Time-Gated Surface-Enhanced Raman spectroscopy (TG-SERS) was utilized to assess recombinant protein production in Escherichia coli. TG-SERS suppressed the fluorescence signal from the biomolecules in the bacteria and the culture media. Characteristic protein signatures at different time points of the cell cultivation were observed and compared to conventional continuous wave (CW)-Raman with SERS. TG-SERS can distinguish discrete features of proteins such as the secondary structures and is therefore indicative of folding or unfolding of the protein. A novel method utilizing nanofibrillar cellulose as a stabilizing agent for nanoparticles and bacterial cells was used for the first time in order to boost the Raman signal, while simultaneously suppressing background signals. We evaluated the expression of hCNTF, hHspA1, and hHsp27 in complex media using the batch fermentation mode. HCNTF was also cultivated using EnBase in a fed-batch like mode. HspA1 expressed poorly due to aggregation problems within the cell, while hCNTF expressed in batch mode was correctly folded and protein instabilities were identified in the EnBase cultivation. Time-gated Raman spectroscopy showed to be a powerful tool to evaluate protein production and correct folding within living E. coli cells during the cultivation.
Escherichia coli is a widely used host organism for the production of recombinant proteins, for example for industrial enzymes1 or pharmaceuticals2,3. One major limitation when overexpressing heterologous proteins is aggregation or misfolding within the cells which may result in physiological stress to the host organism1,4. This stress, activated by the σ32-promotor5,6, results in the formation of chaperone proteins and proteases5,6,7. The σ32-promotor also is activated during the exponential growth phase of E. coli and is switched off during the stationary growth phase. Since the σ32 protein is unstable and degraded within 4 minutes within the cell, cellular responses are rapid6.
For heterologous protein production there is an optimal time-window. The correlation between the growth rate, μ, and the specific protein production rate, qp, for induced batch and fed-batch cultures8 indicate that a slow growth rate under induced conditions gives little to no product. In addition, there is a limited duration of expression and qp, in batch cultures7. Several methods probe physiological stress indirectly, either by evaluating bioprocess parameters7, or by use of reporter genes under the σ32-promotor9. These give some insight about the protein aggregation in the cell, and thus ultimately the protein quality10. Other techniques aim to measure the amount of protein produced directly from the biomass via a reporter protein11 or after sampling12. However, there are limited reports on the direct evaluation of the desired product during production in the host cells without removing cells from the culture.
Raman spectroscopy is a promising technique to observe proteins and their secondary structure in a real-time and label free setting without the need for invasive sample handling13. It allows to collect accurate qualitative data in the form of a spectrum (fingerprint) of the sample and quantitative data as the intensity of the compounds (vibrations of molecules) in the sample with the use of specific Raman-probes14. The quantitative signal should be considered with caution, since any change of the setup, such as focal distance to the sample, stability of the excitation laser source, the detector, as well as the acquisition time have significant influence to the intensity of the Raman peak height and the signal-to-noise ratio. A major advantage of Raman spectroscopy compared to other varieties of spectroscopy, e.g. infrared spectroscopy is that there is very little interference from the vibration of water molecules. This makes Raman spectroscopy an ideal tool for studying liquid samples. However, auto-fluorescence initiated from various biomolecules very often superimposes with the relatively weak Raman signals. There are several methods to suppress interfering fluorescence15, and one promising approach is to use time-gated Raman spectroscopy. Surface-Enhanced Raman spectroscopy (SERS) is an approach focusing on the strong enhancement of the Raman signal, which further can minimize the influence of auto-fluorescence16. Although Raman setups in the ultraviolet (UV) and infrared (IR) spectral range show less interference of sample-induced auto-fluorescence, the Raman intensity is proportional to the fourth power of the laser excitation frequency and therefore a measurement in UV and IR range may result in less intense Raman emissions and eventual sample degradation15. However, excellent protein spectra can be obtained via a thoughtful protocol17,18, mainly in low fluorescent matrices.
