- Methodology article
- Open Access
Reconstitution of Drosophila and human chromatins by wheat germ cell-free co-expression system
BMC Biotechnology volume 20, Article number: 62 (2020)
Elaboration of the epigenetic regulation of chromatin is a long-standing aim in molecular and cellular biology. Hence, there is a great demand for the development of in vitro methods to reconstitute chromatin that can be used directly for biochemical assays. The widely used wheat germ cell-free protein expression method provides broad applications to investigate the function and structure of eukaryotic proteins. Such advantages, including high translation efficiency, flexibility, and possible automatization, are beneficial for achieving native-like chromatin substrates for in vitro studies.
We describe a novel, single-step in vitro chromatin assembly method by using the wheat germ cell-free protein synthesis. We demonstrated that both Drosophila and human chromatins can be reconstituted in the course of the in vitro translation of core histones by the addition of chromatin assembly factors, circular plasmid, and topoisomerase I in an ATP-dependent manner. Drosophila chromatin assembly was performed in 4 h at 26 °C, in the presence of premixed mRNAs encoding the core histones, dAcf1/dISWI chromatin remodeling complex, and nucleosome assembly protein, dNAP1. Similarly, the human chromatin was assembled by co-expressing the human core histones with Drosophila chromatin remodeling factor, dISWI, and chromatin chaperone, dNLP, for 6 h at 26 °C. The presence of reconstituted chromatin was monitored by DNA supercoiling assay, also the regular spacing of nucleosomes was assessed by Micrococcal nuclease assay. Furthermore, Drosophila linker histone H1-containing chromatin was reconstituted, affirming that the in vitro assembled chromatin is suitable for downstream applications.
The method described in this study allows the assembly of Drosophila and human chromatins, possibly in native-like form, by using a wheat germ cell-free protein expression. Although both chromatins were reconstituted successfully, there were unexpected differences with respect to the required ratio of histone-coding mRNAs and the reaction time. Overall, our new in vitro chromatin reconstitution method will aid to characterize the unrevealed structure, function, and regulation of chromatin dynamics.
Chromatin enables high-level compaction of the enormous genomic DNA into a few microns of nuclei in every eukaryote. The histone octamer, that is composed of four core histones, H2A, H2B, H3, and H4, is tightly wrapped around by approximately 147 base pair of DNA in a left-handed superhelix [1,2,3,4]. Moreover, spatiotemporal changes of chromatin post-translational modification and its overall structure during the cell-cycle contribute to multiple cellular processes such as DNA replication [5, 6], repair [7, 8], gene regulation [9,10,11], and cell proliferation [12, 13]. Such chromatin dynamics have been studied for decades, and chemical modifications on the N-terminal regions of histones are thought to play pivotal roles in the prior processes.
The first detailed nucleosome structure was described by determining the X-ray crystallography of the refolded, purified, and in vitro assembled nucleosome on human α-satellite DNA . Since then, various nucleosome structures from different organisms were determined at higher resolution by X-ray crystallography and other methods [4, 14], additionally, oligomeric nucleosomal structures were obtained by cryo-electron microscopy . The majority of the abovementioned approaches utilize unmodified/purified/refolded four core histones with defined DNA sequences that possess nucleosome positioning capability, and the assembly was achieved by the salt gradient method [16,17,18]. Based on these determined structures, the influence of particular post-translational modification of histone tails on nucleosome has been widely studied. For instance, the partially synthetic histone H4 K16Ac along with the other three core histones was assembled into nucleosome in vitro, and the physicochemical characterization of the modified nucleosome was determined . Additionally, the detailed analysis of the effect of the fully chemical synthetic K56 acetylated histone H3 on nucleosome formation was reported . Furthermore, similar approaches were taken place to understand the role of post-translational modifications of histone proteins on the chromatin structure and functions [21, 22].
Besides the salt dialysis chromatin reconstitution technique, ATP-dependent chromatin assembly methods have been applied in a vast range of chromatin research, which utilizes a set of chromatin assembly factors [23,24,25,26]. The first report was published by using the Xenopus laevis oocytes extract, and the assembly of nucleosome was determined to be ATP-dependent . Then, Becker and Wu published the method by using a Drosophila melanogaster embryo cell-free system, and it was shown that unknown factors in the embryo facilitated the formation of chromatin . Later, several key factors in the Drosophila embryo were defined, including ATP-utilizing assembly factor (dAcf1 and dISWI), and nucleosome assembly protein-1 (dNAP1), that together help to assemble the regularly spaced chromatin, and became one of the standard methods [25, 26, 28]. The ATP-dependent chromatin assembly methods have been often employed to investigate the molecular mechanisms of the way of the chromatin assembly in the cell nuclei since this chromatin reconstitution procedure is more analogous to the physiological process, compared to the abovementioned salt dialysis method. Recently, Kadonaga’s group reported that by using bacterially produced chromatin assembly factors, dISWI and dNLP, human chromatin reconstitution can be attained in vitro .
In this study, we sought to develop a novel chromatin reconstitution method by using a well-established wheat germ cell-free protein synthesis [30, 31] and on the basis of conventional chromatin assembly methods [25, 26, 28, 29]. The wheat germ cell-free protein synthesis is known to enable the production of N-methionine processed, native, and functional protein, thus making it the ideal method of choice for chromatin reconstitution [32, 33]. Previously, we and others successfully synthesized dozens of proteins of different organisms by using the wheat cell-free system [34,35,36,37,38,39], thus we applied this method for the expression of the Drosophila and human core histones, ATP-utilizing assembly factor, nucleosome assembly protein, and histone chaperone. For achieving the reconstitution of both Drosophila and human chromatins in co-expression manner, each set of core histones was translated along with the appropriate pairs of Drosophila chromatin assembly factors. Furthermore, the ratio of the mRNAs of core histones and incubation time were optimized in both Drosophila and human chromatin assembly systems. Finally, the reconstituted chromatins were evaluated by supercoiling and Micrococcal nuclease (MNase) assays. Overall, we describe a single-step in vitro chromatin assembly method, which may serve as a new, viable protocol for chromatin research and epigenetic studies.
