- Open Access
Construction and comprehensive characterization of an EcLDCc-CatIB set—varying linkers and aggregation inducing tags
Microbial Cell Factories volume 20, Article number: 49 (2021)
In recent years, the production of inclusion bodies that retained substantial catalytic activity was demonstrated. These catalytically active inclusion bodies (CatIBs) were formed by genetic fusion of an aggregation inducing tag to a gene of interest via short linker polypeptides and overproduction of the resulting gene fusion in Escherichia coli. The resulting CatIBs are known for their high stability, easy and cost efficient production, and recyclability and thus provide an interesting alternative to conventionally immobilized enzymes.
Here, we present the construction and characterization of a CatIB set of the lysine decarboxylase from Escherichia coli (EcLDCc), constructed via Golden Gate Assembly. A total of ten EcLDCc variants consisting of combinations of two linker and five aggregation inducing tag sequences were generated. A flexible Serine/Glycine (SG)- as well as a rigid Proline/Threonine (PT)-Linker were tested in combination with the artificial peptides (18AWT, L6KD and GFIL8) or the coiled-coil domains (TDoT and 3HAMP) as aggregation inducing tags. The linkers were fused to the C-terminus of the EcLDCc to form a linkage between the enzyme and the aggregation inducing tags. Comprehensive morphology and enzymatic activity analyses were performed for the ten EcLDCc-CatIB variants and a wild type EcLDCc control to identify the CatIB variant with the highest activity for the decarboxylation of l-lysine to 1,5-diaminopentane. Interestingly, all of the CatIB variants possessed at least some activity, whilst most of the combinations with the rigid PT-Linker showed the highest conversion rates. EcLDCc-PT-L6KD was identified as the best of all variants allowing a volumetric productivity of 457 g L− 1 d− 1 and a specific volumetric productivity of 256 g L− 1 d− 1 gCatIB−1. Noteworthy, wild type EcLDCc, without specific aggregation inducing tags, also partially formed CatIBs, which, however showed lower activity compared to most of the newly constructed CatIB variants (volumetric productivity: 219 g L− 1 d− 1, specific volumetric activity: 106 g L− 1 d− 1 gCatIB− 1). Furthermore, we demonstrate that microscopic analysis can serve as a tool to find CatIB producing strains and thus allow for prescreening at an early stage to save time and resources.
Our results clearly show that the choice of linker and aggregation inducing tag has a strong influence on the morphology and the enzymatic activity of the CatIBs. Strikingly, the linker had the most pronounced influence on these characteristics.
Enzymes produced by microbial systems becoming increasingly important, e.g., for the sustainable production of platform chemicals and bio-based polymers [1,2,3,4]. Due to their advantages, like heat resistance, tensile strength and electrical insulation, polyamides are interesting for diverse applications in the electrical, automotive and textile industry as well as for consumer articles and in the medical sector . One successful example of a biotechnologically produced precursor for a bio-based polyamide is 1,5-diaminopentane (DAP). Together with dicarbonic acids like sebacic acid, this C5 diamine building block is used to build up polyamides (PA). The resulting PA 5.10 (5: 1,5-diaminopentane (C5); 10: sebacic acid (C10)) shows comparable or even better material properties compared to the widely used petroleum-based polyamide PA 6 (6: caprolactam (C6)) . DAP can be biotechnologically produced from l-lysine by enzymatic decarboxylation through the constitutive lysine decarboxylase (LDCc)  or the acid-induced variant CadA  from Escherichia coli. Both enzymes use pyridoxal 5’-phosphate (PLP) as a cofactor. Kloss and coworkers showed a workflow where Corynebacterium glutamicum was used to produce l-lysine from glucose. The l-lysine was then enzymatically decarboxylated to yield DAP by the native EcLDCc, which was overproduced in E. coli, .
In biocatalysis such enzymatic conversions are often performed using whole cell systems or purified soluble enzymes, whereas Kloss et al. used catalytically active inclusion bodies (CatIBs) of the EcLDCc to decarboxylate l-lysine to DAP [7,8,9]. Even though purified enzymes can be used to catalyze reactions with high activities, their application requires respective costly and laborious downstream processing and purification procedures [10,11,12,13]. Moreover, the recycling of purified enzymes from biotransformations is more difficult to achieve and usually requires application of membrane separation, membrane reactor application or particle-based immobilization strategies [14,15,16].