This contribution used commercially available time-gated Raman spectroscopy19, and compared this technology with continuous wave (CW) Raman spectroscopy in order to assess its ability to reduce the high fluorescence signals from complex media and E. coli cells. We also compared SERS versus non-enhanced evaluation of the Raman spectra. Finally, we evaluated induced and non-induced E. coli batch and fed-batch like cultures at different stages of their growth curve.
Materials and Methods
2x bacto Yeast extract, bacto Tryptone, Phosphate (Thermo Fisher, USA), Glucose (YTPG) medium20, Luria-Bertani broth (LB medium);21 Growdex nanofibrillar cellulose (NC) was purchased from UPM Biochemicals Oyj (Helsinki, Finland). Disodium hydrogen phosphate was obtained from Fisher Scientific (Hampton, USA), potassium dihydrogen phosphate, calcium chloride, 2-(N-morpholino)ethanesulfonic acid (MES), sodium chloride, glucose, Ethylene diaminetetraacetic acid (EDTA), sodium azide, silver nanoparticles (Ag NPs) − 40 nm particle size (Ag NP; #730807) were obtained from Merck Sigma-Aldrich (Darmstadt, Germany), and potassium chloride was obtained from Honeywell Riedel de Haën (Seelz, Germany). Ultra-pure water, phosphate buffer (buffer A) and MES buffer (buffer B) were prepared as before22.
The pRSETA-HspA1 plasmid was synthesized and codon optimized for E. coli (ThermoFisher, USA). The pOPIN-(6HIS)-hCNTF plasmid was synthesized as previously described3. The pET3a-Hsp27 plasmid was a kind gift of Prof. W. Boelens. The complete DNA sequences of all genes were verified by gene sequencing (GATC, DE) prior to use. E. coli NEB5-alpha competent cells (New England Biolabs, USA; chemically competent cells #C2987I) were transformed and used for plasmid propagation21. The pRSETA-HspA1 and pET3a-Hsp27 were then transformed separately to E. coli strains BL21(DE3) pLYsS and the pOPIN-(6HIS)-hCNTF plasmid to E. coli strain Rosetta 2 (DE3) pLysS (Novagen, Merck KGaA, Darmstadt, Germany) for protein production.
Cellular protein expression and protein purification
Expression of HSPA1 and Hsp27 were carried out in BL21(DE3) E. coli cells, and hCNTF in Rosetta-2 (DE3) E. coli cells. First the transformants were grown overnight (o/n) in LB medium with 100 μg/ml ampicillin and 1% (w/v) glucose at 30 °C from previously prepared glycerol stocks according to Sambrook and Russel (2001)21. In the case of hCNTF in Rosetta-2 E. coli cell, 34 μg/ml chloramphenicol (ICN, USA) was added as well. Fifty ml of 2xYPTG medium was inoculated at an OD600 of 0.15 at 37 °C from the LB pre-cultures. In addition 2 ml of the hCNTF Rosetta-2 E. coli o/n culture was used to inoculate 50 ml of EnPressoB medium (EnBase system)23 with 100 µg/ml ampicillin and 34 μg/ml chloramphenicol at 30 °C. All cultures were cultivated at 225 rpm (1” amplitude shaker) in high yield flasks24 with AirOtop seals (Thomson Instrument Company, CA, USA) to maximize oxygen transfer. Cells in 2xYPTG were induced at OD600 = 0.4−0.5 (see Table 1) with 0.4 mM IPTG final concentration and grown for 4 hours (hCNTF) or 6 hours (HspA1) after induction. Cells in the EnBase cultures were induced with 0.4 mM IPTG after 24 h and grown for another 24 hours as instructed by the manufacturer. As reference cultures, non-transformed BL21(DE3) E. coli cells were cultivated under the same conditions in 2xYPTG and the EnBase system. EnPressoB medium used in the EnBase cultivations was also incubated under the same conditions as the cultivations for the cell dry weight (CDW) measurements to determine the biomass of the EnBase cultures. All samples are summarized in Table 1 and were kept on ice until measured or further processed.