Histones and chromatin assembly factors synthesized by wheat germ cell-free synthesis
The Drosophila core histones DmH2A, DmH2B, DmH3, and DmH4, and chromatin assembly factors, dAcf1, dISWI, and dNAP1 were cloned into the pEU-E01-MCS expression vector from the original pET plasmids [26, 40]. The Drosophila nucleoplasmin, dNLP, coding gene was amplified from the cDNA library of adult Drosophila whole body, then cloned into the pEU-E01-MCS vector. The human core histones were amplified from the human cDNA library and cloned into a pEU-E01-LICNot expression vector . The pEU vector used in this study has been optimized to maximize the efficiency of in vitro wheat germ-based cell-free protein synthesis [41, 42]. The applied vectors do not possess an affinity tag coding region since we aimed to achieve the physiological state of histones and a single-step nucleosome assembly without affinity purification. Additionally, we performed a proteomic analysis of the wheat germ extract in order to confirm that there is no detectable wheat histone peptide in the extract (see Additional file 1). In the total of 744 proteins identified in the wheat germ cell-free extract, the most abundant proteins were annotated as heat shock proteins, followed by the proteins that related to protein synthesis such as a translation elongation factor. There were no wheat core histones H2A, H2B, H3, nor H4 found in the wheat extract. Prior to performing in vitro chromatin assembly reaction, all target genes were transcribed in vitro, and each protein product was cell-free synthesized in a cup dialysis mode and analyzed on SDS-PAGE gel (Fig. 1). Total translation mixtures of Drosophila core histones (Fig. 1a), along with human counterparts (Fig. 1b), and Drosophila chromatin assembly factors, dACF1, dISWI, dNAP1, and dNLP (Fig. 1c and d) were successfully produced with their expected molecular weight (Table 1). Among synthesized Drosophila core histones, DmH2A and DmH2B were synthesized less effectively, ~ 70% than DmH3 and DmH4 under a bilayer method using the same amount of mRNAs. In contrary to Drosophila core histones, the human histones HsH2A, HsH2B, HsH3.1, and H4 were produced less effectively by the bilayer method, ~ 20% of corresponding Drosophila histones, thus human core histones were synthesized by the cup dialysis mode (Fig. 1b), which is a more robust way of wheat cell-free synthesis . By densitometry analysis of the SDS-PAGE, HsH2A, HsH2B, and HsH3.1 seemed to be synthesized equally, however, the product of HsH4 was ~ 30% less than other core histones. The further use of the wheat cell-free protein synthesis for chromatin assembly method was convincing based on the protein expression profiles.
Assembly of Drosophila chromatin using wheat germ cell-free synthesis
Generally, Drosophila chromatin assembly methods employ either bacterially expressed and refolded histones or native histones extracted from eukaryotic cell nuclei, along with the ATP-dependent chromatin remodeling factor and nucleosome assembly factor in the presence of template DNA [23, 43, 44]. To develop a new chromatin assembly method by using wheat germ cell-free translation, initially, we aimed to reconstitute Drosophila chromatin with the reported ATP-dependent chromatin remodeling factors and nucleosome assembly chaperone, dAcf1, dISWI, and dNAP1 [25, 26]. The scheme of our novel single-step chromatin assembly method is shown in Fig. 2, which describes the in vitro co-expression of proteins, and the reconstitution of chromatin can be accomplished concurrently in one tube. We hypothesized, if histones and chromatin assembly factors are synthesized successfully, translation and assembly may occur concomitantly. To perform the co-expression chromatin assembly in the wheat cell-free system, a set of the pre-transcribed mRNAs encoding four core histones DmH2A, DmH2B, DmH3, and DmH4 were co-translated with the mRNAs of Drosophila chromatin assembly factors, dAcf1, dISWI, and dNAP1 in the presence of carrier DNA with unbiased sequence, pBSK plasmid and a trace amount of topoisomerase I enzyme under a bilayer mode. For ease, the two premixed mRNAs encoding core histones were prepared by pairwise, DmH2A/DmH2B, and DmH3/DmH4 for translation-coupled chromatin assembly reaction. The ratio of mRNAs of DmH2A/DmH2B and DmH3/DmH4 was optimized in order to make equimolar proteins among the histone octamers during the reaction. According to the earlier studies, the in vitro Drosophila chromatin assembly may be completed in 2 to 4 h [26, 45]. Thus, a series of different ratio of mRNAs encoding DmH2A/DmH2B and DmH3/DmH4 was tested that range from 2:1, 1.5:1, 1:1, 1:1.5, and 1:2, and incubated for 4 h at 26 °C. Importantly, the amount of expected histone protein products to the DNA template in this reaction condition was adjusted to be around 1:1 (w/w) mass ratio by estimating the histone synthesis for 4 h. Subsequently, the formation of circular chromatin was verified by DNA supercoiling assay (Fig. 3a and Fig. S1a), which is a standard method to evaluate chromatin assembly on closed circular DNA [46, 47]. Under the tested assembly condition, the 1.5:1 and 2:1 ratio of DmH2A/DmH2B to DmH3/DmH4 resulted in the highest degree of supercoil formation, consistent with the observation of independent histone protein synthesis shown in Fig. 1a. The following experiments were performed by applying the 1.5:1 ratio of the mRNAs (DmH2A/DmH2B:DmH3/DmH4). Next, we aimed to test the reaction time as 1, 4, and 6 h, followed by supercoiling assay (Fig. 3b and Fig. S1b). We concluded that Drosophila chromatin was sufficiently reconstituted after 4 h and unchanged after prolonged reaction time. To test whether the assembled chromatin is canonical DNA-histone octamer complex or not, in other words, if DNA is wrapped around histone octamers for the expected length, we assessed the apparent nucleosome repeat length (NRL) by MNase assay (Fig. 3c). The formation of mono-, di-, and trinucleosomes was observed after 5 min of MNase digestion, and the domination of mononucleosomal DNA was detected under longer MNase digestion. The average NRL of rigorous digestion by MNase was estimated at 152 ± 3 bp, in agreement with the reported nucleosomal DNA of around 145–147 bp [3, 4, 45]. From these results, the Drosophila chromatin was assembled in the system of co-expression wheat cell-free synthesis, proven by the supercoiling formation with the canonical nucleosome unit, an octamer wrapped around 1.7 times by approximately 150 bp DNA.