To simplify the reusability and enhance the stability, immobilization of enzymes is often used, resulting in macromolecular or heterogeneous catalysts [17,18,19]. Common immobilization strategies rely first on the production of the soluble enzyme in an expression host. Subsequently, purification and lastly immobilization by e.g. covalent binding, cross-linking, binding the enzyme to carrier or entrapment of the enzyme is performed [20, 21]. However, enzyme immobilization often comes at the expense of overall activity of the immobilized enzyme preparation. This could be either due to reduced activity of the enzyme or the reduced mass transfer of reaction partners within the immobilized protein matrix.
A simpler and more cost efficient strategy is the use of CatIBs. For a long time, inclusion bodies (IBs) were regarded as inactive and misfolded protein aggregates. However studies revealed that catalytically active inclusion bodies with a reasonable residual activity can be produced by fusion of an enzyme of interest with a linker, composed of a few amino acids, and an aggregation inducing tag. Two recent reviews provided a comprehensive overview over suitable linker and aggregation inducing tags that have been successfully used for CatIB formation [22, 23]. The aggregation inducing tags in this study are the coiled coil domain of the cell-surface protein tetrabrachion from Staphylothermus marinus (TDoT) as well as the dimeric coiled coil domain from Pseudomonas aeruginosa (3HAMP) [9, 24, 25]. Moreover, the aggregation inducing tag properties of three artificial peptides, a small surfactant-like L6KD peptide, an amphipathic α-helical peptide (18AWT) and a hydrophobic self-assembling peptide (GFIL8) were also analyzed [26,27,28]. In contrast to other enzyme formulations CatIBs possess many advantages, such as (i) simple purification, (ii) high stability, (iii) easy long-term storage, (iv) carrier-free, biodegradable and biologically produced immobilization technology, (v) reusability as well as they are considered as (vi) essentially GMO-free after separation from the producer cells [9, 22, 24, 29, 30].
However, at present, there is only limited knowledge that would allow predicting a successful combination of a target enzyme, a linker and an aggregation inducing tag. For example, CatIB formation was tested for different enzymes, such as the benzaldehyde lyase from Pseudomonas fluorescens, the alcohol dehydrogenases from Ralstonia sp. and Lactobacillus brevis as well as for the Bacillus subtilis lipase A. Here, CatIBs with varying residual activity were formed, depending on the selected aggregation inducing tag [24, 26,27,28]. Thus, to realize efficient CatIB formation, many different variations need to be generated and tested to find the best-performing combination of target enzyme, linker and aggregation inducing tags. So far, most of the CatIBs described in literature were generated using traditional cloning methods, which limits the fast access to a CatIB library [24–28;31–35].
One option to create such a library is Golden Gate Assembly, which relies on Type IIS restriction enzymes. These enzymes cleave the DNA outside their recognition site, allowing the generation of specific desired overhangs. The generated four-nucleotide overhang can only be ligated to the matching DNA overhang from the following fragment. Because restriction digest and ligation happen at the same time, the reaction takes place in a so-called “one-pot setup” . Due to these features of the Golden Gate Assembly, three different DNA elements can be assembled in an effortless manner, thereby allowing the high-throughput generation of large CatIB libraries. This speeds up the search for the best performing CatIB-construct, while at the same time allowing the generation of large datasets useful for understanding structure/function relationships between the CatIB constituting modules. This in turn, could enable a more rational prediction of suitable elements for CatIB formation in the future.
Here, we report the generation and characterization of an EcLDCc-CatIB set, generated via Golden Gate Assembly. A combination of two different linkers and five different aggregation inducing tags were fused to the C-terminus of the EcLDCc resulting in ten different combinations. The resulting CatIB variants were analyzed comprehensively with regard to CatIB and cell morphology as well as activity of the CatIBs, proving that the linker and aggregation inducing tag revealed a strong influence on these features.