Raman spectroscopy was performed with both, continuous wave (CW)-Raman and pulsed laser time-gated (TG)- Raman. The TG-Raman instrument (Timegate Instruments Ltd.) was a commercial system to set the benchmark for auto-fluorescence suppression. Both instruments had a laser excitation wavelength of λexc = 532 nm which is in the fluorescence and Raman maximum response. The commercial CW excitation Raman spectrometer was equipped with a confocal microscope (Nikon Corporation, Tokyo, Japan) with a numerical aperture of 0.22, type alpha 300 RA (WiTec, Ulm, Germany). This was used as the reference for the TG Raman measurements with magnification of 20 × lens and neutral density (ND) filters and laser power of approximately 20 mW (Ophir Nova II laser power meter, Ophir Optronics Solutions Inc., Jerusalem, Israel) at the sample to avoid photo-bleaching. The commercial CW-Raman system was comprised of a conventional thermo-electrically temperature-stabilized charge-coupled device (CCD) detector with optional electron multiplying EM-option (EMCCD) Newton DU970-BV (Andor Technology Ltd, Belfast, Northern Ireland) at operational temperature of −60 °C during the measurements. The spectrometer had a resolution of 4 cm−1 full-width-at-half-maximum (FWHM). The TG- Raman instrument was comprised of a non-cooled CMOS SPAD-detector with a 100 ps pulsed Nd:YVO4 green laser and adjusted laser power of 20 mW (confirmed with above mentioned laser power meter) at the sample in combination with ND-filters. The system was attached via an adapter to a confocal microscope (Olympus Corporation, Tokyo, Japan) with a magnifying lens of 20 × (NA = 0.4). The TG-Raman spectrometer with a spectral resolution of 10 cm−1 (FWHM) had a limited spectral range of 500–1700 cm−1. The system was set to cover the temporal decay time of t = 0.5–5.5 ns to measure the Raman and fluorescence signal while being able to separate both signals from each other. A detailed description of the time-gating principle used in the Timegate Instruments Ltd. device can be found elsewhere15,25,26.
Measurement procedure and spectral data processing
The commercial Ag NPs stock solution was centrifuged (Eppendorf 5804 R, rotor FA–45–6–30) at 4500 rpm for 4 min., followed by the removal of the supernatant which reached a final concentration of around 0.06 g L−1. The experimental Raman setups including the assay (bottom-up) of NC, Ag NPs, and sample is depicted in Fig. 1. Preceding the actual Raman/SERS measurements, each well of an in-house made anodized aluminum microwell plate (Fig. S1) with a total volume of 90 µL/well (Fig. 1) was filled with 25 µL NC. Layered on top was 25 µL Ag NPs before 25 µL of the sample (Table 1) was added, with a total volume of 75 µl. Each sample was prepared fresh for each microwell (i.e. the layering of NC, Ag NPs and cells) with the same settings prior to each Raman/SERS measurement, both in CW and time-gated settings. The final concentration of the cells was approximately 4 * 108 cells/ml (hCNTF 2, 4, and 24 hours, and HspA1 6 hours after induction). The final concentration for hCNTF and HspA1 1 hour after induction was approximately 2.4 * 108 cells/ml, considering the volume of NC and Ag NP solutions. The aluminum has proven to not interfere with the measurements27,28. In addition, due to the relatively low intensity of background from complex media from the E. coli cell samples with NC and Ag NPs this contribution was not subtracted from final spectra (Fig. S6).
Spectral data processing was performed with OriginPro (V. 2016b and 2018b, OriginLab, Northampton, MA, USA). The data was normalized in an intensity interval between 0 and 1 and plotted with an offset for better presentation, except for Figs. 4 and 6 (bottom row) where Raman intensities from two TG-Raman measurements were compared with each other. Prior detailed spectral analysis and comparison, all TG-Raman data was pre-processed with the TG-Raman instrument spectral processing tool (Timegate Instruments Oy, Oulu, Finland). Prior to the measurements, both Raman spectrometers were wavelength calibrated and the excitation lasers sources operated normally.