Human chromatin assembly using wheat germ cell-free synthesis
Following the success of the Drosophila in vitro chromatin assembly, the reconstitution of human chromatin was tested in a co-expression manner in the presence of appropriate chromatin assembly factors and pBSK plasmid. Despite a long history of in vitro chromatin reconstitution of the Drosophila system, the human chromatin reconstitution had been somewhat challenging until recently. A recent report described the details of in vitro human chromatin assembly , of which they utilized dISWI and dNLP as essential chromatin assembly factors. Thus, we carried out the reconstitution of human chromatin by the in vitro co-expression of human core histones and Drosophila dISWI and dNLP in a bilayer mode. Analogous to the Drosophila chromatin assembly reaction for 4 h at 26 °C, the ratio of HsH2A/HsH2B to HsH3.1/HsH4 was first assessed by the best degree of supercoiling formation (Fig. 4a and Fig. S2a), and an optimum mRNA ratio between HsH2A/HsH2B and HsH3.1/HsH4 was determined to be 1:1.5 and 1:2. Under the optimized histone mRNA ratio of 1:2 (HsH2A/HsH2B:HsH3.1/HsH4), the reconstitution reaction time was tested for 1, 4, 6, and 8 h followed by supercoiling assay (Fig. 4b and Fig. S2b). From this result, apparent complete supercoiling was obtained after 6 h, which is longer than the reported incubation time . In the previous study, human chromatin was reconstituted by a two-step method, an initial pre-reconstitution of histone octamers extracted from the HeLa cells with dNLP followed by an ATP-dependent enzymatic core histone assembly on DNA. Hence, the current one-step co-expression chromatin assembly method is different from the reported reaction scheme, and we rationalize that this difference may affect reaction time. The in vitro reconstituted human chromatin was analyzed by MNase assay, and mono-, di-, tri-, and tetranucleosomes were obtained under a series of digestion time (Fig. 4c). The average NRL of human chromatin was assessed at around 152 ± 7 bp, suggesting that the newly assembled human chromatin in a co-expression protocol indeed consistent with the canonical nucleosome unit .
Co-expression of four core histones and linker histone H1 assembly
To provide evidence that the reconstituted chromatin can be used for further downstream applications, we had assessed whether the linker histone H1 could be assembled into Drosophila chromatin. DmH1 was amplified from Drosophila cDNA, cloned, in vitro transcribed, then in vitro translated (Fig. 5a). Co-expression Drosophila chromatin assembly was performed in the presence of the premixed mRNAs of four core histones, three chromatin assembly factors, and DmH1-coding mRNA. The NRL of reconstituted chromatins was assessed by MNase assay in the absence and the presence of DmH1 (Fig. 5b). A time-dependent MNase digestion of the histone DmH1 associated, reconstituted chromatin can be seen in Supplementary Figure 4. Apparent NRL of Drosophila chromatin with DmH1 was estimated to be 175 ± 2 bp, which is approximately 23 bp longer than the chromatin without DmH1 (Fig. 3c). Thus, the linker histone H1 incorporation was thought to be achieved in this method.
In this study, both Drosophila and human core histones, and the protein factors that are essential to the chromatin assembly in vitro were successfully synthesized by the wheat cell-free protein translation (Fig. 1). As was shown in a framework of our method in Fig. 2, both Drosophila and human chromatins were in vitro reconstituted (Figs. 3 and 4). Although we developed a new method to reconstitute both Drosophila and human chromatins in a co-expression manner, there are distinct differences between the two systems. Between the two systems, different ratios of a pair of H2A/H2B and H3/H4 mRNAs are needed to be used in the reactions, and also reconstitution time was longer in the human chromatin than the Drosophila chromatin. We initially assumed that the two systems are comparable since the amino acid sequences of histone proteins are highly conserved between two species. However, the amount of core histone products between Drosophila and human by the wheat germ cell-free synthesis are quite different (Fig. 1). Moreover, the productivities among core histones were different from each other, i.e., more DmH3/DmH4 were produced than the DmH2A/DmH2B; more HsH2A/HsH2B/HsH3.1 were synthesized than the HsH4. Although, in general, the wheat germ cell-free protein synthesis does not require codon optimization, our result indicated that the codon usage of mRNAs encoding Drosophila and human histones affects the wheat protein synthesis rate . Consistent with this notion, different ratios of two pairs of histones H2A/H2B and H3/H4 mRNAs were optimized between Drosophila and human chromatin assembly reactions. The Drosophila chromatin assembly was optimized at around 1.5:1 to 2:1 (DmH2A/DmH2B:DmH3/DmH4) ratio (Fig. 3a), while the ratio was 1:1.5 to 1:2 (HsH2A/HsH2B:HsH3.1/HsH4) for human (Fig. 4a). We concluded that the differences found between Drosophila and human chromatin assembly systems mainly result from the fitness of the codon-usages in the wheat cell-free protein synthesis platform.
Additionally, we speculated that the different chromatin assembly factors used in the Drosophila and human chromatin might affect the time of chromatin reconstitution. The Drosophila chromatin was reconstituted by using the well-documented chromatin assembly system, which employs a combination of the Drosophila ATP-utilizing assembly factor (dAcf1 and dISWI) and nucleosome assembly protein (dNAP1). Consistent with the previous studies, the Drosophila chromatin in our system was completed within 4 h. While, the combination of human core histones, Drosophila nucleoplasmin (dNLP), and dISWI was used in the human chromatin assembly, and the optimum reaction time was determined to be 6 h. Preeminently histone H3s and H4s, each of which differ only one amino acid between Drosophila and human (Fig. S3a and b), while the protein sequences between DmH2A and HsH2A of 84.6% similarity (110/130AA), and DmH2B and HsH2B of 78.6% similarity (99/126 AA) (Fig. S3c and d). Particularly, the first 30 amino acids from the N-terminus of DmH2B and HsH2B are highly variable, and only 9 amino acids are conserved (Fig. S3d). In the previous studies, an ortholog of dNLP in Xenopus oocytes, eNP, was shown to interact with Xenopus histone H2A/H2B dimer, H3/H4 dimer or tetramer, and octamer prior to the incorporation of octamers into nucleosomes, and this process was suggested to occur sequentially in the nuclei [49, 50]. Thus, we think that different histone sequences between Drosophila and human histones H2As and H2Bs affect the sequential formation of human histone octamer, and so nucleosome assembly mediated by dNLP. This finding is not a concern in the reported human nucleosome reconstitution method, which utilizes the dISWI and the pre-reconstituted dNLP-histone octamer complex, hence dNLP would only interact with the pre-reconstituted octamer before assembly .
Finally, we performed the chromatin and linker histone H1 co-assembly reaction to prove that the chromatins assembled in this study can be utilized for downstream applications. Drosophila chromatin was reconstituted in the presence of the premixed mRNAs encoding four core histones and linker histone, and other necessary factors used in the co-expression chromatin assembly reaction (Fig. 5). The assembled Drosophila chromatin in the presence of DmH1 showed longer NRLs than the chromatin without linker histone assessed by MNase assay (Fig. 5b and Fig. S4). Thus, the reconstituted chromatin is thought to be useful for downstream applications. Such downstream applications may involve epigenetic enzyme screening, including acetyltransferases, methyltransferases, and others, and ultimately in vitro reconstitution of the currently unavailable protein-chromatin complex such as heterochromatin reconstitution, can be achieved.