Results and discussion
Production of CatIBs and microscopic analysis
The lysine decarboxylase of E. coli (EcLDCc; EC 220.127.116.11), was C-terminally fused with one of two linkers (a flexible SG- or a rigid PT-Linker) as well as one aggregation inducing tag out of the set of five, TDoT, 18AWT, L6KD, GFIL8 and 3HAMP [9, 26,27,28, 37]. EcLDCc shows a decameric quaternary structure with the N-terminus being buried at the inner side of the decameric ring-like structure. Therefore, the linkers and the aggregation inducing tags were fused to the C-terminus of the EcLDCc. The ten different CatIB variants were produced in E. coli BL21(DE3) using M9 autoinduction medium (See Additional file 1: Table S2). The formation of EcLDCc-CatIBs in this host was verified using phase contrast microscopy with a 1000-fold magnification (see Methods). CatIBs appear as white refractive particles or granule-like structures at the cell poles (Fig. 1), which is typical for IBs .
Microscopic analyses of all strains were performed to test if the CatIB variants produce CatIBs with different morphologies, and if CatIB production, in turn, affects the morphology of the producing cells. The positive control (EcLDCc-Xa-SG-TDoT, more data about this variant was published by Kloss et al. ) formed dense CatIBs, whereas the negative control (empty pET28a vector) did not show any detectable IBs. Contrary to expectation, the wild type EcLDCc control also formed IBs, which usually is a consequence of strong gene expression and often results in complete activity loss of the enzyme [39,40,41].
Microscopic analysis of the EcLDCc-CatIB variants revealed that different combinations of linkers and aggregation inducing tags led to different shapes of cells and IBs and morphologies. IBs were found very similar with both linkers and with the aggregation inducing tags L6KD, GFIL8, and 3HAMP. In contrast, the TDoT variant formed large and dense IBs in combination with the flexible SG-Linker only, while the respective EcLDCc-PT-TDoT generated only small and diffuse IB structures and only 61 % of the cells carrying this construct produced IBs at all (Table 1). By contrast, the other CatIB producing variants showed that 71 % to 88 % of the cells produced CatIBs with a mean number of CatIBs per cell in the range of 1.18 for EcLDCc-PT-L6KD up to 1.83 for EcLDCc-PT-3HAMP. Strikingly, E. coli cells carrying constructs with the aggregation inducing tag 18AWT did not show any visible dense IBs at all. This might be because this tag is known to show a tendency to bind to the cell membrane , which could be responsible for the abnormal shape of the cells. Because of the absence of dense, refractive IBs, no further CatIB morphology analysis could be performed for these variants (Fig. 1). Absence of IBs in phase contrast microscopic images of the variants with aggregation inducing tag 18AWT, do not necessarily mean that there were no IBs at all. Small shaped or membrane associated IBs might had not detected, although IBs or even CatIBs could have been present. In this sense, different picture generating methods with higher precision, such as scanning electron microscopy could provide better insights.
Microscopic images were used for comprehensive image analysis to determine the size distribution of the CatIBs and their E. coli producer cells (Fig. 2). The cells, carrying the CatIB plasmid with the rigid PT-Linker, were smaller, except for the TDoT and 18AWT-Tag, compared to the cells with the flexible SG-Linker (Fig. 2a; Table 1). The cells producing the EcLDCc-PT-TDoT variant showed the largest cells (6.14 µm2) and the largest cell area distribution (1 µm2 to 6.14 µm2). The cell types producing the 18AWT variants revealed the smallest area (SG: 0.65 µm2, PT: 0.93 µm2) and the smallest median of the cell area distribution (SG: 2.01 µm2, PT: 2.11 µm2). These observations indicate that the linkers, as well as the aggregation inducing tags affect the cell morphology, i.e. size and shape.
Similar to the cell area analysis, the CatIB size analysis showed that the CatIBs seem to be smaller in combination with the PT-Linker (Fig. 2b). This time, also the TDoT variants showed the same trend. Only in combination with L6KD-Tag, the median of the distribution is similar for both linker types (PT: 0.66 µm2 vs. SG: 0.65 µm2) (Table 1). The TDoT-Tag combined with each one of the linkers revealed the smallest median of CatIB area and the smallest distribution of all variants (PT: 0.3 µm2 vs. SG: 0.38 µm2). Furthermore, EcLDCc-PT-TDoT revealed the smallest CatIB area per cell area (15 %) due to large cells with small IBs. Compared to that, EcLDCc-PT-L6KD showed the highest proportion of CatIB area per cell area (37 %) due to large IBs together with comparatively smaller cells. As mentioned before, no visible CatIBs were formed in combinations with 18AWT-Tag, which prohibited further morphological CatIB analysis. To conclude, the strongest influence on the CatIB area was observed for the aggregation inducing tag, while the two linkers showed quite similar data for the same aggregation inducing tag.