Heterologous protein production performed in shake flasks, in batch mode using E. coli expression strains, were monitored for their cell-growth by sampling every hour and measuring the optical density with a spectrophotometer at λabs = 600 nm (OD600). Absorbance levels of OD600 > 0.5 were diluted to avoid a bias in the measurements (Table 1).
The impact of heterologous protein production after induction on the growth of E. coli is clearly observable (Figs. 2 and 3). E. coli cells that did not contain an expression plasmid obtained a much higher final cell-density than induced cultures. Rosetta-2 cells expressing hCNTF grew slower and were induced later than the other samples, hence the relative shorter expression time of 4 hours versus 6 hours in BL21(DE3) cells.
EnBase system cultures mimicked a fed-batch cultivation23 and therefore reached a much higher optical density. They were induced at OD600 = 11.7 after 24 hours of growth and harvested at OD600 = 43.8 (Table 1). As can be seen in Fig. 3, Hsp27 and hCNTF proteins were produced, while the levels of HspA1 were barely visible on the SDS-PAGE gel after Coomassie staining. From previous experience we know that most of the HspA1 protein ends up in inclusion bodies (IB) due to misfolding under these conditions (data not shown). Human heat shock proteins are known for their instability during heterologous expression in E. coli fermentations29,30. Unexpectedly, hCNTF expressed with the EnBase system showed 2 bands after induction, while hCNTF produced under similar conditions as before3 showed one product. Since we had stored previous batches of hCNTF in conditions where protein was denaturing, i.e. before we optimized the storage buffer22, we chose HspA1 and both hCNTF samples for further evaluation with Time-Gated Raman spectroscopy as representative samples of 3 types of fermentations: (a) poorly expressed protein (HspA1), well expressed protein (hCNTF batch mode), and a degrading protein (hCNTF in fed-batch like mode). CW-Raman spectra of Hsp27 can be found in the supplementary data (Figure S3).
Time-Gated Raman Spectroscopy in liquid samples
The purpose of our experimental set-up was to measure directly from expression culture, without removal of the expression media or drying the samples. Therefore, we used a relatively large volume of 75 µl with a measured laser power of 20 mW to assure minimal heating of the sample. The fluorescence of the samples is a major problem when measuring at λexc = 532 nm as can be seen in Fig. 4. Figure 4A shows the comparison between Continuous Wave (CW)-SERS (red curve) and TG-SERS (green curve) measurements of hCNTF 1 hour after induction under the same experimental set-up as depicted in Fig. 1. For clarity, the intensities have been standardized in an interval between 0 and 1 and off-set separated. These results clearly demonstrates the ability of the TG-Raman technique to suppress interfering fluorescence. Even when Ag NPs are added to CW-Raman measurements, the signals are barely distinguishable from the background signals (Figs. 4 and S3). When looking at the overall spectral range (200–3000 cm−1) of the CW-SERS measurements (Figure S2) the level of fluorescence appears as a broad bump. However, some weak spectral peaks are faintly visible (724, 850–860, 950–960, 1330 as well as 1450 cm−1) which correspond to the more clearly identifiable TG-Raman spectra. Figure 4B represents a measurement of enhanced Green Fluorescent Protein (eGFP) sample with CW-Raman (red) and TG-Raman (green) with even stronger fluorescence background in the conventional CW-Raman setup. Furthermore, even though the CW-Raman system has an excellent detector, it saturated very rapidly, i.e. under 10 seconds acquisition time, and no obvious Raman-protein spectrum was observed. In comparison, the TG-Raman spectrometer at even at over 1 million photon-counts obtained a typical Raman protein spectrum (Fig. 4) in line with peaks at intensities described before (Table 2).