The most significant advantage of this method compared to other conventional chromatin assembly methods is that chromatin dynamics coop with other proteins/enzymes that can be reconstituted since the entire procedure is in one tube. In the conventional methods, a set of core histones is prepared before chromatin assembly reaction in either a salt dialysis method [16,17,18] or ATP-dependent chromatin assembly reactions [23,24,25,26,27,28,29]. In contrast, our method can provide a streamline of translation of core histones (and histone H1), chromatin assembly factors, and likely other chromatin-associated proteins in a reaction. Thus, unlike conventional methods, our method can be well suited to study chromatin dynamics.
In this study, we report a novel in vitro co-expression chromatin assembly method by utilizing Drosophila and human chromatin systems (Figs. 1 and 2). All the histone proteins and chromatin assembly factors were expressed by in vitro wheat germ cell-free protein synthesis (Fig. 1). The mRNAs encoding Drosophila core histones, DmH2A, DmH2B, DmH3, and DmH4, and Drosophila chromatin assembly factors were co-translated with the circular plasmid DNA, the reaction was optimized, and assessed by DNA supercoiling and MNase assays (Fig. 3). Analogously, the four human core histones, HsH2A, HsH2B, HsH3.1, and HsH4, and Drosophila chromatin assembly factors, dISWI, and dNLP were co-translated and assembled on the circular plasmid, optimized, then subjected to supercoiling and MNase assays (Fig. 4). Several surprising differences were observed between Drosophila and human chromatin assembly reaction, such as the ratio of the input mRNAs encoding core histones and reconstitution time. We discussed multiple possibilities related to the amino acid sequences between Drosophila and human histones (Fig. S3) and the codon usages between two species that may explain the observed differences between the two systems. At last, histone H1-containing Drosophila chromatin was reconstituted successfully (Fig. 5), which indicates a potential usage for downstream applications .
Conventional methods typically carry out in vitro chromatin assembly in two-steps, which allows the equimolar formation of histone octamer prior to the assembly, thus the reconstitution reaction may only rely on the activity of ATP-dependent chromatin remodeling factor, and nucleosome assembly factors. In contrast, our method let protein synthesis and chromatin assembly concomitantly, which makes this method fundamentally distinct from conventional methods.
In summary, the described method presents a quick, convenient, and perhaps near-physiological tool for chromatin reconstitution of both Drosophila and human, providing a straightforward approach to future chromatin research, including chromatin formation, chromatin epigenetics, and epigenetic drug studies.
General reagents used in cDNA synthesis (Nippon Genetics), cloning (Toyobo), in vitro transcription (Promega), protein expression, including wheat germ extract (WEPRO7240H Lot: 15AQ02, CellFree Sciences) and SUB-AMIX translation buffer (CellFree Sciences), and creatine kinase (Roche Diagnostics, GmbH) were purchased. Reagents used in chromatin assembly reaction, including pBluescript II SK plasmid DNA (Addgene), SUB-AMIX solution (CellFree Sciences), creatine kinase (Roche Diagnostics, GmbH), and Topoisomerase I (Takara Bio Inc.) were also purchased. For gel analyses,100 bp DNA molecular weight marker (Toyobo) and protein size marker (Bio-Rad Laboratories) were purchased.
Total RNA extracts of human culture Jurkat cell line (RCB3052, RIKEN BioResource Research Center) were a kind gift of Ryotah Uehara (Hokkaido University) and total RNA extracts of adult Drosophila were prepared by using FastGeneTM kit (Nippon Genetics). cDNA libraries were synthesized by using 100 ng total RNA and with random 6-mer primer with PrimeScript II (Takara Bio Inc) by following the manufacturer protocol.
Genes encoding Drosophila core histones, DmH2A (UniProt ID: P84051), DmH2B (UniProt ID: P02283), DmH3 (UniProt ID: P02299), and DmH4 (UniProt ID: P84040), linker histone H1 (UniProt ID: P02255) and Drosophila chromatin assembly factors dAcf1 (UniProt ID: Q9V9T4), dISWI (UniProt ID: Q24368), and dNAP1 (UniProt ID: Q9W1G7) were a kind gift from Prof. Kadonaga (UC San Diego, USA). Genes encoding human core histones HsH2A (UniProt ID: Q6FI13), HsH2B (UniProt ID: P62807), HsH3.1 (UniProt ID: P68431), and HsH4 (UniProt ID: P62805), and Drosophila chromatin assembly factors dNLP (UniProt ID: Q27415) were amplified from human and Drosophila cDNA libraries, respectively. Genes of Drosophila core histones and chromatin assembly factors were cloned into a pEU-E01-MCS expression vector (CellFree Sciences) by PIPE-cloning . Genes of human core histones were inserted into the pEU-E01-LICNot vector by ligation-independent cloning . The pEU-E01-LICNot, the affinity tag-free version of the vector was generated by the elimination of His6-tag by PCR mediated deletion  with the usage of the following primers 5′-TATTGGATTGGAAGTAACTAGTGATATCTTGGTGA-3′ and 5′- CCAAGATATCACTAGTTACTTCCAATCCAATATTG-3′.
Proteomic analysis of the wheat germ cell-free extract
The sample preparation and proteomic analysis were performed by following the previous study . Briefly, 10 μg equivalent of the wheat germ cell-free extract (WEPRO7240H Lot: 15AQ02, CellFree Sciences) was precipitated by 20% (vol/vol) trichloroacetate (Wako Pure Chemical Corporation), and incubated for 20 min on ice, followed by ice-cold acetone wash for two times. The pellet was resuspended in 10.0 μl of 8 M urea, then 70 μl 25 mM ammonium bicarbonate (Wako Pure Chemical Corporation) was added. The reduction and alkylation reactions were performed by adding 5 mM DTT (Wako Pure Chemical Corporation) for 30 min at 50 °C, and 15 mM iodoacetamide (Wako Pure Chemical Corporation) for 30 min at 25 °C in the dark, respectively. Tryptic digestion was performed by adding 0.5 μg of proteomic grade trypsin (Roche Diagnostics, GmbH), and incubated for 4 h at 37 °C. The trypsin-digested peptides were separated by using a nanoLC1000 (Thermofisher Scientific) hooked up with a C18 column (NTCC-360/75–3-125; Nikkyo Technos) connected to a hybrid linear ion trap-orbitrap mass spectrometer (Q-Exactive Plus; ThermoFisher Scientific) and operated by using an Xcalibur software v3.1 (Thermofisher Scientific). Peptide fragments were separated by a linear gradient rased from 5 to 30% acetonitrile in 0.1% formic acid (Fisher Chemical) for 240 min and monitored at a scan range of 300.0 to 20,000 m/z and a resolution of 70,000. Raw MS/MS data were analyzed by using Proteome Discoverer software v1.4 (ThermoFisher Scientific) under the following settings: the peptide mass tolerance was set to 10.0 ppm, and the fragment mass tolerance was set to 0.8 Da. A list of proteins encoded in the Triticum aestivum genome was obtained from the NCBI on April 2014. Fixed modification of carbamidomethyl at cysteine and dynamic modifications of oxidation at methionine were used for the database search. The abundance of each protein was estimated by the Sequest score calculated by the Proteome Discoverer software.
