Genetic engineering of Pyrococcus furiosus to use chitin as a carbon source
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Bioinformatic analysis of the genes coding for the chitinase in Pyrococcus furiosus and Thermococcus kodakarensis revealed that most likely a one nucleotide insertion in Pyrococcus caused a frame shift in the chitinase gene. This splits the enzyme into two separate genes, PF1233 and PF1234, in comparison to Thermococcus kodakarensis. Furthermore, our attempts to grow the wild type strain of Pyrococcus furiosus on chitin were negative. From these data we assume that Pyrococcus furiosus is most likely unable to use chitin as a carbon source. The aim of this study was to analyze in vivo if the one nucleotide insertion is responsible for the inability to grow on chitin, using a recently described genetic system for Pyrococcus furiosus.
A marker-less genetic system for Pyrococcus furiosus was developed using simvastatin for positive selection and 6-methylpurine for negative selection. Resistance against simvastatin was achieved by overexpression of the hydroxymethylglutaryl coenzyme A reductase gene. For the resistance to 6-methylpurine the hypoxanthine-guanine phosphoribosyltransferase gene was deleted. This system was used to delete the additional nucleotide at position 1006 in PF1234. The resulting chitinase in the mutant strain was a single subunit enzyme and aligns perfectly to the enzyme from Thermococcus kodakarensis. A detailed analysis of the wild type and the mutant using counted cell numbers as well as ATP and acetate production as growth indicators revealed that only the mutant is able to use chitin as a carbon source. An additional mutant strain containing a reduced chitinase version containing just one catalytic and one chitin-binding domain showed diminished growth on chitin in comparison to the mutant containing the single large enzyme.
Wild type Pyrococcus furiosus is most likely unable to grow on chitin in the natural biotope due to a nucleotide insertion which separates the chitinase gene into two ORFs, whereas a genetically engineered strain with the deleted nucleotide is able to grow on chitin. The overall high sequence identity of the two chitinases between P. furiosus and T. kodakarensis indicates that this mutation occurred very recently or there is still some kind of selection pressure for a functional enzyme using programmed +/−1 frameshifting.
KeywordsChitin Simvastatin Chitinase Chitinase Gene Colloidal Chitin
Chitin binding domain
Polymerase chain reaction
Chitin is the second most abundant polysaccharide on earth after cellulose. It is the major component of the exoskeletons of insects, the shells of crustaceans and of fungal cell walls . Chitin consists of N-acetylglucosamine subunits which are linked by β-1,4-glycosidic bonds. The degradation of chitin is catalyzed by chitinases which hydrolyze these β-1,4-glycosidic bonds. Based on amino acid sequence similarity, chitinases have been classified into the glycoside hydrolases families 18 and 19 . Family 18 chitinases contain a multidomain structure and are widely distributed in all domains of life. The common features of these enzymes are catalytic domains which consists of a (βα)8 (TIM barrel) fold with a conserved DXDXE motif and chitin-binding domains (ChBD) which are involved in the binding to the substrate [3, 4].
Most chitinases described so far have been found in the eukaryal and the bacterial domains . Within the domain of Archaea, only ten euryarchaeal chitinases and one crenarchaeal have been identified so far . Most of these archaeal enzymes have been only annotated by sequence comparison. Experimental data about the activity and the structure of the enzymes are limited to the genera of Halobacterium, Thermococcus and Pyrococcus[7, 8, 9, 10]. The first and best characterized archaeal chitinase was from Thermococcus kodakarensis[7, 11]. A mutational analysis revealed that the enzyme possesses two catalytic domains (A and B) and three ChBDs . The N-terminal catalytic domain A functions as an exochitinase and liberates diacetyl-chitobiose. The C-terminal catalytic domain B acts as an endochitinase which produces N-acetyl-chitooligosaccharides of various length, which could be further hydrolyzed to diacetyl-chitobiose by the N-terminal catalytic domain A. Further degradation to N-acetylglucosamine is the result of a concerted action of diacetyl-chitobiose deacetylase and exo-β-D-glucosaminidase .
In contrast to the single chitinase of Thermococcus kodakarensis the chitin-degrading enzymes of Pyrococcus furiosus are encoded by two open reading frames ChiA (PF1234) and ChiB (PF1233) which are separated by 37 nucleotides . The gene product of PF1233 has a ChBD and a catalytic domain which is closely related to the T. kodakarensis catalytic domain B. The structure of this catalytic domain was determined in detail by NMR and X-ray analysis [13, 14, 15]. These data also indicate an endochitinase activity for PF1233 very similar to T. kodakarensis, however in contrast to the extracellular T. kodakarensis enzyme, the separated P. furiosus enzyme has no signal peptide at the N-terminal region. This would mean that the P. furiosus enzyme is intracellular and the substrates have to be imported into the cell.