To ensure that the time-gated laser would sample enough E. coli cells in the measuring area under the objective and avoid cell movements due to convection currents, we made use of nanofibrillar cellulose (NC) to immobilize the cells (Fig. 1). NC has been shown to be an excellent inert matrix for cells31, however since cellulose has a rather strong Raman spectrum overlapping with protein peaks, we used Ag NPs to suppress the Raman signals from the underlying matrix (Fig. 5). As can clearly be seen, even at relative low concentrations of 0.06 g L–1of AgNPs, most of the cellulose spectra were suppressed, while citric acid present in the Ag NPs solution as preservative is not observed in the final NC, Ag NPs, and cell samples (Figure S5).
Evaluation of protein production in E. coli cells with Raman Spectroscopy
Living E. coli cells were evaluated with CW-Raman spectroscopy and TG-Raman spectroscopy with and without SERS enhancement. The results for HspA1 and two different hCNTF cultivations are summarized in Fig. 6. Due to the strong background fluorescence, not much can be seen in the CW-Raman/SERS spectra (Figs. 4A, 6, S2 and S3). Hence, in order to evaluate the protein quality within the cells normalized TG-Raman spectra were compared (Fig. 6A–C). In addition, the changes of the real intensities of the spectra (Fig. 6D–F) for the same amount of cells indicate the protein production rate and identify additional quality parameters. All cultivation data shown in Fig. 6 have been scaled within the same spectral range in order to simplify comparison between the different spectra.
In general, three strong spectral peaks were very distinctive in HspA1 and the hCNTF cultivations, namely around 1000, 1400 and 1650 cm−1, but their intensities depended on the stage of the cultivation. In particular it appears that the phenylalanine peak around 1000 cm−1 is broad and seems to be a convolution of another peak at around 1050 cm−1 (cp. Table 2). In addition, the peaks around 1400 cm−1 in all cultivations at different time points showed a double or triple peak. This might indicate either a symmetric deformation of CH3 or an overtone of Amide V was present. It also appears it was the strongest and widest peak increasing as a function of time. Even though, the increase of the peaks around 1400 cm−1 are clearly due to increase of protein per cell (Fig. 6E,F), quality parameters are harder to identify, since these peaks in the normalized spectra of Fig. 6A–C may also be present in the cultivation media (Figure S6).
Small differences can be identified at the different time points, i.e. HspA1 (first row) after 1 h of induction shows an elevated background with DNA signatures at 710 and 742 cm−1 that is not present in later stages of the cultivation. During the exponential growth phase approximately 3% of the cell dry weight consists of DNA32, however growth rates tend to be lower under induced conditions8 and DNA amounts per cell are lower at lower growth rates33. The peaks around 850 cm−1 are weak which may indicate that NC as “soft bed” for the assay (Fig. 5) does not interfere while observing the protein Raman spectra. We speculate that the peak can be attributed to tyrosine, due to the shift of the maximum intensity from 846 cm−1 to 862 cm−1 in the HspA1 cultivation (Fig. 6A), which indicates changes in local interactions within the protein. We do not observe this effect in the hCNTF cultivation, thus we attribute this shift due to protein aggregation or the formation of IBs.
Larger differences can be observed when comparing the intensity values (Fig. 6D–F). The differences of the HspA1 and hCNTF batch cultivations after 1 hour of induction region are rather small, but shift clearly in the later time points. The spectral data reflect the amount of protein produced per cell, which is evident when comparing expression levels in the SDS-PAGE gel (Fig. 3). The total amount of protein in a non-induced culture compared to an induced culture after 24 hours of protein expression in the EnBase system hCNTF (EN hCNTF; Fig. 6F) is higher than in the batch phase protein expression of hCNTF depicted in Fig. 6B,E. The amide III peaks at 1242 cm−1 and around 1300 cm−1 are clearly seen as shoulders of the main peak around 1400 cm−1 of cells under induced conditions. The pronounced amide I peak is increasing as well during the hCNTF cultivations. Clearly visible is the difference between HspA1 and hCNTF cultivations. HspA1 shows peaks at 1520–1680 cm−1 with traces of Amide II and aromatic structures at 1550 and 1605 cm−1, while the shoulder at ~1590 cm−1 of the α-helical hCNTF is indicative of aromatic modes34.
