Genome editing is crucial for genetic engineering of organisms for improved traits, particularly in microalgae due to the urgent necessity for the next generation biofuel production. The most advanced CRISPR/Cas9 system is simple, efficient and accurate in some organisms; however, it has proven extremely difficult in microalgae including the model alga Chlamydomonas. We solved this problem by delivering Cas9 ribonucleoproteins (RNPs) comprising the Cas9 protein and sgRNAs to avoid cytotoxicity and off-targeting associated with vector-driven expression of Cas9. We obtained CRISPR/Cas9-induced mutations at three loci including MAA7, CpSRP43 and ChlM, and targeted mutagenic efficiency was improved up to 100 fold compared to the first report of transgenic Cas9-induced mutagenesis. Interestingly, we found that unrelated vectors used for the selection purpose were predominantly integrated at the Cas9 cut site, indicative of NHEJ-mediated knock-in events. As expected with Cas9 RNPs, no off-targeting was found in one of the mutagenic screens. In conclusion, we improved the knockout efficiency by using Cas9 RNPs, which opens great opportunities not only for biological research but also industrial applications in Chlamydomonas and other microalgae. Findings of the NHEJ-mediated knock-in events will allow applications of the CRISPR/Cas9 system in microalgae, including “safe harboring” techniques shown in other organisms.
Microalgae have emerged as the third generation biofuel feedstocks that are excellent renewable and sustainable energy sources for the future. Their use would allow us to replace the current fossil fuels that have been blamed for serious environmental problems, including pollution and global warming1. Microalgae have many advantages over the previous generations of biofuel feedstocks: they have much higher photosynthetic productivity, require less land, may not compete with food sources, and can generate more value-added products2. However, microalgal biofuels are currently impractical due to their high production costs. This can be partly solved by genetic improvements of microalgal strains to produce more biomass and/or lipids that can be converted to biofuels.
The green unicellular flagellate alga, Chlamydomonas reinhardtii, is a good model organism, with genetic, molecular and genomic resources available for both research fields of basic and applied sciences. Numerous techniques have been used to transform the nucleus, chloroplast and mitochondria of this microalga3,4,5, allowing genetic improvements of traits for various purposes. These advanced resources and techniques have been applied to other microalgae for more practical purposes: for example, transformation techniques have been used to improve production of biomass and/or biofuels in industrial microalgae by overexpression of certain metabolic or regulatory genes6,7. However, a remaining challenge in the genetic engineering of microalgae is the need for efficient methods to specifically knock-down or knockout unwanted genes.
Targeting specific genes for down-regulation or disruption has been well established in many organisms8,9,10,11,12. In microalgae, genes can be down-regulated by RNA silencing techniques involving RNA interference (RNAi) or artificial microRNAs (amiRNA)13,14,15,16,17. These techniques can be used to study essential genes, for which recessive mutations are lethal, particularly in haploid microalgae; however, these methods are often limited by low efficiency, non-specific targeting and silencing of the RNA constructs9,18. Stable and permanent disruption of unwanted genes can be achieved by homologous recombination (HR), and by sequence-specific recombinant nucleases including zinc-finger nuclease (ZFN) and transcription activator-like effector nuclease (TALEN)11,12. In some microalgae, only a few reports have described the specific disruption of genes via HR19,20 and ZFN- or TALEN-based knockout21,22,23; however, these techniques are very hard to achieve in most microalgae.
Recently, a new system based on components of the clustered regularly interspaced short palindromic repeats (CRISPR)/CRISPR associated protein 9 (Cas9), has become very popular in disrupting a gene due to its simplicity, improved specificity and higher versatility compared to ZFN and TALEN24,25. The CRISPR/Cas9 system was initially identified as a bacterial adaptive immune system against invading plasmids and viral DNAs, where the system was found to cleave target DNAs guided by small RNAs24,26. Since the introduction of CRISPR/Cas9 for heterologous genome editing27, a plethora of studies have used CRISPR/Cas9 to knockout targeted genes28. However, it has proven difficult to use this system for genome editing in microalgae. Only one such report exists for Chlamydomonas, and extremely low targeting efficiency was observed, possibly reflecting toxicity induced by vector-driven Cas9 expression29.
In this study, we improved the targeting efficiency of CRISPR/Cas9 in Chlamydomonas by directly delivering the Cas9 protein and single-chain guide RNAs (sgRNAs), known as Cas9 ribonucleoprotein (RNP), which has been successfully tested in other organisms28,30,31. We targeted three genes: the MAA7 gene that encodes the beta subunit of tryptophan synthase (TSB); the antennal assembly gene CpSRP43 that encodes chloroplast SRP43; and the chlorophyll biosynthetic gene ChlM that encodes Mg-protoporphyrin IX S-adenosyl methionine O-methyl transferase. Mutations of MAA7 can be positively selected using 5-fluoroindole (5-FI)32,33, while mutations of cpsrp43 and chlm can be selected by a lighter colony color due to reduced antenna size and chlorophyll synthesis, respectively34,35. For the latter two genes, we employed co-transformation of vectors that confer resistance to hygromycin due to low delivery efficiency in Chlamydomonas. Interestingly, the vectors used in our mutagenic screen were found to be integrated at the Cas9 cut site, indicating that the knock-in mutations were mediated by non-homologous end joining (NHEJ). In summary, we obtained many auxotrophic and visible colonies from the primary screen, and succeeded in obtaining sizable number of mutations targeted at the Cas9 cut sites.