In vitro transcription and translation
The plasmid constructs were transcribed by in vitro transcription according to the previous study [30, 33], briefly, 2.0 μg vector was transcribed for 4 h at 37 °C in 20.0 μl total reaction volume. 6 U RNase-free DNase I (Nippon Gene) was added to remove the plasmid DNA templates. The mRNAs were purified by acidic phenol-chloroform-IAA (pH 4.5) extraction followed by ethanol precipitation, resuspended in 20.0 μl of RNase-free water. The amount of mRNA’s was determined by spectrophotometer at 260 nm. All protein products shown in Fig. 1 and Fig. 5a were translated by a cup dialysis method [31, 42] by mixing 20.0 μl purified individual mRNA, 16.7 μl wheat germ extract, 4.0 μg creatine kinase, and 48.0 μl 1x SUB-AMIX solution in a total of 100.0 μl reaction in the dialysis cup (10 K MWCO, Slide-A-Lyzer, Thermofisher Scientific). The mixture was incubated for 72 h at 15 °C with 1.5 ml 1x SUB-AMIX filling the outside of the dialysis cup. Both bilayer and dialysis cup methods yielded approximately 5–10.0 μg target protein per reaction. Then, 1.5 μl each of translation products was mixed with 2x loading buffer (Bio-Rad Laboratories), incubated for 5 min at 95 °C, then analyzed by SDS-PAGE. 18.0% SDS-PAGE gel and Coomassie Blue staining were used for Drosophila and human histone proteins, 10% stain-free SDS-PAGE (Bio-Rad Laboratories) was used for chromatin assembly factors and proteins were visualized by the gel documentation system (Bio-Rad Laboratories). For DmH1, a sample was run on 18% SDS-PAGE followed by Coomassie Blue staining. Expected molecular weights of in vitro translated proteins: Drosophila core histone DmH2A 13.4 kDa, DmH2B 13.7 kDa, DmH3 15.6 kDa, DmH4 11.4 kDa; human core histone HsH2A 14.1 kDa, HsH2B 14.0 kDa, HsH3.1 15.4 kDa, HsH4 11.4 kDa; Drosophila chromatin assembly factors, dAcf1 170.4 kDa, dISWI 118.9 kDa, dNAP1 42.8 kDa, dNLP 17.0 kDa (Table 1). The size of DmH1 on SDS-PAGE was larger than the expected molecular weight of 26.4 kDa, but our observed was consistent with the previous study .
In vitro wheat germ cell-free nucleosome assembly of Drosophila chromatin
The mRNAs of Drosophila core histone DmH2A, DmH2B, DmH3 and DmH4 were mixed pairwise (DmH2A with DmH2B, DmH3 with DmH4) after in vitro transcription, precipitated and resuspend in 10.0 μl of RNase-free water (Nippon Gene). The ratio of appropriate amount core histone mRNAs was determined by testing the ratio of DmH2A/DmH2B and DmH3/DmH4 coding mRNAs from 1:0.5 to 1:2 in total of approximately 2.0 μg/reaction, then a stock mRNA mixture was made, that was used directly for chromatin assembly reaction. The reaction was performed by mixing 1.0 μl of Drosophila core histone mRNA mixture, 0.4 μl dAcf1, 0.4 μl dISWI, 0.4 μl dNAP1 mRNAs, 2.5 μg of supercoiled pBSK plasmid, 2 U of Topoisomerase I, 5.0 μl wheat germ extract, and 0.4 μg of creatine kinase and supplemented to 10.7 μl final volume with 1x SUB-AMIX solution. The mixture was gently underlaid to 103.0 μl of 1x SUB-AMIX solution in a 96-well plate to form bilayer. The reaction was carried out at the indicated time (Fig. 3) at 26 °C. The co-expression reaction of DmH1-containing chromatin assembly was performed by using the ratio of DmH2A/DmH2B:DmH3/DmH4:DmH1 = 1:0.67:0.42 under the same reaction conditions.
In vitro wheat germ cell-free nucleosome assembly of human chromatin
The stock solution of the mRNAs of human core histone HsH2A, HsH2B, HsH3.1 and HsH4 was prepared pairwise as was described in the case of Drosophila core histone mRNAs. The ratio of appropriate amount core histone mRNAs was determined by testing the ratio of HsH2A/HsH2B and HsH3.1/HsH4 coding mRNAs from 1:0.5 to 1: 2 in total of approximately 2.0 μg/reaction, then a stock mRNA mixture was made, and used directly for chromatin assembly reaction. The chromatin assembly reaction was performed by mixing 1.0 μl of human core histone mRNA mixtures, 0.4 μl ISWI, 0.4 μl NLP mRNAs, 2.5 μg of supercoiled pBSK plasmid, 2 U of Topoisomerase I, 5.0 μl wheat germ extract, and 0.4 μg of creatine kinase and supplemented to 10.7 μl final volume with 1x SUB-AMIX solution. The mixture was gently underlaid to 103.0 μl of 1x SUB-AMIX solution in a 96-well plate to form bilayer. The reaction was carried out at the indicated time at 26 °C (Fig. 4).
Fifty-five point zero microliter of the total chromatin assembly reaction mixture was purified by phenol-chloroform-IAA (25:24:1, v/v) extraction (pH 8.0) followed by ethanol precipitation, and the purified DNA was resuspended in HD buffer (25 mM HEPES, 1 mM DTT, pH 7.6) containing a trace amount of Ribonuclease a (Macherey-Nagel GmbH & Co.). Supercoiled plasmid DNAs were separated by 0.8% TBE agarose gel in 0.5x TBE buffer, visualized with ethidium bromide (Nippon Gene), and analyzed by gel documentation system (Bio-Rad Laboratories).