Overall, the time-gated Raman spectra showed similar spectra compared to cell or protein spectra provided by the references listed in Table 2.
Biotechnology and synthetic biology are considered of increasing importance to provide solutions for the sustainable production of food, medicine, vaccines, industrial enzymes, chemicals, and components for materials such as bioplastics. The EU lists industrial biotechnology as one of the key enabling technologies (KET) for our future. In comparison to other technologies, biotechnological production is still complex and undefined, and product quality is not easy to control. Therefore, new accurate methods are needed to better understand the manufacturing of products. As an analogy, the industrial revolution was driven by mass production of standardized parts. In a similar way to truly transform the biotechnology industry for precision manufacturing, the lack of tools to directly monitor the intermediate products during manufacturing within the living cells must be addressed.
In this study, we showed for the first time the use of TG-SERS for the direct evaluation of recombinant protein production within living bacterial cells and compared this with CW-SERS. The use of TG-SERS significantly reduced the interference of the background fluorescence. We utilized a novel method to stabilize our cultivation media samples for the measurements on top of NC. Furthermore, we utilized the effect of the Raman enhancement with SERS to provide a more stable measurement surrounding in order to compare measurements from different time points in the cultivations. We could clearly identify differences in the cultures without the need to dry the samples or break the cells.
HspA1 consists of two domains: (a) the substrate binding domain, which consists mainly of β-sheets and one alpha-helix35 and (b) the ATP binding domain, which consists of both α-helices and β-sheets36. When comparing the HspA1 spectra with the spectra of the helical protein hCNTF (Fig. 6), besides the difference of the amide I peaks34, the valine peak at 926 cm−1 is prominent; HspA1 contains 7% of valine. One other prominent feature of human HSPA1 Raman spectra is the shoulder of the broad 1014 cm−1 peak at 1050 cm−1, which could be assigned to lipids. However, it was shown by Höhl et al. (2019) that a distinct peak at 1100 cm−1 after data post-processing could be contributed to pure HSPA1 and not to Hsp90 under the same conditions37. Therefore, we speculate that the shoulder at 1050 cm−1 could be due to the δC-H plane bending of aromatic side chains, such as phenylalanine, tryptophan and/or tyrosine (Table 2).
The preparation of soluble and active HspA1 is often limited by misfolding during expression, which in E. coli can lead to the formation of IBs29,38. The misfolding of HspA1 is evident when observing the shift of the amide I peak from 1680 to 1650 cm−1 between 1 to 4 hours of expression. This shift is due to the formation of amyloid structures and additional β-sheets, and is linked to protein aggregation39,40.
Another issue of HSPA1 expression in BL21(DE3) strains is the interaction of HSPA1 with native E. coli GAPDH, which may result in a slower growth41. Briand et al. described the leakage of the hHSPA1 gene and the interaction with GAPDH, which resulted in the auto-induction of hHSP70 production due to the inactivation of the LacI gene in pET plasmids. However, the expression plasmid pRSETA we utilized in our study did not contain the LacI gene. The limited expression rate of HspA1 in our experiments is evident when comparing the SDS-PAGE gel (Fig. 3, lanes 3–4) with the relative small increase of the phenylalanine peak (1014–1050 cm−1) in Fig. 6D after four and six hours induction. Low growth rates are known to have an effect on protein production rates in E. coli8.
Human CNTF is a small, fully α-helical protein42,43. Throughout the expression, the amide I peak at 1650 cm−1 clearly has the characteristic shape originating from an α-helical structure with its maximum at 1650 cm−1 (Table 2) and the aromatic modes or amide II peak at 1598 cm−134. During the expression, the phenylalanine peak shifts to a lower wavenumber of 1014–1022 cm−1, presumably due to folding of the protein. This behavior was not observed in the HspA1 cultivation. The most abundant amino acid in hCNTF is leucine (13%), which may be a reason why the maximum of the broad peak at ~1400, mainly due to the culture media (Figure S6), is shifted slightly to a lower wavelength, since leucine does show a peak at a maximum of 1395 cm−144.