A few years ago, Oku and Ishikawa suggested a different explanation for this observation: In principle, P. furiosus has also a single chitinase gene like T. kodakarensis, but a one nucleotide insertion at position 1006 in PF1234 caused a frame shift which resulted in the separation of the chitinase gene into two genes. Furthermore, their attempts to grow P. furiosus on chitin failed . This result is in perfect agreement with previous growth experiments on chitin which also failed [17, 18]. So far, there is only one report that P. furiosus is able to use chitin as a carbon source .
To reveal this issue, we used a genetic system for P. furiosus which allows the removal of the one nucleotide insertion in PF1234 to redesign the chitinase to a single enzyme . Growth experiments with the wildtype and the mutant clearly demonstrate that the wild type strain of P. furiosus is - in contrast to the mutant with the redesigned chitinase - unable to efficiently use chitin as the main carbon source.
Strains and growth conditions
P. furiosus was cultivated at 90°C in SME medium, as described previously . For the growth of Pyrococcus strain MUR27Pf with the deleted xanthine-guanine phosphoribosyltransferase gene (xgprt) the medium was supplemented with 6 mM guanosine monophosphate (Sigma, St. Louis, USA). For solidification, gelrite was added to a final concentration of 1%. The antibiotic simvastatin (Toronto Research Inc., Toronto, Canada) was dissolved in ethanol and 6-methylpurine (Sigma, St. Louis, USA) was dissolved in water. Both supplements were sterilized by filtration. SME-chitin medium was supplemented with 0.5% colloidal chitin, 0.025% yeast extract and 0.025% peptone.
For preparation of colloidal chitin 20 g of chitin powder (practical grade, from shrimp shells; Sigma, St. Louis, USA) were mixed with at least 200 ml 37% HCl (pre-cooled to 4°C) and stirred for 1 h at 4°C . The suspension was poured into 1 l of H2O (pre-cooled to 4°C) and was filtered through paper filter (311853, Schleicher and Schüll, Dassel, Germany). The filtrate was washed three times with 1 l of H2O, resuspended in 1 l of H2O and neutralized by the addition of NaOH until pH 7.0. The suspension was filtered and washed with 3 l of H2O to deionize the chitin. The resulting suspension was filtered and a part was dried to determine the content of liquidity.
Escherichia coli strain DH5α was used as a host strain for plasmid constructions and was cultivated at 37°C in Luria-Bertani (LB) medium. For the selection of transformants, ampicillin was added at 100 μg ml-1 to the medium.
General DNA manipulations and plasmid constructions
Restriction enzymes and DNA polymerases for PCR reactions were purchased from NEB (Ipswich, USA). Plasmid DNA and DNA fragments from agarose gels were isolated using a Wizard® Plus SV Miniprep DNA Purification System or Wizard® SV Gel and PCR Clean-Up System from Promega (Mannheim, Germany). DNA sequencing was performed by Seqlab (Göttingen, Germany). Genomic DNA from P. furiosus wild type and genectically engineered strains was isolated as described previously .
The plasmid pMUR37 was created to enable a markerless deletion of PF1950 (xgprt). It contained three DNA fragments which were joined by single overlap extension PCR reactions: An upstream region of PF1950 (primers Pf1950single_mi_fus-F 5´ -aacagaagtttaagccttcgaagaattgggaagagggaga-3´ and Pf1950ml_up_fus1500bp_R 5´ -gctttttccttatccactacttatatgaccgcaggtattc-3´ ), a downstream region of PF1950 (primers Pf1950ml_mi-fus1500bp_F 5´ -gaatacctgcggtcatataagtagtggataaggaaaaagc-3´ and Pf1950_hr_do_R 5´ - gttgaaacagttgcaactcttgg-3´ ) and for the selection with simvastatin the resistance cassette (primers Pf1950single_up_BamHI_F 5´ -gggcccggatccgggcatttcatcattttt-3´ and Pf1950single_up_fus_R 5´ -tctccctcttcccaattcttcgaaggcttaaacttctgtt-3´ ) as described previously . The fused fragment was hydrolyzed with BamHI and SacI and was ligated into the corresponding sites of pUC19.