Downstream processing and enzymatic activity of ten EcLDCc-CatIB variants
Besides the retained enzymatic activity of the CatIBs, a simple purification procedure, as well as a final high overall yield are important factors. In the end, the CatIB variant will be preferred that can be produced in high amounts in the cells and shows a high activity after purification. Thus, to find the best CatIB variant, not only microscopic and activity analyses, but also the CatIB purification process was included in the evaluation.
A previously established purification protocol  was simplified by using lysozyme instead of a high-pressure homogenizer for cell disruption, and testing the CatIBs directly after purification without lyophilization to enable the testing of many CatIB variants in parallel. Aliquots containing the same amount of purified CatIBs were prepared and half of these aliquots were used for the determination of CatIB weight and the other half was used for activity measurements. After purification, the production of EcLDCc-CatIBs was verified by sodium dodecyl sulfate- (SDS) polyacrylamide gel electrophoresis (SDS-PAGE, Fig. 3). The SDS gel clearly shows respective bands of all EcLDCc-CatIB variants only in the insoluble pellet fraction. Besides, the wild type EcLDCc control showed a protein band in both the soluble and the pellet fraction. This is in good agreement with the microscopic images showing wild type EcLDCc IB formation to some extent (Fig. 1). Variations in the apparent molecular mass of the different CatIB fusion proteins are due to different sizes of the aggregation inducing tags, with 3HAMP (172 aa) and TDoT (50 aa) being larger than the short tags L6KD (8 aa), 18AWT (18 aa) and GFIL8 (8 aa).
After CatIB purification and analysis via SDS-PAGE, an enzymatic activity assay was performed in 50 mM Kpi buffer (pH 7.2) using l-lysine (10 mM) as a substrate and PLP (0.1 mM) as the cofactor. First, the reproducibility of the CatIB purification procedure and the enzymatic activity assay workflow were tested. To this end, three biological replicates, as well as three analytical replicates of each sampling point were sampled from EcLDCc-SG-L6KD and EcLDCc-PT-L6KD (Fig. 4). Activity of the CatIBs was determined by measurement of DAP formation from l-lysine over a time course of 20 minutes reaction time. Although both CatIB variants showed activity, L6KD in combination with the PT-Linker gave CatIBs with a much higher conversion rate (93 % after 3 min) compared to the SG-Linker variant (20 % after 3 min). The standard deviation between the different replicates was on average below 2.2 % for the analytical replicates and ≤ 5 % for most of the biological replicates, which proves high reproducibility of the experimental and analytical workflow procedures.
After having determined the reproducibility of the activity for the L6KD variants, the remaining eight CatIB constructs as well as controls were tested for their activity. As expected, the negative control, E. coli BL21(DE3) with an empty pET28a vector did not show any enzymatic activity (Fig. 5a; Table 1). Another control was the soluble fraction of the EcLDCc-SG-TDoT CatIB producing strain. The soluble fraction showed a very low conversion of l-lysine (4 % after 3 min) meaning that a very small portion of the EcLDCc was still present in the soluble fraction. Interestingly, the wild type EcLDCc displayed enzymatic activity in the pellet (57 % conversion after 3 min) as well as in the supernatant fraction (24 % conversion after 3 min). Strikingly, these natural CatIBs seemed to be more active compared to the supernatant fraction of the wild type enzyme. However, the wild type EcLDCc showed a smaller fraction on the SDS gel (Fig. 3), i.e., a substantial portion of the soluble protein fraction seemed to be converted into insoluble IBs during production of the recombinant protein. These natural IBs showed a higher specific volumetric productivity (specific Pv) compared to three of the SG-Linker variants (EcLDCc-SG-18AWT/L6KD/GFIL8). In comparison with all PT-Linker variants, the specific Pv of these natural IBs was lower (Table 1). Nevertheless, the conversion with the wild type EcLDCc reached only approx. 80 % in 20 min, which might be a result of low enzyme stability, resulting in deactivation of the enzyme.