In order to explain the differences in hCNTF spectra between the batch cultivation and the EnBase fed-batch like cultivation (Fig. 6B,C,E,F) we further evaluated the difference between a new and an old batch of hCNTF cultivation with TG-SERS. These samples were purified and stored in buffer3 or directly measured after purification by using an optimized buffer for improved stability22. Figure 7 shows the results within a spectral range of 900–1500 cm−1. Differences at 960, 976, around 1000 and 1080, 1128, 1190, 1315, 1332 cm−1 are noticeable also after repeated measurements. However, shape and structure of the spectra remains practically the same.
We compared the expression of hCNTF in the SDS-PAGE gel (Fig. 3; lanes 6 and 8) with the spectra observed in Figs. 6 and 7, and it is evident that hCNTF cultivated with the EnBase system shows signs of degradation at the end of the cultivation. The additional strong band at ~ 23 kDa in Fig. 7 (lane 8) is weak in the batch cultivation (lane 6) indicating protein degradation. In the Raman spectra obtained during the cultivations (Fig. 6), we observed the following differences in the EnBase cultivation compared to the hCNTF batch cultivation: (1) a minor phenylalanine peak at 662 cm−1, (2) a shift of the tyrosine peak to 816 cm−1, (3) a distinct valine peak at 918 cm−1, (4) minor peaks at 1130 and 1195 cm−1, and (5) indication of β-sheet formation due to the rise of a peak at 1332 cm−1. Thus, the changes in the protein environment are seen via the aromatic amino acids. In addition, degraded/aggregated hCNTF in buffer compared to newly prepared hCNTF shows two small, but distinct peaks at ~1130 and ~1195 cm−1. These peaks are indicative of protein degradation during protein expression in the EnBase system. Taken together, we found several indications of protein degradation of hCNTF in the time-gated-Raman spectra during the EnBase system cultivation.
Time-gated Raman spectroscopy showed to be an advantageous spectroscopic tool to evaluate protein expression conditions during E. coli fermentations. Despite the longer sampling time compared to CW-Raman spectroscopy, the suppression of highly fluorescent signal is crucial to obtain meaningful Raman signals when measuring directly from living E. coli cells within complex cultivation media. Time-gated Raman spectroscopy can identify the increase of protein levels in the cell after induction and specific peaks indicative of protein quality, e.g. protein aggregation or degradation. More specifically, we showed with Raman spectroscopy measurements that protein production levels were low and that the protein was aggregating during the cultivation of HspA1. Regarding the cultivation of hCNFT we identified specific quality parameters indicative of correct protein folding. Therefore, time-gated Raman spectroscopy is a powerful tool to directly monitor the intermediate production steps during manufacturing with living cells needed for future precision manufacturing of proteins.
Availability of data and materials
The datasets supporting the conclusions of this article are included within the article and the supplementary data file.
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We thank Dr. Wilbert Boelens of Raboud University (Nijmegen, the Netherlands) for providing us with the pET3a-Hsp27 plasmid containing the human Hsp27 gene. We also would like to thank Dr. Afsahi Ghazaleh (Aalto University, Finland) and Leena Pietilä (University of Helsinki, Finland) for their kind laboratory assistance and Regina Casteleijn-Osorno of AaltoEE (Finland) for comments that greatly improved the manuscript. Furthermore, we thank the Academy of Finland with FOULSENS-project (292253), the “Disrupting biotechnology to achieve high quality synthesis for biological drug development” Key-project (303884), and the VTT technical research centre of Finland for financial support. This work was funded and supported by Academy of Finland project 303884, 292253 and the VTT Technical Research Institute Finland.
The authors declare no competing interests.
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Kögler, M., Itkonen, J., Viitala, T. et al. Assessment of recombinant protein production in E. coli with Time-Gated Surface Enhanced Raman Spectroscopy (TG-SERS). Sci Rep 10, 2472 (2020). https://doi.org/10.1038/s41598-020-59091-3