For the construction of the plasmids pMUR47 and pMUR50, a modified pUC19 plasmid with an additional AscI recognition sequence within the multiple cloning site was used. For both constructs two PCR fusion products were ligated using a common NotI restriction site and inserted into the modified vector using AscI and SbfI restriction sites.
In the case of pMUR47 the first fusion PCR product with the deleted nucleotide was created using the following two primer pairs: (Pf1234_AscI_F 5´ -atcgaaggcgcgcctgctcggtattgtgcttgc-3´ /Pf1234_Del_Fus_R 5´ -tttatcttctaattcggcttgatc-3´ ) and (Pf1233_Del_Fus_F 5´ -ataaaaaagagtatctcctaactgcagc-3´ / Pf1233_NotI_A_R 5´ -ggtgcagcggccgctggagttggtgatggtgttg-3´). The second fusion PCR product consisted of a two-gene resistance cassette which was needed for the selection-counter-selection system. The resistance cassette contained a gdh promoter, the hmgCoA reductase from T. kodakarensis, the region coding for the xgprt (PF1950) and the histone A1 terminator sequence of P. furiosus. The first part was amplified using the primers SimV_NotI_F 5´ -gatgcgcggccgcgggcatttcatcatttttatgaactttgatgaacg-3´ and SimV_Rv 5´ -tcaccctagaaaaagataagcc-3´ . For the second part, the primer pair Pf1950_F_fus1233A 5´ -gcttatctttttctagggtgacctgggatccaattaccg-3´ and Pf1233_SbfI_R 5´ -atacggcctgcaggttggagtgggtgtggg-3´ was used. Both PCR products were combined with single-overlap extension PCR.
Plasmid pMUR50 was constructed by combination of a PCR product containing the upstream region up to the signal peptide region of PF1234 (primers Pfup1234_AscI_B_F 5´ -atacgaggcgcgccaactccaatttccctgagc-3´ and Pf SP_up1234_ R 5´ -ggccgatactggatagaatagagatat-3´ ) and a PCR product coding for the catalytic domain of PF1233 (primers Pf SP_1233_fus_F5´ -tatccagtatcggccactacccctgtcccag-3´ and Pf1233_NotI_B_R 5´ -cctaatgcggccgctagaggaattgagcctgc-3´ ). The resulting PCR product was combined with the PCR-amplified resistance cassette using primer pair Pf1950_NotI_F 5´ -tagcatgcggccgctcaccctagaaaaagataagcc-3´ and PfhmgCoA_SbfIR 5´ -gataggcctgcagggggcatttcatcatttttatg-3´ and inserted into the modified vector as mentioned before. The resulting constructs were verified by DNA sequencing.
Transformation of P. furiosus
Standard heat shock transformation of P. furiosus was performed as described previously . To obtain the marker-less mutant MUR27Pf, circular plasmid DNA of pMUR37 was used and the corresponding transformants were selected with 10 μM simvastatin in SME-starch liquid medium at 85°C for 48 h. Pure cultures of the intermediate mutant MUR27Pf_i were obtained by plating the cells on solidified medium in the presence of 10 μM simvastatin. The integration of the plasmid into the genome by single cross-over was verified by analyzing corresponding PCR products.
Cultures of the correct intermediate mutant were washed with medium under anaerobic conditions to remove the simvastatin. In detail, 1.5 ml of a grown culture were centrifuged in an anaerobic chamber for 4 min at 6,000g and resuspended in fresh culture medium without simvastatin. This procedure was repeated three times. For the counter selection the cultures were plated in the presence of 50 μM 6-methylpurine to induce a second homologous recombination step to recycle the selection marker and to eliminate integrated plasmid sequences. In the case of mutant MUR23Pf linearized plasmid pMUR47 was used for the transformation. The genotype of the final mutants was confirmed by PCR and Southern blot experiments.
Growth analysis on chitin medium
For a more detailed analysis of the growth behavior of Pyrococcus on chitin, bottles with 200 ml chitin medium were used and incubated at 90°C. Cell numbers were analyzed with a Thoma counting chamber (0.02-mm depth; Marienfeld, Lauda-Königshofen, Germany) using a phase-contrast microscope.
For the preparation of cell extracts to measure the ATP content, 0.5 ml of Pyrococcus cultures was centrifuged (3 minutes, 10,000g). The cell pellet was washed three times in 0.8 ml PBS buffer, resuspended in 200 μl PBS and treated with glass beads using a FastPrep-24 (M. P. Biomedicals, Irvine, CA) for cell lysis. After centrifugation (10,000g for 3 minutes at 4°C), the ATP amount in the supernatants was quantified by a luciferin/luciferase assay (FluoProbes, Interchim, Montluçon Cedex, France) using a portable tube luminometer (Junior LB 9509, Berthold Technologies, Bad Wildbad, Germany) according to the instruction manual.