Design of sgRNAs and in vitro assessment of the Cas9 activity
To avoid the probable problems of toxicity29 and off-targeting30 that have been associated with vector-driven expression of the guide RNA and Cas9, we used synthetic sgRNAs and the Cas9 protein manufactured by ToolGen, Inc. (Republic of Korea)30 instead of cloning their genes in a vector. The sgRNAs for the individual target genes were designed to maximize the generation of mutations, as described in the Methods section as per the manufacturer’s guidelines (ToolGen, Inc., Republic of Korea). Target genes were chosen to facilitate easy selection of mutants. Mutants of the MAA7 gene were identified via tryptophan auxotrophic selection using 5-FI32,33, whereas mutations in CpSRP43 and ChlM were identified by visual selection due to the reduced chlorophyll contents of these mutants34,35.
The activities of the sgRNAs and Cas9 protein were assessed by in vitro reactions using individual genomic fragments containing the Cas9 cut site (Fig. 1). The primers used to amplify the relevant genomic fragments are summarized in Table S1. Figure 1 summarizes the genomic maps, the locations and sequences of the guide RNAs, the protospace adjacent motifs (PAMs) and the Cas9 cut site for MAA7, CpSRP43 and ChlM. We tested two sgRNAs for MAA7 and found that the first (MAA7-1) failed to cleave, while the second (MAA7-2) succeeded in cleaving the genomic DNA target of 783 bp into two fragments of 488 bp and 295 bp (Fig. 1d left panel). The CpSRP43 Cas9 RNP cleaved the 795 bp target DNA into 418 bp and 377 bp fragments, while the ChlM Cas9 RNP cleaved the targets of 1010 bp into 274 bp and 736 bp fragments (Fig. 1d right panels). Consistent with these in vitro results, our later in vivo mutagenic screens failed to isolate any targeted mutations for the MAA7-1 sgRNA (See below, and Table 1).
Small indel mutations found among the MAA7 auxotrophic mutants
In vivo mutagenesis was carried out by electroporating MAA7 Cas9 RNPs into C. reinhardtii CC-124. To optimize the delivery and mutagenic efficiencies, we performed experiments in which the amounts of sgRNA and Cas9 were varied while the mass ratio was kept constant at 4:3, as suggested by ToolGen, Inc. (Table 1). Selection with 5-FI yielded three and 21 tryptophan auxotrophic mutants from experiments performed using the MAA7-1 and MAA7-2 sgRNAs, respectively. The growth of some of these primary auxotrophic mutants on media containing tryptophan and 5-FI is shown in Fig. 2A. A MAA7 RNAi mutant (MAA7 RNAi #33) was used as a reference strain17,36. Our mutant strains all showed comparable tolerances to 5-FI, but were consistently less tolerant than MAA7 RNAi #33 (Fig. 2A). Genomic DNA was amplified using primers M2_F and M2-R (Table S1), and sequencing of the generated fragments revealed that zero and eight targeted mutations had been obtained using the MAA7-1 and MAA7-2 sgRNAs, respectively (Table 1, Fig. 2B). Therefore, as noted above, the MAA7-1 sgRNA failed to cleave the target DNA in vitro and produced no mutations in vivo. It is not clear why we obtained such different outcomes from the two target sites closely located on the same locus. However, our results suggest that it is important to test the compatibility of the sgRNA and Cas9 protein prior to undertaking a laborious mutagenic screen.
Sequencing of the eight targeted mutations revealed an interesting pattern of small indel mutations that involved three base pairs or multiples. This yielded point mutations of only a few amino acids rather than the frameshift mutations commonly found in CRISPR/Cas9-induced mutations in other organisms. Our targeted mutations could be grouped into four types. The main type (found in mutants of MAA7 20-1, 40-1, 40-5, 40-12 and 40-20; mutant designation indicated amount sgRNA followed by a serial number.) was deletion of the CGC next to the Cas9 cut site producing a D54E point mutation and a deletion of A55. For convenience, we defined a conserved motif, RPDAN, flanking the Cas9 cut site (Fig. 2B); it was changed to RPEN in these mutants. The other three mutation types were alteration of the RPDAN motif to RPAN (MAA7 40-22), alteration of the RPDAN motif to RPDN (MAA7 40-6), and a 33 bp insertion at the Cas9 cut site (MAA7 20-10) that changed the RPDAN motif to RPDKWSLCYSESYYAN via insertion of the 11 underlined amino acids.