Micrococcal nuclease assay
MNase assay was performed by the addition of Micrococcal Nuclease (Bio-Rad Laboratories) and MNase buffer (20 mM Tris-HCl (pH 8.0), 5 mM NaCl, 2.5 mM CaCl2) to 28.0 μl of total reaction mixture followed by 5, 10, 20, 30, 40 min incubation at 25 °C. The final concentration of MNase for Drosophila chromatin was 14 U/μl and for human chromatin was 10 U/μl. For the DmH1-containing chromatin, 13 U/μl MNase was used. The assay was halted by EGTA, and proteins were eliminated by phenol-chloroform-IAA extraction followed by ethanol precipitation. The purified DNA was resuspended in HD Buffer (25 mM HEPES, 1 mM DTT, pH 7.6) containing a trace amount of Ribonuclease A and analyzed by 2.0% TAE agarose gel in 1x TAE buffer. Gels containing Drosophila DNA were stained with GelRed (Wako Pure Chemical Corporation) and human DNA was stained with ethidium bromide. The average mononucleosomal DNA length measurement was performed by the gel documentation system (Bio-Rad Laboratories).
ATP-dependent chromatin assembly factor large subunit
Chromatin-remodeling complex ATPase chain Iswi
Nucleosome assembly protein NAP-1
Nucleotide repeat length
Polymerase Incomplete Primer Extension
- d and Dm:
van Holde KE. Chromatin. New York: Springer New York; 1989. https://doi.org/10.1007/978-1-4612-3490-6.
Kornberg RD, Lorch Y. Twenty-five years of the nucleosome, fundamental particle of the eukaryote chromosome. Cell. 1999;98:285–94 http://www.ncbi.nlm.nih.gov/pubmed/10458604.
Luger K, Mäder AW, Richmond RK, Sargent DF, Richmond TJ. Crystal structure of the nucleosome core particle at 2.8 A resolution. Nature. 1997;389:251–60. https://doi.org/10.1038/38444.
Davey CA, Sargent DF, Luger K, Maeder AW, Richmond TJ. Solvent mediated interactions in the structure of the nucleosome core particle at 1.9 a resolution. J Mol Biol. 2002;319:1097–113. https://doi.org/10.1016/S0022-2836(02)00386-8.
Shibahara K, Stillman B. Replication-dependent marking of DNA by PCNA facilitates CAF-1-coupled inheritance of chromatin. Cell. 1999;96:575–85. https://doi.org/10.1016/S0092-8674(00)80661-3.
Almouzni G, Cedar H. Maintenance of epigenetic information. Cold Spring Harb Perspect Biol. 2016;8:a019372. https://doi.org/10.1101/cshperspect.a019372.
Dabin J, Fortuny A, Polo SE. Epigenome maintenance in response to DNA damage. Mol Cell. 2016;62:712–27. https://doi.org/10.1016/j.molcel.2016.04.006.
Zhu B, Chen S, Wang H, Yin C, Han C, Peng C, Liu Z, Wan L, Zhang X, Zhang J, Lian CG, Ma P, Xu Z, Prince S, Wang T, Gao X, Shi Y, Liu D, Liu M, Wei W, Wei Z, Pan J, Wang Y, Xuan Z, Hess J, Hayward NK, Goding CR, Chen X, Zhou J, Cui R. The protective role of DOT1L in UV-induced melanomagenesis. Nat Commun. 2018;9:259. https://doi.org/10.1038/s41467-017-02687-7.
Rice JC, Allis CD. Histone methylation versus histone acetylation: new insights into epigenetic regulation. Curr Opin Cell Biol. 2001;13:263–73. https://doi.org/10.1016/S0955-0674(00)00208-8.
Segal E, Fondufe-Mittendorf Y, Chen L, Thåström A, Field Y, Moore IK, Wang J-PZ, Widom J. A genomic code for nucleosome positioning. Nature. 2006;442:772–8. https://doi.org/10.1038/nature04979.
Schmidl C, Rendeiro AF, Sheffield NC, Bock C. ChIPmentation: fast, robust, low-input ChIP-seq for histones and transcription factors. Nat Methods. 2015;12:963–5. https://doi.org/10.1038/nmeth.3542.
Stewart-Morgan KR, Petryk N, Groth A. Chromatin replication and epigenetic cell memory. Nat Cell Biol. 2020;22:361–71. https://doi.org/10.1038/s41556-020-0487-y.
Heard E, Martienssen RA. Transgenerational epigenetic inheritance: myths and mechanisms. Cell. 2014;157:95–109. https://doi.org/10.1016/j.cell.2014.02.045.
Zhou K, Gaullier G, Luger K. Nucleosome structure and dynamics are coming of age. Nat Struct Mol Biol. 2019;26:3–13. https://doi.org/10.1038/s41594-018-0166-x.
Song F, Chen P, Sun D, Wang M, Dong L, Liang D, Xu R-M, Zhu P, Li G. Cryo-EM study of the chromatin fiber reveals a double helix twisted by tetranucleosomal units. Science. 2014;344:376–80. https://doi.org/10.1126/science.1251413.
Stein A. Reconstitution of chromatin from purified components. Methods Enzymol. 1989;170:585–603 http://www.ncbi.nlm.nih.gov/pubmed/2770553.
Lowary PT, Widom J. New DNA sequence rules for high affinity binding to histone octamer and sequence-directed nucleosome positioning. J Mol Biol. 1998;276:19–42. https://doi.org/10.1006/jmbi.1997.1494.
Takasuka TE, Stein A. Direct measurements of the nucleosome-forming preferences of periodic DNA motifs challenge established models. Nucleic Acids Res. 2010;38:5672–80. https://doi.org/10.1093/nar/gkq279.
Shogren-Knaak M, Ishii H, Sun J-M, Pazin MJ, Davie JR, Peterson CL. Histone H4-K16 acetylation controls chromatin structure and protein interactions. Science. 311(2006):844–7. https://doi.org/10.1126/science.1124000.
Shimko JC, North JA, Bruns AN, Poirier MG, Ottesen JJ. Preparation of fully synthetic histone H3 reveals that acetyl-lysine 56 facilitates protein binding within nucleosomes. J Mol Biol. 2011;408:187–204. https://doi.org/10.1016/j.jmb.2011.01.003.
Fierz B. Synthetic chromatin approaches to probe the writing and erasing of histone modifications. ChemMedChem. 2014;9:495–504. https://doi.org/10.1002/cmdc.201300487.
Fierz B, Muir TW. Chromatin as an expansive canvas for chemical biology. Nat Chem Biol. 2012;8:417–27. https://doi.org/10.1038/nchembio.938.
Becker PB, Wu C. Cell-free system for assembly of transcriptionally repressed chromatin from Drosophila embryos. Mol Cell Biol. 1992;12:2241–9. https://doi.org/10.1128/mcb.12.5.2241.
Ito T, Tyler JK, Kadonaga JT. Chromatin assembly factors: a dual function in nucleosome formation and mobilization? Genes Cells. 1997;2:593–600 http://www.ncbi.nlm.nih.gov/pubmed/9427281.