The comparison of SG-Linker variants combined with different aggregation inducing tags revealed strongly differing activities between the five CatIB constructs (Fig. 5b; Table 1). The variant with the TDoT-Tag showed the fastest conversion rate (67 % after 3 min), followed by the 3HAMP variant (59 % after 3 min), the GFIL8 variant (41 % after 3 min), the 18AWT variant (36 % after 3 min) and the L6KD variant (20 % after 3 min). In contrast, the aggregation inducing tags in combination with the more rigid PT-Linker resulted in faster conversion (65 % to 93 % after 3 min) (Fig. 5c; Table 1). Interestingly, all CatIB variants with SG-/PT-Linker showed substantial enzyme activity. However, only two SG-Linker variants reached full conversion after 12 min, while all PT-Linker variants already reached full conversion at this time point, demonstrating superior performance of all PT-Linker variants. Strikingly, the L6KD aggregation inducing tag revealed opposite results when using the SG- or the PT-Linker, respectively. While the combination of L6KD with PT shows fastest conversion of all variants, the construct with the SG-Linker resulted in the slowest conversion of all variants. This clearly demonstrates that for the investigated EcLDCc CatIBs, the linker selection is a key factor of high relevance. The PT-Linker is expected to provide more rigidity than the SG-Linker and one may speculate that for the given example the linker rigidity might be an important structural aspect for the CatIB structure-function relationship.
A general comparison of the specific Pvs of the ten EcLDCc-CatIB variants clearly illustrated that the PT-Linker led to higher specific Pvs of the variants compared to the SG-Linker combinations (Fig. 6). Only the EcLDCc-SG-TDoT variant showed a higher specific Pv compared to the PT variant, namely EcLDCc-PT-18AWT. Furthermore, EcLDCc-SG-3HAMP just revealed a slightly lower specific Pv of EcLDCc-PT-18AWT. In both linker combinations the 18AWT-Tag showed the lowest or second to lowest specific Pv, which makes 18AWT the weakest aggregation inducing tag of these CatIB variants. Although the activity of the 18AWT variants were low, the fact that they show substantial activity is a striking result, since visible IBs were absent in the microscopic pictures (Fig. 1) and no activity might be expected. Thus, it can be assumed that insoluble structures were formed, that were not visible under the microscope, due to potential association with parts of the cell membrane like mentioned before .
Comparison of the enzymatic activity data, i.e., conversion after 3 min, with the specific Pv of the CatIB variants led to similar results (Table 1). This gives rise to the conclusion that the applied normalization of the amount of biomass prior to purification of the different CatIBs was an effective approach to harmonize the data. Moreover, the purification efficiency seemed to be quite similar for all variants, since the optical density of the cell suspensions were normalized beforehand, and similar intensities of the protein bands were observed (Fig. 3). This indicates that there was no general distortion of the data by the purification process. There was only a small change of EcLDCc-PT-3HAMP and EcLDCc-PT-TDoT, with EcLDCc-PT-3HAMP showing a slightly higher activity, which might be due to a slightly higher CatIB amount that was produced and purified from the cell culture. However, the most important finding can be derived from data of activity as well as specific Pv: (i) overall the PT-Linker variants showed a higher activities and specific Pv, (ii) the L6KD-Tag showed very different activity levels depending on the linker and (iii) 18AWT seemed to be the less suitable aggregation inducing tag for the tested system. Especially, the SG/PT-L6KD example showed that CatIBs that have the same morphology (Fig. 1) and the same amount of CatIBs per cell (Table 1) could provide very different enzymatic activity levels. The SG-Linker may result in less active CatIBs, since the portion of active enzyme inside the CatIBs could be less, or this linker may have led to a CatIB conformation that suffered from transport limitation of substrate.
Enzymatic activity vs. morphology of EcLDCc-CatIB variants
After analyzing the microscopic images as well as the enzymatic activity of the variants, both data were combined to see if the CatIB morphology had an impact on the enzymatic activity. In case of the 18AWT-Tag an abnormal cell morphology was found. The cells did not form dense, refractive IBs, resulting in only low enzymatic activity, volumetric productivity and specific volumetric productivity (Table 1).
Three out of four PT-Linker CatIB variants, for example the CatIBs of EcLDCc-PT-TDoT, showed smaller CatIB areas compared to the SG variants (PT-TDoT: 0.3 µm2 vs. SG-TDoT: 0.38 µm2). It is thus tempting to speculate that smaller IBs may retain higher enzymatic activity, possibly due to improved substrate supply to the active centers. The faster conversion rate of the PT-variants also resulted in higher PVs and specific PVs. However, in case of the TDoT variants, the enzymatic activity of both variants were in the middle range of all variants (Fig. 6). In this particular case, the size as well as the linkers seemed to have only a small impact on the enzymatic activity.