To assess the significance of the RPDAN motif and validate our CRISPR/Cas9-induced mutagenic screen using 5-FI, we performed additional experiments including phylogenetic analyses of TSB homologs, sequencing of MAA7-associated genes, and complementation of MAA7 mutants. Phylogenetic analyses of TSB homologs from various organisms representing the kingdoms of bacteria, plants and microalgae revealed that the RPDAN motif was a part of a conserved region found in all organisms (Fig. 2C; Fig. S1 for the full alignment; Fig. S2 for the phylogenetic tree). The R52 residue was conserved in plants and microalgae, P53 and D54 were invariable in all studied organisms, and A55 appeared to be conserved in bacteria and microalgae. Bacteria and microalgae that shared conservation of A55 appeared to share aspects of the entire sequence phylogeny, as they grouped together in the phylogenetic tree (Fig. S2). The RPDAN motif is clearly distant from the catalytic site of TSB33. We suggest that it may be involved in the interaction with tryptophan synthase alpha subunit (TSA), based on our structural modeling of TSA and TSB in bacteria (Fig. S3). When we compared the reported bacterial TSA-TSB structures with the amino acid sequence of MAA7, we found that the RPDAN motif was located proximal to the four-stranded β-sheet that is involved in the interaction between TSA and TSB (Fig. S3). Because the interface between the two subunits is crucial for the necessary consecutive enzyme reactions37, we speculate that the mutation-based impairment of interface might reduce the enzyme activity of the protein. To exclude the possibility that this second locus might be involved in the suppression during the auxotrophic selection, we sequenced the genes encoding TSA and TSB in WT and mutants MAA7 20-1, 40-22, 40-6 and 20-10 (representing all four mutation classes). We did not identify any mutations other than those at the Cas9 cut site as shown in Fig. 2B. Alternatively, the RPDAN motif might be involved in other critical functions such as stability of the protein, which may explain the low expression of mutated TSB (Fig. S4c).
Complementation of the MAA7 mutations
We further analyzed the functional significance of the RPDAN motif in vivo by performing complementation analyses. The TSB coding sequences (CDSs) were amplified from WT and the MAA7 20-1 mutant (containing RPEN instead of the RPDAN motif), cloned into the pCr202 vector38 together with sequences encoding the FLAG tag, and transformed into MAA7 RNAi #33 (Fig. S4a). The WT TSB CDS was also transformed into MAA7 20-1 to see if the defective TSB function of this mutant could be complemented by WT TSB. PCR was used to confirm transformation (Fig. S4b), and the expression of the TSB proteins tagged with the FLAG tag was assessed by Western blotting using an anti-FLAG antibody (Fig. S4c). All strains complemented with WT TSB (designated 20 W for the MAA7 20-1 mutant complemented with the WT TSB; RW for MAA7 RNAi #33 transformed with the WT TSB) showed relatively high level of TSB expression. For unknown reasons, strains complemented with the mutagenized TSB CDS from MAA7 20-1 showed relatively lower expression levels.
Complementation was evaluated by analyzing the sensitivity to 5-FI (Fig. 3). All strains used in the complementation assay showed normal growth when cultured in TAP medium supplemented with tryptophan (Fig. 3A). In the presence of 5-FI, MAA7 RNAi #33 transformed with WT TSB showed almost complete complementation when WT TSB expression was high (RW #19), but incomplete complementation when low WT TSB expression was low (RW #13). This dose dependence appears to be reasonable considering that higher level of WT TSB expression can counteract the RNA silencing in MAA7 RNAi #33. WT TSB also completely complemented MAA7 20-1 as shown in 20 W #1 and 20 W #6 (Fig. 3B). This indicates that the defects found in MAA7 20-1 (Fig. 2A) arose solely from the RPEN mutation of the RPDAN motif, since no other mutation was found in the genes encoding TSA or TSB.
The results obtained from complementation with the TSB CDS containing point mutations in the RPDAN motif provide additional evidence for the functional importance of this motif. We transformed MAA7 RNAi #33 with the TSB CDS from MAA7 20-1, which contained the RPEN mutation of the RPDAN motif (designated R20 #58 and R20 #61). Compared to the strains complemented with WT TSB (RW #13 and RW #19), these R20 strains completely failed to complement the RNAi mutation (Fig. 3B), even though the expression of TSB-FLAG in these strains was low (Fig. S4c). Nevertheless, this result suggests that the RPEN mutant protein lacks a significant portion of the WT TSB function. Notably, mutations in the RPDAN motif were weaker than the RNAi knockdown mutation (MAA7 RNAi #33), as their tolerance to 5-FI was lower than that of MAA7 RNAi #33 (Figs 2A and 3B).
NHEJ-mediated knock-in mutations at the CpSRP43 locus
We tested our CRISPR/Cas9 systems for two more genes that affect the chlorophyll contents allowing visual selection of their mutants. Considering the extremely low delivery efficiency of transgenic materials in Chlamydomonas, we co-transformed vectors carrying a selection maker. We were thus able to first select transformed colonies, and then identify mutants by visual selection of lighter green colonies. We targeted CpSRP43 by delivering CpSRP43-specific sgRNA (Fig. 1b,d), Cas9 protein and XbaI-linearized pCr202 vector. Our initial screen yielded 283 colonies that showed resistance to hygromycin; from them, we selected three colonies that stably showed a lighter green coloration. CpSRP43 is involved in antennal protein assembly and its mutations are well known. We obtained two deletion mutants, CC-4561 and CC-456234, from the Chlamydomonas Resource Center, and used these as reference strains. We also included two negative controls: CpSRP43 20-1 was from the same screen but showed a normal green colony color; vec-2 was from a vector-only transformation with no sgRNAs or Cas9, and had a normal green colony color.
