.8) containing 150 mM NaCl, 1 mM EDTA, 1 mM DTT, 0.8 M ammonium sulfate and 2% glycerol. The concentrations of LH2 and Bt-LH2 were varied (1 μM–0.5 mM). Reactions were initiated by injection of Mg-ATP (2 mM final concentration). Kinetic constants (Table 1) were determined using the nonlinear least squares method of the Enzyme Kinetics Pro software (SynTex), which fits data from the Michaelis–Menten equation to a rectangular hyperbola; kcat was determined from initial velocities taken as peak light emission 1 min after the initiation of bioluminescence.
Transfection of HEK293T cells and preparation of lysates
In all experiments described below, HEK293T cells were plated in 24 well plates at a density of 150,000 cells/well in Dulbecco’s Modified Eagle’s Medium (Corning) +10% fetal bovine serum and grown overnight. The cells were transfected in triplicate with varying amounts of each plasmid (transfection mix included 500 ng total DNA including empty vector and 1.5 µL Lipofectamine 2000 in 0.1 mL OptiMEM) and grown overnight at 37 °C with CO2. The next day growth media were removed; the cells were washed with PBS, and lysed in 0.1 mL PLB.
Bioluminescence emission of PLR1 and PLG3 in HEK293T cell lysates
Lysates (5 μL) from HEK293T cells transfected with pCMV-PLR1 or pCMV-PLG3 were added individually or mixed together into cuvettes containing 0.5 mL of DSM with gentle mixing. After 1 min, BL spectra were recorded (Fig. 1c,d) with a Horiba Jobin-Yvon iHR imaging spectrometer equipped with a liquid N2 cooled CCD detector. Data were collected at 22 °C over the wavelength range 450 nm–750 nm with the emission slit width set to 5 nm and were corrected for the spectral response of the CCD using a correction curve provided by the manufacturer.
Detectability of PLR1 and PLG3 in HEK293T cell lysates
Stock solutions of lysates from HEK293T cells transfected with pCMV-PLR1 or pCMV-PLG3 (prepared as described above) were diluted 10-fold in PBS containing 1 mg/ml BSA. Serial 10-fold dilutions of the pCMV-PLR1 and pCMV-PLG3 lysates were made and 5 µL of each dilution of pCMV-PLR1 was mixed with 5 µL of the same dilution of pCMV-PLG3 in the wells of a white 96-well plate. Bioluminescence was initiated by automatic injection of 0.1 mL of DSM. After a 1 min delay, emission signals were recorded on a Synergy™ 2 microplate luminometer (BioTek, Winooski, VT) using 516 ± 10 nm (green) and 635 ± 16 nm (red) filters (BioTek). The instrument records the mean intensity of the flat signals over 10 s by alternately taking readings for 0.02 s with the green and red filters. Data shown in Fig. 1b were expressed in moles of each Luc and were obtained from a standard curve constructed using known amounts of purified proteins.
Comparison of the DART and Chroma-Glo™ Luciferase assay systems
Equal numbers of HEK293T cells were transfected with the following plasmids: pCMV-PLR1, pCMV-PLG3, pCMV-CBR, or pCMV-CBG99, and cell lysates were prepared as described above. In triplicate experiments, lysates from each plasmid were diluted 10-fold in PBS and 5 µL of each dilution were added to the wells of a white 96-well plates. For pCMV-PLR1 and pCMV-PLG3, DART assays were performed as described below. The BL of pCMV-CBR and pCMV-CBG99 were assayed according to the manufacturer’s protocol12 using the Chroma-Glo™ reagent except that cells were lysed with PLB and the Biotek filters were used.
The DART assay
To perform the DART assay, HEK293T cells were plated in 24 well plates at a density of 150,000 cells/well in Dulbecco’s Modified Eagle’s Medium (Corning) +10% fetal bovine serum. The next day cells were co-transfected in duplicate with plasmids expressing PLR1 (reporter) under control of the promoter of interest and PLG3 (normalization control) under control of a CMV or TK promoter. The transfection mix included 500 ng total DNA (optimized amounts of each plasmid and empty vector) and 1.5 µL Lipofectamine 2000 in 0.1 mL OptiMEM. Cells were grown overnight at 37 °C with 5% CO2. The next day, growth media were removed; the cells were washed with PBS, and lysed in 0.1 mL. Aliquots of lysates (5–20 µL) were added to duplicate wells of white 96-well plates. Bioluminescence was initiated by automatic injection of 0.1 ml of DSM that was either prepared fresh or thawed at room temperature after storage at −80 °C. After a 1 min delay, emission signals were recorded on a Synergy™ 2 microplate luminometer (BioTek, Winooski, VT) using 516 ± 10 nm (green) and 635 ± 16 nm (red) filters (BioTek). The instrument records the mean intensity of the flat signals over 10 s by alternately taking readings for 0.02 s with the green and red filters. To normalize the reporter signal, the mean signal over 10 s with the red filter (PLR1) was divided by the mean signal over 10 s with the green filter (PLG3).
Validation of the DART method
To validate the DART method, we performed a previously described reporter experiment18,19 that employed the widely used DLR® system. In HeLa18 and Cos-719 cells, the transactivation of the MEF3/TATA promoter by Six4 and Eya2 was evaluated (Fig. 3). A set of reporter plasmids pMEF3/TATA-PLR1 and pMEF3/TATA-Luc+ was made by replacing the luc+ gene of the available18,21 MEF3/TATA-Luc+ vector with the cDNA of PLR1 using the NcoI and XbaI restriction sites. The internal controls were pCMV-PLG3 and the Renilla Luc (pRL-CMV plasmid) under the control of the CMV promoter. HEK293T cells were transfected in duplicate (as described above) with pMEF3/TATA-PLR1 (60 ng) and pCMV-PLG3 (0.5 ng) or pMEF3/TATA-Luc+ (60 ng) and pRL-CMV (10 ng). Additionally, each reporter-control pair was transfected with pcDNA3.1-Six4 (60 ng) with and without the inclusion of pcDNA3.1-Flag-Eya2 plasmid (120 ng). Twenty-four hours after transfection, the cells were washed with PBS and lysed in 0.1 mL PLB. The DART assay was performed as described above and the DLR assay was performed according to the manufacturer’s protocol5; 20 µL of lysate per well was used for all assays.
Student’s t tests were used to assess the level of significance between methods using the Data Analysis ToolPak in Microsoft Excel.
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This work was supported by the National Science Foundation (B.R.B., MCB-1410390), the Hans & Ella McCollum 21 Vahlteich Endowment (B.R.B.), the Air Force Office of Scientific Research (B.R.B., FA9550-18-1-0017), and the National Institutes of Health (M.J.G., R15CA125731-02).
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