The CatIBs with the L6KD-Tags were the only ones that showed a similar size (PT: 0.66 µm2 vs. SG: 0.65 µm2), despite different linkers. Contrary to the above mentioned hypothesis, the similar morphologies of the L6KD-CatIBs were not reflected in their enzymatic activities, PVs nor specific PVs (Table 1). Whereas the combination of the SG-Linker with L6KD led to the lowest activity level (20 % conversion after 3 min), PV (105 g L− 1 d− 1) and specific PV (63 g L− 1 d− 1 gCatIB− 1) of all variants, the combination with the PT-Linker reached the highest activity levels (93 % after 3 min), PV (457 g L− 1 d− 1) as well as specific PV (256 g L− 1 d− 1 gCatIB−1). Whereas the aggregation inducing tag seemed to have a stronger effect on the CatIB and cell morphology (Fig. 1), especially, the different activity levels of L6KD showed that the impact of the linker on the activity was more pronounced.
Although there was no clear correlation between the microscopic data and enzymatic activity, the microscopic analysis is an important tool to prove the presence of IBs in the cells. Strains which do not form dense IBs and only show little cell growth, like in case of the EcLDCc-18AWT variants, can be dismissed and only the strains generating clearly visible CatIB structures need to be analyzed regarding their enzymatic activity to save time and resources.
All EcLDCc-CatIB variants tested showed at least some lysine decarboxylase activity. The most productive CatIB variant was L6KD in combination with the PT-Linker, showing a superior specific Pv. However, in combination with TDoT or 3HAMP, the SG-Linker showed lower specific Pv. Moreover, it was unexpected that the wild type EcLDCc control did form natural CatIBs. However, the specific Pv of the natural CatIBs was much lower compared to most of the generated set of CatIBs.
Finally, it is still challenging to determine the molecular factors which led to different activities observed for different CatIBs. The analysis of the ten EcLDCc-CatIB variants revealed no clear dependency on the particle size of the IBs. A more probable hypothesis could be a combination of more than one factor. For example, for the tested ten EcLDCc-CatIBs it turned out that the more rigid PT-Linker resulted in CatIBs which were more active resulting in a faster conversion rate. Besides the enzymatic activity, also mass transfer could have an impact on the conversion rate. The flexible SG-Linker possibly led to denser CatIB structures that might hinder efficient substrate diffusion to the inner part of the CatIBs or may results in incorrectly folded EcLDCc.
In summary, the results of our study demonstrate that for any given target enzyme the efficiency of formation and residual activity of CatIBs cannot be predicted beforehand. Thus, a large number of linkers and aggregation inducing tags need to be tested. However, the generation and testing of large CatIB libraries is time-consuming. Hence, automation of molecular biology workflows for CatIB construction, detection and activity determination are required to identify the optimal CatIB for each target enzyme.
Reagents and chemicals
All chemicals were purchased from ROTH and Merck (Sigma-Aldrich), unless stated otherwise. Enzymes for molecular biology were purchased from New England Biolabs GmbH (Frankfurt am Main, Germany).
Construction of expression plasmids
The synthetic gene of the EcLDCc, the two linkers, SG- and PT-Linker as well as the five aggregation inducing tags, TDoT-, 18AWT-, L6KD-, GFIL8- and 3HAMP-Tag, were synthesized by Synbio Technologies (Monmouth Junction, New Jersey, USA). The synthetic sequences contained the BsaI restriction and recognition sites, needed for Golden Gate Assembly. For Golden Gate Assembly, the synthetic gene encoding for EcLDCc was assembled with one of the two linkers, one of the five aggregation inducing tags as well as the so-called suicide plasmid in a ratio of 1:1:1:3. The suicide plasmid functioned as the expression plasmid backbone. It is a pET28a vector with an integrated ccdB gene, coding for the CcdB toxin, which is lethal for E. coli DH5α and E. coli BL21(DE3). It served as a control for accurate Golden Gate Assembly, because of zero-background cloning . During Golden Gate Assembly BsaI removed the ccdB gene and the T4-ligase inserted the CatIB-Linker-Tag sequence. After transformation of E. coli DH5α with the Golden Gate Assembly mixture only strains with the successful CatIB plasmid can grow while strains carry the original vector will be killed due to the produced toxin. Moreover, 2.5 % (v/v) T4-ligase as well as 2.5 % (v/v) BsaI restriction enzyme, were added to the mixture. The Golden Gate Assembly was performed in a PCR cycler (37 °C, 5 min and 16 °C, 5 min—cycles; 65 °C, 20 min). Information about all plasmids that were used in this study are summarized in Table S1, Additional file 1. The final expression plasmids were sequenced and verified for the correct assembly (Eurofins GmbH, Hamburg, Germany). Information about construction of the positive control strain EcLDCc-Xa-SG-TDoT together with experimental characterization is provided by Kloss et al. .