Our phenotypic analyses began with a visual assessment in which we loaded the same number of cells to each well of a multi-well plate, and compared their colors (Fig. 4A). Consistent with the colors observed for their colonies, the isolated candidates of cpsrp43 mutants induced by CRISPR/Cas9 (CpSRP43 10-1, 10-2 and 10-3) were light green, similar to the cpsrp43 deletion mutants CC-4561 and CC-4562. In contrast, the WT control, CC-124, and the other negative controls were dark green (Fig. 4A). We further analyzed the chlorophyll contents of these strains, and calculated the ratio of chlorophyll a to chlorophyll b, which is a simple criteria used for reduced antenna mutants39,40. As expected from their lighter green color, the chlorophyll contents of the candidate mutants were low, and their ratios of chlorophyll a to chlorophyll b were higher than 8, similar to the deletion mutants (Fig. 4B). Critically, when Western blotting was performed with an anti-CpSRP43 antibody, our CRISPR/Cas9-induced mutants and the deletion mutants all lacked the CpSRP43 protein with the expected size of 43 kDa (Fig. 4C). These data indicate that CpSRP43 sgRNA and Cas9 successfully induced mutations at the CpSRP43 locus.
The molecular nature of the CRISPR/Cas9-induced mutants was analyzed with PCR using primers SRP43_2F and SRP43_2R (Table S1) with the expected size of 795 bp encompassing the Cas9 cut site. Initially, we failed to detect any amplification of the relatively small fragments with exception of a few fragments that were found to be nonspecific upon sequencing (Fig. 5A top panel). However, all of the transformants contained the vector sequence for the hygromycin resistance gene (Fig. 5B). Repeated PCR experiments using primer pairs spanning different areas of the locus yielded similar results. We thus sequenced their genomes, and found that the vector sequence was integrated at the Cas9 cut site with small insertions of a few nucleotides at either end (Fig. 5C). The insertion was further verified with PCR using different primer pairs (amplifying regions A, B and C) (Fig. 5B). Using optimized PCR conditions, we successfully amplified the whole CpSRP43 locus in the mutants (Fig. 5A bottom panel). Assembly of all sequence information revealed that the vector sequence had been re-organized prior to integration as shown in Fig. 5C. All three mutants contained the same integrated sequence, suggesting that they arose from a single transformation event. We also characterized their integration in the genome by performing the Southern blot, and found that the integration was a single copy insertion with the same size of restriction fragments (Fig. S5A,B).
Off-targeting of the CpSRP43 Cas9 RNP was assessed in our mutagenic screen by using Cas-OFFinder (http://www.rgenome.net/cas-offinder/)41. The guide sequence was searched on the Chlamydomonas reference genome sequence allowing 3 mismatches and 2 bulges, and a total of 404 off-target candidate sites could be identified. Among these, we were able to locate 340 sites on our WT (CC-124) genomic sequence that matched those of the Chlamydomonas reference sequence (CC-503)4. We surveyed these 340 sequences on the genomic sequences of CpSRP43 10-1, 10-2 and 10-3, and confirmed the presence of 333 sites. These sites contained no mutations, suggesting that there were no, or rare, incidences of off-targeting with the CpSRP43 Cas9 RNP. This may be possible because the Cas9 RNP could have been degraded and/or diluted soon after electroporation.
NHEJ-mediated knock-in mutations at the ChlM locus
Finally, we used our optimized CRISPR/Cas9 delivery conditions to mutate another gene, ChlM, involved in chlorophyll biosynthesis35. Vector pCr112 containing the hygromycin resistance marker was co-transformed for selection purpose. We obtained about 6000 initial transformants. From them, we isolated 10 clones that showed yellow or brown colony color, and designated ChlM-3, -4, -9, -10, -11, -17, -19, -21, -22, -24 (Fig. 6). Visual assessment of coloration (Fig. 6a) and measurement of chlorophyll contents (Fig. 6b) revealed that the mutant phenotype was associated with the expected chlorophyll deficiency35. We performed semi-quantitative RT-PCR, and found no detectable expression of ChlM mRNA in the mutants (Fig. 6c). Southern blot analyses were performed to characterize genomic integration patterns after digestion of their genomic DNAs with NcoI that does not cut the vector (Fig. S5c,d). Most of the selected transformants contained a single copy of the vector except for ChlM-4 that contained two copies. Two pairs of clones (ChlM-10 and ChlM-17; ChlM-22 and ChlM-24) showed the same banding patterns, suggesting that they were duplicate clones representing the same integration events. We thus observed at least eight independent integration events, most of which were single-copy integration of the vector.