Ito T, Levenstein ME, Fyodorov DV, Kutach AK, Kobayashi R, Kadonaga JT. ACF consists of two subunits, Acf1 and ISWI, that function cooperatively in the ATP-dependent catalysis of chromatin assembly. Genes Dev. 1999;13:1529–39 http://www.ncbi.nlm.nih.gov/pubmed/10385622.
Fyodorov DV, Kadonaga JT. Chromatin assembly in vitro with purified recombinant ACF and NAP-1. Methods Enzymol. 2003;371:499–515. https://doi.org/10.1016/S0076-6879(03)71037-4.
Glikin GC, Ruberti I, Worcel A. Chromatin assembly in Xenopus oocytes: in vitro studies. Cell. 1984;37:33–41. https://doi.org/10.1016/0092-8674(84)90298-8.
Fyodorov DV, Levenstein ME. Chromatin assembly using Drosophila systems. Curr Protoc Mol Biol. Chapter 21 (2002) Unit 21.7. https://doi.org/10.1002/0471142727.mb2107s58..
Khuong MT, Fei J, Cruz-Becerra G, Kadonaga JT. A simple and versatile system for the ATP-dependent assembly of chromatin. J Biol Chem. 2017;292:19478–90. https://doi.org/10.1074/jbc.M117.815365.
Madin K, Sawasaki T, Ogasawara T, Endo Y. A highly efficient and robust cell-free protein synthesis system prepared from wheat embryos: plants apparently contain a suicide system directed at ribosomes. Proc Natl Acad Sci U S A. 2000;97:559–64 http://www.ncbi.nlm.nih.gov/pubmed/10639118.
Endo Y, Sawasaki T. Cell-free expression systems for eukaryotic protein production. Curr Opin Biotechnol. 2006;17:373–80. https://doi.org/10.1016/j.copbio.2006.06.009.
Kanno T, Kitano M, Kato R, Omori A, Endo Y, Tozawa Y. Sequence specificity and efficiency of protein N-terminal methionine elimination in wheat-embryo cell-free system. Protein Expr Purif. 2007;52:59–65. https://doi.org/10.1016/j.pep.2006.09.007.
Sawasaki T, Ogasawara T, Morishita R, Endo Y. A cell-free protein synthesis system for high-throughput proteomics. Proc Natl Acad Sci U S A. 2002;99:14652–7. https://doi.org/10.1073/pnas.232580399.
Nagy SK, Darula Z, Kállai BM, Bögre L, Bánhegyi G, Medzihradszky KF, Horváth GV, Mészáros T. Activation of AtMPK9 through autophosphorylation that makes it independent of the canonical MAPK cascades. Biochem J. 2015;467:167–75. https://doi.org/10.1042/BJ20141176.
Kohoutová L, Kourová H, Nagy SK, Volc J, Halada P, Mészáros T, Meskiene I, Bögre L, Binarová P. The Arabidopsis mitogen-activated protein kinase 6 is associated with γ-tubulin on microtubules, phosphorylates EB1c and maintains spindle orientation under nitrosative stress. New Phytol. 2015;207:1061–74. https://doi.org/10.1111/nph.13501.
Horvath BM, Kourova H, Nagy S, Nemeth E, Magyar Z, Papdi C, Ahmad Z, Sanchez-Perez GF, Perilli S, Blilou I, Pettkó-Szandtner A, Darula Z, Meszaros T, Binarova P, Bogre L, Scheres B. Arabidopsis RETINOBLASTOMA RELATED directly regulates DNA damage responses through functions beyond cell cycle control. EMBO J. 2017;36:1261–78. https://doi.org/10.15252/embj.201694561.
Bianchetti CM, Takasuka TE, Deutsch S, Udell HS, Yik EJ, Bergeman LF, Fox BG. Active site and laminarin binding in glycoside hydrolase family 55. J Biol Chem. 2015;290:11819–32. https://doi.org/10.1074/jbc.M114.623579.
Glasgow EM, Vander Meulen KA, Takasuka TE, Bianchetti CM, Bergeman LF, Deutsch S, Fox BG. Extent and origins of functional diversity in a subfamily of glycoside hydrolases. J Mol Biol. 2019;431:1217–33. https://doi.org/10.1016/j.jmb.2019.01.024.
Goshima N, Kawamura Y, Fukumoto A, Miura A, Honma R, Satoh R, Wakamatsu A, Yamamoto J, Kimura K, Nishikawa T, Andoh T, Iida Y, Ishikawa K, Ito E, Kagawa N, Kaminaga C, Kanehori K, Kawakami B, Kenmochi K, Kimura R, Kobayashi M, Kuroita T, Kuwayama H, Maruyama Y, Matsuo K, Minami K, Mitsubori M, Mori M, Morishita R, Murase A, Nishikawa A, Nishikawa S, Okamoto T, Sakagami N, Sakamoto Y, Sasaki Y, Seki T, Sono S, Sugiyama A, Sumiya T, Takayama T, Takayama Y, Takeda H, Togashi T, Yahata K, Yamada H, Yanagisawa Y, Endo Y, Imamoto F, Kisu Y, Tanaka S, Isogai T, Imai J, Watanabe S, Nomura N. Human protein factory for converting the transcriptome into an in vitro-expressed proteome. Nat Methods. 2008;5:1011–7. https://doi.org/10.1038/nmeth.1273.
Klock HE, Lesley SA. The Polymerase Incomplete Primer Extension (PIPE) method applied to high-throughput cloning and site-directed mutagenesis. Methods Mol Biol. 2009;498:91–103. https://doi.org/10.1007/978-1-59745-196-3_6.
Nagy SK, Kállai BM, András J, Mészáros T. A novel family of expression vectors with multiple affinity tags for wheat germ cell-free protein expression. BMC Biotechnol. 2020;20:17. https://doi.org/10.1186/s12896-020-00610-5.
Takai K, Sawasaki T, Endo Y. Practical cell-free protein synthesis system using purified wheat embryos. Nat Protoc. 2010;5:227–38. https://doi.org/10.1038/nprot.2009.207.
Schultz MC, Hockman DJ, Harkness TA, Garinther WI, Altheim BA. Chromatin assembly in a yeast whole-cell extract. Proc Natl Acad Sci U S A. 1997;94:9034–9 http://www.ncbi.nlm.nih.gov/pubmed/9256430.
Schnitzler GR. Isolation of histones and nucleosome cores from mammalian cells. CurrProtoc Mol Biol. Chapter 21 (2001) Unit 21.5. https://doi.org/10.1002/0471142727.mb2105s50.