Protein production, cell disruption and protein purification
CatIB production was performed by cultivating E. coli BL21(DE3) carrying the respective expression plasmids in M9 autoinduction medium (See Table S2, Additional file 1). Following a modified protocol by Lamm et al. , 500 mL shaking flasks were used with a filling volume of 50 mL and a shaking frequency of 170 rpm (Infors HT Multitron Standard, Infors AG, Bottmingen, Swiss). The main cultivation was inoculated with an OD600 nm of 0.05 of an overnight culture in LB complex medium (37 °C, 170 rpm). The incubation was performed in two phases. The first one was a growth phase at 37 °C for 3 h, followed by a second phase at15°C for 69 h to produce active EcLDCc-CatIBs. The optical density of the main cultures was determined to perform a normalization of the cell cultures to OD600 nm = 12.5. The purification process was continued with 15 mL cell suspension with the specific optical density. The cells were harvested by centrifugation at 5000 xg for 10 min. Another centrifugation step (3 min at 5000 xg) was performed after washing the cell pellet with 10 mL of 0.9 % NaCl solution. Cell lysis was performed by adding 1.35 mL cell lysis buffer, BugBuster® HT Protein Extraction Reagent (Merck KGaA, Darmstadt, Germany) with the addition of 0.146 g L− 1 lysozyme, to the cell pellet. The suspension was incubated at 20 °C for 20 min and 750 rpm. After cell lysis the soluble and insoluble protein fraction were separated by centrifugation at 5000 xg for 30 min. The pellet was washed with 10 mL Milli-Q® followed by centrifugation. 15 mL Milli-Q® was added to the CatIB pellet and 1 mL aliquots in 1.5 mL Eppis were made. A centrifugation step was performed and the Milli-Q® was discarded (10,000 xg for 5 min). The pellets were used for enzyme assay or for weight determination. The CatIB weight was determined via drying the pellet at 80 °C for 24 h and was then weighed. The enzymatic assay samples were stored on ice at 4 °C overnight and used for enzyme activity measurements the next day.
Sodium dodecyl sulfate‐polyacrylamide gel electrophoresis (SDS-PAGE)
Sample preparation for SDS-PAGE analysis was performed by adding 2x Laemmli sample buffer to a purified CatIB-Milli-Q® suspension originated from a cell culture with a normalized OD600 nm of 12.5 (See Protein production, cell disruption and protein purification) as well as to the soluble fraction. After sample incubation for 10 min at 95 °C, the samples with the insoluble fraction were centrifuged for 5 min at 11,000 x g. Samples were applied to a Criterion™ 4–12 % Bis-Tris protein gel, 1.0 mm, with 18 wells (Bio-Rad Laboratories GmbH, Feldkirchen, Germany) together with a protein marker (PageRuler Prestained Protein ladder, ThermoFisher Scientific). Gel electrophoresis was performed in NuPAGE™ MES SDS running buffer (1×) at 200 V, 500 mA and 150 W. The gel was stained with SimplyBlue™ SafeStain. The theoretical molecular mass of the enzymes were determined by using the Protein isoelectric point calculator tool (http://isoelectric.org/).