We further characterized the molecular nature of the CRISPR/Cas9-induced mutations at the ChlM locus (Fig. 7). The initial PCR for the ChlM locus spanning the Cas9 cut site failed to amplify genomic DNA from the isolated mutants. We tested combinations of primers (Table S1) located in the ChlM locus and the vector, and successfully determined the junction sequences for six clones including ChlM-3, -9, -10, -19, -22 and -24 (Fig. 7B–G). All of them showed integration of the vector at the Cas9 cut site, and were characterized by different rearrangements of vector sequences and different small indels next to the Cas9 cut site. ChlM-22 and ChlM-24 showed the same vector sequence, but contained different deletions at the junctions (Fig. 7F,G). Our results indicate that the 10 isolated mutants represent at least nine independent integration events with extensive rearrangements of the vector sequences. Interestingly, the six clones with identified junction sequences were examples of NHEJ-mediated knock-in of the vector, because the vector contained no sequences homologous to the ChlM locus. We failed to identify the integration junction sequences for the remaining four clones; however, ChlM-4, ChlM-11 and ChlM-17 showed the same bands hybridized to both probes of ChlM and aphVII, suggesting that they are also knock-ins of the vector sequence. Only ChlM-21 showed different bands for the ChlM and aphVII probes, suggesting that the integration occurred at a location outside of the ChlM locus. ChlM-21 showed a smaller band for the ChlM probe compared to that of WT, suggesting that it contained a sizable deletion of about 200 bps (Fig. S5c,d). The nature of ChlM-21 has not been analyzed further, even though we speculated that there was a deletion of about 200 bps in the ChlM locus based on the Southern blot (Fig. S5c,d). It should be noted that ChlM-4 contained two copies of vector sequences: one at the ChlM locus and the other at an unknown location, based on the Southern blot (Fig. S5d). These mutations could be categorized into three classes as summarized in Fig. S5e: simple knock-ins (ChlM-3, -9, -10, -11, -17, -19, -22, -24), knock-in plus integration at another location (ChlM-4), and deletion plus integration at other location (ChlM-21).
We successfully generated a sizable number of CRISPR/Cas9-induced mutations at the MAA7, CpSRP43 and ChlM loci by delivering Cas9 RNP. This is a significant improvement over the first report of a CRISPR/Cas9-induced mutation in Chlamydomonas29. This improvement may be attributed to the delivery of the Cas9 RNP, as employed successfully in other organisms28,30,31. Vector-driven expression of Cas9 may be toxic to Chlamydomonas, probably due to the continuous expression29. Delivery of purified Cas9 RNP may have other advantages including technical simplicity and fewer occurrences of off-target events30,42. From the auxotrophic selection of MAA7 mutations, we obtained eight small indel mutations that were specifically induced by the MAA7-2 sgRNA and the Cas9 protein. Occurrence of these targeted mutations was highest when cells were delivered with the highest amount of Cas9 and MAA7-2 sgRNA (Table 1), even though we have not determined optimum conditions that might have to be determined empirically. However, none of the CRISPR/Cas9-induced mutations were frame-shifts; we observed only small indels of three base pairs or multiples. This odd mutation pattern defies a clear explanation, but there are reports of non-random occurrence of mutations induced by CRISPR/Cas9, including the insertion of an A or in-frame deletions43,44,45. The error-prone double strand break (DSB) repair of DNA must be involved in generation of small indel mutations46, and the mechanism of DSB repair in Chlamydomonas might have played a role in the unique pattern of mutations obtained in our mutagenic screen. We also found that the indels generated at the ChlM locus (not counting the vector insertion) tended to be in-frame except for ChlM-24: ChlM-3 and ChlM-22 showed no change; ChlM-9 and ChlM-19 contained in-frame indels. Alternatively, complete loss-of-function mutations could not survive the selection conditions employed in our auxotrophic screens. Even though tryptophan was supplemented in the media, uptake of tryptophan in Chlamydomonas is not known, since no true loss-of-function mutations of TSB have been characterized17,33.
It is interesting to note that the integration of the vector sequences at the Cas9 cut sites of CpSRP43 and ChlM was mediated by NHEJ, since the co-transformed vectors did not contain any sequence from the target genes or the neighboring loci. Knock-in can be achieved by homology-driven recombination (HDR) wherein the vector sequence contains wings of target-flanking sequences, or by NHEJ that does not require any cloning of the wings24,47,48,49,50,51. It is not clear why we obtained predominantly knock-in events. It is possible that DSBs induced by Cas9 facilitated integration of available free ends of co-transformed vectors at the cut site. Our present finding opens up a range of possible applications of NHEJ-mediated knock-in, including insertion of a gene at a specific location without requiring the cloning of homologous sequences.
Conclusively, delivery of Cas9 RNPs improved mutagenic efficiency and specificity of the CRISPR/Cas9 system at the MAA7, CpSRP43 and ChlM loci in Chlamydomonas. The efficiency of obtaining targeted mutations was up to 100 fold improvement compared to the first report of CRISPR/Cas9-induced mutagenesis in Chlamydomonas29. The direct delivery of Cas9 RNPs may have other advantages including minimized off-targeting events, less toxicity of Cas9, and no laborious cloning work compared to the transgenic techniques30. In our mutagenic screen targeting the CpSRP43 locus, sequencing the whole genomes of cpsrp43 mutants revealed no incidences of off-targeting by using Cas-OFFinder41. We also found predominant NHEJ-mediated knock-in events when co-transformed with unrelated vectors used for the selection purpose. New concepts of the targeted transgene integration for stable expression, such as the “safe harbor” technique and other gene manipulations, are already underway in some organisms47,52. This work can be applied not only to biological research in Chlamydomonas, but also to industrial applications of genome editing in other microalgae for large scale production of biofuels and other biomaterials.
Target genes and sgRNA design
We chose target genes based on our ability to identify mutations via auxotrophic or visual means. The MAA7 gene (GenBank accession: XM_001703345) in Chlamydomonas encodes the beta subunit of tryptophan synthase (TSB; XP_001703397), and its mutations can be positively selected using 5-FI32,33. Mutations in the other two tested genes could be selected based on the lighter colony color arising from reduced chlorophyll synthesis34,35. The CpSRP43 gene (GenBank accession: XM_001703652) and ChlM gene (GenBank accession: XM_001702328) encodes chloroplast SRP43 (XP_001703704) and Mg-protoporphyrin IX S-adenosyl methionine O-methyl transferase (XP_001702380), respectively. For the latter two genes, we co-transformed cells with a hygromycin-resistance vector and used antibiotic selection to improve the delivery efficiency in Chlamydomonas.