Torigoe SE, Urwin DL, Ishii H, Smith DE, Kadonaga JT. Identification of a rapidly formed nonnucleosomal histone-DNA intermediate that is converted into chromatin by ACF. Mol Cell. 2011;43:638–48. https://doi.org/10.1016/j.molcel.2011.07.017.
Germond JE, Hirt B, Oudet P, Gross-Bellark M, Chambon P. Folding of the DNA double helix in chromatin-like structures from simian virus 40. Proc Natl Acad Sci U S A. 1975;72:1843–7 http://www.ncbi.nlm.nih.gov/pubmed/168578.
Simpson RT, Thoma F, Brubaker JM. Chromatin reconstituted from tandemly repeated cloned DNA fragments and core histones: a model system for study of higher order structure. Cell. 1985;42:799–808. https://doi.org/10.1016/0092-8674(85)90276-4.
Harbers M. Wheat germ systems for cell-free protein expression. FEBS Lett. 2014;588:2762–73. https://doi.org/10.1016/j.febslet.2014.05.061.
Ramos I, Martín-Benito J, Finn R, Bretaña L, Aloria K, Arizmendi JM, Ausió J, Muga A, Valpuesta JM, Prado A. Nucleoplasmin binds histone H2A-H2B dimers through its distal face. J Biol Chem. 2010;285:33771–8. https://doi.org/10.1074/jbc.M110.150664.
Franco A, Arranz R, Fernández-Rivero N, Velázquez-Campoy A, Martín-Benito J, Segura J, Prado A, Valpuesta JM, Muga A. Structural insights into the ability of nucleoplasmin to assemble and chaperone histone octamers for DNA deposition. Sci Rep. 2019;9:9487. https://doi.org/10.1038/s41598-019-45726-7.
Lusser A, Kadonaga JT. Strategies for the reconstitution of chromatin. Nat Methods. 2004;1:19–26. https://doi.org/10.1038/nmeth709.
Bardóczy V, Géczi V, Sawasaki T, Endo Y, Mészáros T. A set of ligation-independent in vitro translation vectors for eukaryotic protein production. BMC Biotechnol. 2008;8. https://doi.org/10.1186/1472-6750-8-32.
Hansson MD, Rzeznicka K, Rosenbäck M, Hansson M, Sirijovski N. PCR-mediated deletion of plasmid DNA. Anal Biochem. 2008;375:373–5. https://doi.org/10.1016/j.ab.2007.12.005.
Hori C, Song R, Matsumoto K, Matsumoto R, Minkoff BB, Oita S, Hara H, Takasuka TE. Proteomic characterization of lignocellulolytic enzymes secreted by the insect-associated fungus, Daldinia decipiens oita, isolated from the forest in northern Japan. Appl Environ Microbiol. 2020. https://doi.org/10.1128/AEM.02350-19.
We thank Prof. James Kadonaga who provided us a set of chromatin assembly factors, dAcf1, dISWI, and dNAP1 coding genes. We also thank Profs. Ryota Uehara and Nobuaki Tanaka, Faculty of Science, Hokkaido University, for providing total RNA extract from human cell line for cDNA production and Drosophila adults for the total RNA extraction, respectively. We thank Dr. Ryo Morishita and Riho Suzuki for technical assistance.
This study was supported by SKN’s 129083 grant of the National Research, Development and Innovation Office, Hungary and partially supported by the funding of the Graduate School of Global Food Resources, Hokkaido University. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
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Supplementary Table S1. Protein list of mass spectrometry analysis of the wheat germ extract. Results of proteins determined in the wheat germ cell-free extract (WEPRO7240H). Seven hundred forty-four proteins were identified in the total of 61,984 protein sequences listed in the FASTA file. The score indicated the enrichment of proteins calculated by the Proteome Discoverer.
Supplementary Figure S1. Full scans of gel images shown in Fig. 3a and b. a A full gel image of determination of the appropriate ratio of DmH2A/DmH2B and DmH3/DmH4 mRNAs in the Drosophila chromatin reconstitution reaction shown in Fig. 3a. Supercoiling assay was performed, samples were analyzed by 0.8% agarose TBE gel. Relaxed, linear, and supercoiled plasmid DNAs are indicated as RC, L, and SC, respectively. b Supercoiling assay of assembled Drosophila chromatin under the indicated reaction time 0, 1, 4, and 6 h, where 0 indicated the reconstitution reaction in the absence of mRNAs encoding histones shown in Fig. 3b. Supercoiling assay was performed, samples were analyzed by 0.8% agarose TBE gel. Mr and pBSK indicate 1000 bp DNA molecular marker, and the supercoiled plasmid control, respectively. Supplementary Figure S2. Full scans of gel images shown in Fig. 4a and b. a A full gel image of DNA supercoiling assay to optimize the ratio of HsH2A/HsH2B and HsH3.1/HsH4 mRNAs in the chromatin reconstitution reaction for 4 h shown in Fig. 4a. b Supercoiling assay of assembled human chromatin. Incubation time indicated with 0, 1, 4, 6, and 8 h, where 0 indicated the reconstitution reaction in the absence of mRNAs encoding histones, which is shown in Fig. 4b. Supercoils were analyzed by 0.8% agarose TBE gel. Relaxed, linear, and supercoiled DNA are indicated as RC, L, and SC, respectively. Mr and pBSK indicate 1000 bp DNA molecular marker, and the supercoiled plasmid control, respectively. Supplementary Figure S3. Sequence alignment of Drosophila and human histones. Amino acid sequence alignment of a DmH3 and HsH3.1, b DmH4 and HsH4, c DmH2A and HsH3.1, d DmH2B and HsH2B are shown, respectively. Asterisks and light purple-highlighted amino acids showed the identical amino acid sequence between two species. Supplementary Figure S4. Time course of MNase digestion for the reconstituted Drosophila chromatosome. Assembled DmH1-incorporated chromatin was digested by 10 U/μl MNase for 0, 5, 10,20, 30, 40 min, then run on 2.0% agarose gel and visualized by ethidium bromide. Detected bands corresponding to mono-, di-, and tri-nucleosomes were indicated. NRL of reconstituted chromatosome was estimated to be 174.6 ± 2.1 bp.
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Okimune, Ki., Nagy, S.K., Hataya, S. et al. Reconstitution of Drosophila and human chromatins by wheat germ cell-free co-expression system. BMC Biotechnol 20, 62 (2020). https://doi.org/10.1186/s12896-020-00655-6
- In vitro chromatin assembly
- Wheat germ cell-free protein expression
- Co-expression chromatin assembly
- Drosophila chromatin
- Human chromatin