Determination of lysine decarboxylase activity
Enzyme activity was determined by adding 1 mL of 50 mM Kpi buffer (pH 7.2), 0.1 mM pyridoxalphosphat (PLP) and 10 mM l-lysine to the CatIB pellet, originated from a cell culture with a normalized OD600 nm of 12.5 (See Protein production, cell disruption and protein purification and incubation). The soluble fraction, after cell lysis, was refilled to the normalized volume of 12 mL with Kpi-PLP-l-lysine ratio compared to the CatIB pellet fraction. 1 mL of the solution was used for the enzyme assay. The samples were incubated at 1000 rpm and 30 °C. Samples were taken after 0, 3, 6, 12 and 20 min and the enzyme was inactivated by adding 80 % (v/v) methanol and subsequently l-lysine and DAP concentrations were determined by HPLC to calculate conversion rate.
To determine the DAP and l-lysine concentration, an amino acid HPLC system (Agilent 1260 Infinity II, Agilent Technologies, Santa Clara, USA) was used. The system was equipped with a fluorescence detector (excitation: 230 nm; emission: 450 nm) and a C18 Kinetex Evocolumn (Phenomenex, Torrence, USA). Before injection, the samples for the enzyme assay (See Activity assay) were diluted with 50 mM Kpi Buffer (pH 7.2) to a final dilution ratio of 1:500 (v/v), filtrated and then 1:1 (v/v) diluted with 100 µM α-aminobutyric acid (Sigma-Aldrich, St. Louis, USA) as the internal standard (Sigma-Aldrich, St. Louis; USA). For analyzing l-lysine and DAP concentrations in the samples, an amino acid quantification method, including a pre-column derivatisation step at 18 °C using 9 µL ortho-phthaldialdehyde (OPA, Sigma-Aldrich) and 1 µL of the sample (6 mixing iteration steps). The mobile phase A contained 2.63 g L− 1 Na2HPO4, 2.08 g L− 1 NaH2PO4 and 0.5 % (v/v) THF in Milli-Q® water, and the mobile phase B contained 50 % (v/v) methanol, 45 % (v/v) acetonitrile, and 5 % (v/v) Milli-Q® water. Chromatographic separation was performed with a linear gradient that was applied with a flow rate of 1 mL min− 1 (0 % B, 0–2 min 0–38 % B, 2–6 min 38–42 % B, 6–7 min 42–70 % B, 713 min 70–100 % B, 13–17 min 100-0 % B). α-Aminobutyric acid showed an approximate retention time of 6.1 min, l-lysine of 9.6 min and DAP of 11.6 min. The DAP and l-lysine concentrations were calculated with a linear calibration curve of eight reference solutions (0.5 µM to 15 µM) after normalization with the internal standard peak area (calibration curve, See Additional file 1: Fig. S1).
Phase-contrast microscopic analysis was performed for E. coli BL21(DE3) strains with CatIB formation and for control strains. Cell suspension samples from cultivation experiments were taken before CatIB purification and analyzed by microscopy. A volume of 1 µL was applied on a microscope slide and covered with a coverslip. The microscope slide was positioned upside down on the desk of an inverted Nikon Eclipse Ti2 microscope (Nikon GmbH, Düsseldorf, Germany). The sample was observed with a CFI Plan Apo Lambda 100X Oil objective (Nikon GmbH, Düsseldorf, Germany) and images were taken with a Thorlab camera DCC154M-GL (Thorlabs Inc., Newton, New Jersey, USA). Analysis of cell images were performed with Fiji ImageJ  to determine the areas of at least 100 inclusion bodies and cells.
Availability of data and materials
All data generated or analyzed during this study are included in this article and its Additional file 1.
Catalytically active inclusion body
Gene of interest
- Pv :
- SDS-PAGE :
Sodium dodecyl sulfate polyacrylamide gel electrophoresis
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This work was funded by the state of North Rhine Westphalia (NRW) and the European Regional Development Fund (EFRE), Project “CLIB-Kompetenzzentrum Biotechnologie (CKB)” 34.EFRE-0300096 and 34.EFRE-0300097.
This work was funded by the state of North Rhine Westphalia (NRW) and the European Regional Development Fund (EFRE), Project “CLIB-Kompetenzzentrum Biotechnologie (CKB)” 34.EFRE-0300096 and 34.EFRE-0300097.
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Küsters, K., Pohl, M., Krauss, U. et al. Construction and comprehensive characterization of an EcLDCc-CatIB set—varying linkers and aggregation inducing tags. Microb Cell Fact 20, 49 (2021). https://doi.org/10.1186/s12934-021-01539-w
- Catalytically active inclusion bodies
- Protein aggregates
- Protein engineering
- Downstream processing
- Microscopic analysis