The sgRNAs were designed by ToolGen, Inc (Republic of Korea) based on the following inclusion criteria: (1) the target site is located within 50% of coding sequence (CDS) from the N terminus; (2) the out-of-frame score is >60; and (3) the mismatch is 2 or greater. The generated sgRNAs included the following guide RNA sequences. For MAA7, MAA7-RG1 (5′-UCGAGCGCUCGCGACGGGA-3′) and MAA7-RG2 (5′-CAUAGCGACCAUUUGCGUCC-3′); for CpSPR43, CpSRP43-RG1 (5′-CGAUUCCGGCCUGCACCGGC-3′); and for ChlM, ChlM-RG1 (5′-CCCGCCCGGCUGUGGCCCGG-3′). Their locations along each locus are shown in Fig. 1a–c. All sgRNAs included the common sequence containing the crRNA, tetraloop (underlined) and tracrRNA: GUUUUAGAGCUAGAAAUAGCAAGUUAAAAUAAGGCUAGUCCGUUAUCAACUUGAAAAAGUGGCACCGAGUCGGUGCUUUUUUU24. The Cas9 protein contained a nuclear localization signal at the C-terminus, of which sequence is PKKKRKV.
Microalgal strains and culture conditions
Chlamydomonas reinhardtii CC-124 was used as the wild type, and was obtained from the Chlamydomonas Resource Center in the University of Minnesota (http://www.chlamycollection.org/). An RNAi knockdown mutant of MAA7 (RNAi #33) was kindly provided by Heriberto Cerutti of Nebraska University-Lincoln17. Mutant strains of CpSRP43 CC-4561 (tla3-Δcpsrp43 cw+ mt+) and CC-4562 (tla3-Δcpsrp43 cw+ mt−) were obtained from the Chlamydomonas Resource Center, and were used as positive controls for our CRISPR/Cas9-induced mutants34. All strains were maintained on Tris-acetate-phosphate (TAP) agar plates [2.42 g/L Tris, 0.375 g/L NH4Cl, 0.1 g/L MgSO4 7H2O, 0.05 g/L CaCl2 2H2O, 0.0108 g/L K2HPO4, 0.0054 g/L KH2PO4, 1 mL/L glacial acetic acid, and 1 mL/L Hutner’s trace elements (50 g/L Na2EDTA 2H2O, 22 g/L ZnSO4 7H2O, 11.4 g/L H3BO3, 5.06 g/L MnCl2 4H2O, 1.61 g/L CoCl2 6H2O, 1.57 g/L CuSO4 5H2O, 1.10 g/L (NH4)6Mo7O24 7H2O, and 4.99 g/L FeSO4 7H2O) at 25 °C under continuous illumination of 50 μmol m−2 s−1.
In vitro digestion of target DNAs with the Cas9 protein
The activities of the sgRNAs and the Cas9 protein were verified in vitro prior to their use in vivo. The DNA targets for this assay were produced by PCR using the Instagene Matrix (Bio-Rad, USA). Briefly, cells were harvested by centrifugation and genomic DNAs were extracted according to the instructions provided with the Instagene Matrix. Substrate DNAs encompassing the Cas9 cut site were amplified using 2Χ EF-Taq PCR Pre-mix (Solgent, Republic of Korea). The utilized primers were as follows: for MAA7, M2_F and M2_R; for CpSRP43, SRP43_2F and SRP43_2R; and for ChlM, CrChlM_F1 and CrChlM_R3 (Table S1). The PCR conditions consisted of 35 cycles of 95 °C for 20 sec, 52–55 °C for 40–60 sec and 72 °C for 1 min. The elongation time was extended to 3 min for the longer amplicon of the CpSRP43 knock-in mutants. The PCR products were purified with a QIAquick Gel Extraction Kit (Qiagen, the Netherlands). For in vitro assays, 500 ng of sgRNA and 600 ng of Cas9 protein were pre-mixed at 37 °C for 5 min. For experiments, 100 ng of PCR amplicons and 3.1 NEB buffer (NEB, USA) were added, and the mixtures were incubated at 37 °C for 2 hours. RNaseA (Bioneer, Republic of Korea) was added, and the mixture was incubated at 37 °C for 20 min. 6× STOP solution (0.5 M EDTA, 80% glycerol, and 10% SDS) was added, and the mixture was incubated 37 °C for 20 min. The final products were separated by 0.8% agarose gel electrophoresis.