The amount of acetate in the culture supernatant was analyzed using an enzymatic acetate determination kit (R-biopharm, Darmstadt, Germany). For quantification 0.5 ml of a Pyrococcus culture was centrifuged and used as indicated in the operating guidelines.
Results and discussion
To exclude the possibilities that the presence of this additional nucleotide is caused by a sequencing error or is only present in the P. furiosus strain used for the genome sequencing project  we ordered a new P. furiosus strain (DSM 3638) from the DSMZ and confirmed the presence of this additional nucleotide by sequencing of a corresponding PCR product (data not shown).
In vitro experiments using an artificial recombinant chitinase from P. furiosus, heterologously expressed in E. coli, indicate that the single enzyme constructed by the deletion of the additional nucleotide is much more active than the separated wild type enzymes . To investigate if this finding from the in vitro experiments could be confirmed by in vivo data we used a modified version of the recently developed genetic system for P. furiosus to delete this additional nucleotide in the genome .
As the genetic system described so far is based on a shuttle vector and did not allow the modification of genes within the genome we started the genetic modification of P. furiosus with the establishment of a selection/counter selection (pop-in/pop-out) system according to a genetic system which was recently described for T. kodakarensis[23, 24]. Santangelo et al. demonstrated that the deletion of the xgprt gene (TK0664) confers resistance to 6-methylpurine. First experiments to inactivate the corresponding gene PF1950 in P. furiosus indicated that this gene can be also used for counter selection experiments in P. furiosus (data not shown).
This strong difference in the observed acetate concentrations clearly indicates that the genetically engineered P. furiosus strain uses chitin as a carbon source. Chitin is highly acetylated and we therefore assume that acetate is released from the chitin during growth of P. furiosus. In comparison, in an experiment with similar cell density and incubation time grown on cellobiose as substrate, an acetate concentration of about 4 mM was observed . Due to the insolubility of the chitin and the fact that many cells stick on the chitin it was very difficult to report reliable OD values, but the visual inspection of the incubated bottles of the wild type and the mutant strain clearly demonstrated chitin degradation (Figure 4C). The bottle containing the wild type after an incubation of 55 h still exhibited a milky turbidity due to the insolubility of the chitin. In contrast, the amount of insoluble chitin in the bottle with the genetically engineered P. furiosus strain was considerably reduced (Figure 4C). Figure 4D shows a phase contrast microscopic picture of the mutant strain. It can be clearly seen that the cells are attached to the chitin particles.
The experiments presented so far clearly indicate that the P. furiosus strain with the redesigned chitinase can grow much better on colloidal chitin than the wild type strain. In this context it is interesting to note the overall high sequence identity of the two chitinases between P. furiosus and T. kodakarensis. This indicates that this mutation occurred very recently or there is still some kind of selection pressure for a functional enzyme. It is possible that P. furiosus is able to synthesize the chitinase as a single enzyme using programmed +/−1 frameshifting which enables the ribosome to bypass the frameshift . This situation was recently described for the expression of the fucA1 gene in Sulfolobus acidocaldarius. However, in this case the expression efficiency is only about 5% in comparison to a gene without the programmed frameshift . To exclude or to confirm the idea of programmed frameshifting additional experiments will be necessary. It is not possible to use available proteomics data of P. furiosus to support this idea as the available proteomics data do not match the chitinases. Furthermore, first attempts to use purified enzyme for a detailed mass spectrometry-based analysis were complicated by the finding that the enzyme is most likely the target of intensive proteolytic cleavage activity (data not shown).
Our data demonstrate that wild type P. furiosus is most likely unable to use chitin as a main carbon source due to a one nucleotide insertion which splits the chitinase into two separate enzymes. In contrast, a genetically engineered strain with the deleted nucleotide is able to grow on chitin. The overall high sequence identity of the two chitinases between P. furiosus and T. kodakarensis indicates that this mutation occurred very recently or there is still some kind of selection pressure for a functional enzyme using programmed +/−1 frameshifting . As the later one resulted in a very low expression level of the chitinase, we conclude that P. furiosus does not rely on chitin as a major carbon source in the natural biotope.
We thank Renate Richau for technical assistance and Emma Gagen for critical reading of the manuscript. The work was supported by the Deutsche Forschungsgemeinschaft TH 422/11-1.
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