Transformation and selection of C. reinhardtii
For transformation of C. reinhardtii, we performed electroporation using a modification of a previously reported protocol53. Cells were cultured under continuous illumination (200 μmol m−2s−1) for 2–3 days to a cell density of 3 × 106 cells/ml. The cells were then concentrated to 3 × 108cells/mL in MAX Efficiency Transformation Reagent for Algae (Thermo Fisher Scientific, USA), and electroporation was conducted using an ECM 830 Square Wave Electroporation System (Bio-Rad, USA) and cuvettes with a 0.2-cm gap (BTX, USA). Prior to electroporation, various amounts of Cas9 and sgRNAs were incubated together at 37 °C for 30 min (Table 1), and cells (300 μL) were placed in the cuvette and cooled on ice for 5 min. To enable visual selection of CpSRP43 and ChlM knockout mutants, 1 μg of pCr202 (for CpSRP43) or pCr112 (for ChlM) were linearized with XbaI and added to the mixture, thereby conferring resistance to hygromycin38. The electroporation voltage and pulse interval were 250 V and 15 ms, respectively. Electroporated cells were recovered for 16 hours in TAP medium containing 40 mM of sucrose, with agitation (120 rpm) under continuous low light. Mutant cells were selected on TAP agar plates containing 1.5 mM of L-tryptophan and 25 μM of 5-FI (Sigma-Aldrich, USA) for tryptophan auxotrophic selection, or on TAP agar plates with 15 mg/L of hygromycin B (Thermo Fisher Scientific, USA) for co-transformation.
Complementation of CRISPR/Cas9-induced MAA7 mutants
To confirm the functional significance of the isolated MAA7 mutations, we cloned the MAA7 CDS from CC-124 and MAA7 20-1 and performed complementation assays on MAA7 20-1 and the RNAi mutant, MAA7 RNAi #3317. Cells were exponentially grown in TAP with shaking at 120 rpm under continuous light of 120 μmol m−2s−1, and total RNAs were isolated using the RNeasy Plant Mini kit (Qiagen, the Netherlands) and the RNase-Free DNase Set (Qiagen, the Netherlands) according to the manufacturer’s instructions. Any remaining DNAs were removed with a DNA-free DNase kit (Ambion, USA), and cDNAs were produced using Superscript III Reverse Transcriptase and oligo (dT)20 primers (both from Invitrogen, USA). Individual CDSs were amplified using the Phusion High-Fidelity DNA Polymerase (NEB, USA) and primers I202TSB_3F and I202TSB_3R, and the obtained fragments were cloned into the pCr202 vector38 using a Gibson Assembly kit (NEB, USA) according to the manufacturer’s instructions. CDS expression was controlled by the HSP70A and RBCS2 promoter and terminated by the psaD terminator54. We added a translation initiation context (AACA) in front of the start codon55 and a FLAG-tag sequence (GACTACAAGGACGACGACGACAAG) next to the CDS56. Cloned plasmids were delivered to MAA7 20-1 and MAA7 RNAi #33 by electroporation, as described in the previous section. After recovery, transformed cells were spread on TAP agar plates containing 1.5 mM L-tryptophan and 15 mg/L hygromycin B. After 1 week, hygromycin-resistant colonies were subjected to PCR verification of the following: transformant status, as assessed by the presence of the aphVII gene (using primers aph72_L and aph72_R); the presence of the transgenic MAA7 gene, as assessed using TSB flag_4F and TSB flag_4R; and proper amplification of the 18S rDNA (using primers SR6 and SR9) as a positive control. Expression of the transgenic MAA7 protein was confirmed by Western blotting using a rabbit anti-FLAG-tag antibody (diluted 1:1000; Cell Signaling Technology, USA). Clones of Western-positive cells were subjected to complementation assays by growth in 24-well plates (SPL, Republic of Korea) under continuous light (120 μmol m−2s−1) with shaking at 150 rpm for 4 days in the presence or absence of 25 μM 5-FI. Cell growth was monitored using the OD750 nm, which was assessed using a SpectraMax M2e Microplate reader (Molecular Devices, USA).
Chlorophyll contents were measured using methanol extraction according to published protocols57. Briefly, 5 mL of cells were centrifuged at 5,035 × g for 10 min and washed twice with distilled water twice. Pellets were resuspended in the same volume of methanol and incubated in the dark at 4 °C for 1 hour. After centrifugation at 5,035 × g for 10 min, the optical density of supernatant was measured at 652 and 665 nm using a UV-1800 UV-VIS Spectrophotometer (Shimadzu, Japan). The concentrations of chlorophyll a and b were calculated as follow:
Chl a [μg/mL] = −8.0962 × OD652 nm + 16.5169 × OD665 nm
Chl b [μg/mL] = 27.4405 × OD652 nm − 12.1688 × OD665 nm
The obtained chlorophyll contents were normalized to the cell density, which was measured using a Cellometer AutoT4™ (Nexcelom Bioscience, USA).
Genomic DNA extraction and whole genome sequencing
Genomic DNA was extracted according to published methods58,59. Briefly, cells were grown to the stationary phase, harvested, washed with 50 mM EDTA, and resuspended in 150 μL distilled water and 300 μL SDS-EB. DNA was extracted with a mixture of phenol and chloroform (1:1), with repeated applications of the mixture (500 μL) made until the interphase became clear. The DNA was washed with 500 μL chloroform and precipitated with two volumes of ethanol. The obtained DNA pellet was washed with 70% ethanol and air-dried, and the DNA was resuspended in 40 μL of TE buffer. Whole-genome sequencing was performed using an Illumina HiSeq 2000 (Illumina, USA) according to the provided protocol. Genomic DNA sequences were read with a paired-end sequencing platform (Seeders, Republic of Korea). The SolexaQA package software (version 1.13) was used to trim the short read sequences for better quality. More specifically, the DynamicTrim module was used to eliminate poor-quality bases (Phred score < 20) and the LengthSort module was used to exclude short read lengths <25 bp. The trimmed reads were assembled using the SOAPdenovo version 2.04 (http://soap.genomics.org.cn//soapdenovo.html) under default options60. The assembled contigs were aligned with the C. reinhardtii reference genome v5.5 (http://www.phytozome.net) and with the sequence of the vector pCr202 for CpSRP43 mutagenic experiments. BLASTN searches were performed using cutoffs of 1e-10 and 90% identity.
Phylogenetic analyses of TSB sequences were performed using the CLC Genomics Workbench version 7.0 (CLC bio, USA). Twenty-three TSB amino acid sequences from organisms representing all five kingdoms were obtained from GenBank (Fig. 2C). For the alignment parameters, the gap-open cost and gap-extension cost were set at 10.0 and 1.0, respectively. The full sequence of the TSB protein, including the Cas9 cut site, is presented in Fig. S1. A phylogenetic tree of the aligned sequences was constructed using the neighbor-joining method, and the Jukes-Cantor model was used to measure protein distance.
Western blot analysis
To confirm our knockout of the CpSRP43 protein, Western blotting was performed. C. reinhardtii cells were grown to the exponential phase, and the cell density was normalized to 107 cells. The cells were harvested, washed once with distilled water, and collected by centrifugation at 13,000 rpm for 10 min. The cell pellets were resuspended with 1.5× Laemmli buffer (62.5 mM Tris-HCl pH 7.6, 7% sodium dodecyl sulfate, 25% glycerol, 5% β-mercaptoethanol, and 0.02% bromophenol blue) and incubated at 100 °C for 5 min. The samples were centrifuged at 13,000 rpm for 5 min, and the supernatants were loaded to Mini-PROTEAN® TGX Stain-FreeTM Gel of Any KD (Bio-Rad, USA) and run in 1× TGX buffer. The resolved proteins were transferred to PVDF membranes using the Trans-Blot® TurboTM System (Bio-Rad, USA). The membranes were blocked with 1× PBS containing 5% skim milk and 0.1% Tween 20 with agitation. The CpSRP43 protein was detected using polyclonal antibodies raised against the antigenic sequence, CERRFKIRWSDGYPTSWEPEE34. The β-subunit of ATP synthase (ATPβ) was detected as a loading control. Then, the blots were incubated with horseradish peroxidase (HRP)-conjugated anti-rabbit secondary antibodies (Cell Signaling Technology, USA) for 1 hour, and the results were visualized by chemiluminescent detection using the Clarity Western ECL substrate and a ChemiDoc system (Bio-Rad, USA).
Southern blot analysis
For Southern blot analysis of the CpSRP43 and ChlM mutants, 10 μg of genomic DNA was digested with Pst I/NcoI and NcoI, respectively, separated by 0.8% agarose gel electrophoresis, and then blotted onto Hybond-N+ nylon membranes (Amersham Biosciences, Sweden). 0.3-kb PCR fragments corresponding to the aphVII, CpSRP43 and ChlM genes were used as probes. The primers used to generate each probe are listed in Table S1. 32P-labeled probes were produced using the RediprimeTM II Random Labeling System (Amersham Biosciences, Sweden) and hybridization was performed following the manufacturer’s instructions. The probe-bound membrane was washed and exposed to a phosphor-imaging plate (IP) for 3 days, and the obtained signals were detected using a Bio-Imaging Analyzer BAS-1800II (Fuji, Japan).
Semi-quantitative RT-PCR analyses
Total RNA was extracted from WT and ChlM mutants using the TRIzol reagent (Invitrogen, USA) according to the manufacturer’s instructions. Reverse transcription was carried out using 2 μg total RNA, 50 μM oligo (dT)18, 200 U M-MLV reverse transcriptase (Promega, USA), 500 μM of each dNTP, and 20 U ribonuclease inhibitor (Thermo Fisher Scientific, USA). For semi-quantitative RT-PCR, cDNAs were amplified with 1.5 U Ex Taq DNA polymerase (TaKaRa, Japan), 100 μM of each dNTP and 10 pmol of each gene-specific primer, using a T1 thermal cycler (Biometra GmbH, Germany). Amplification was performed with 25–40 cycles of 94 °C for 30 s, 56 °C for 30 s, and 72 °C for 30 s. The primers used to amplify the ChlM and IDA5 cDNAs are listed in Table S1.
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We honor and acknowledge deceased Professor Ji-Won Yang for his inspiration on this project and establishment of the Advanced Biomass R&D Center (ABC). We thank Dr. Heriberto Cerutti for providing the MAA7 RNAi #33 strain. This work was supported by the Advanced Biomass R&D Center (ABC) of Global Frontier Project funded by the Ministry of Science, ICT, and Future Planning (ABC-2011-0031350, ABC-2010-0029728 and ABC-2011-0031343) and by a grant from Institute for Basic Science (IBS-R021-D1).
The authors declare no competing financial interests.
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Shin, SE., Lim, JM., Koh, H. et al. CRISPR/Cas9-induced knockout and knock-in mutations in Chlamydomonas reinhardtii. Sci Rep 6, 27810 (2016). https://doi.org/10.1038/srep27810
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