Author response:
The following is the authors’ response to the original reviews.
In revising the manuscript, we have focused on three main priorities raised during review: (1) improving precision around evidential claims, particularly concerning vector maintenance and P2A-mediated protein separation; (2) substantially improving figure quality, accessibility, and legend clarity; and (3) correcting inconsistencies and expanding methodological detail where requested.
This study was intended as a foundational genetic toolkit and methodological framework for Blastocystis ST7-B, establishing practical workflows for DNA delivery, endogenous regulatory-element benchmarking, antibiotic-selected recovery, clonal propagation, and reporter-based analysis in a genetically challenging anaerobic microbial eukaryote. The central evidence presented is therefore functional in nature: reproducible transgene delivery, selectable recovery and propagation of colony-derived transgenic lines, and detectable reporter expression using multiple anaerobic-compatible reporter systems.
We agree with the reviewers that several additional experiments, including Western blot analysis of P2A-containing constructs, outward-facing PCR, plasmid rescue assays, and selection-withdrawal experiments, would further strengthen the mechanistic interpretation of the system and help distinguish episomal persistence from genomic integration. We have therefore revised the manuscript throughout to clearly separate what is directly demonstrated from what remains a plausible working interpretation or important future direction.
Importantly, the revised manuscript no longer presents episomal maintenance or complete P2A-mediated protein separation as demonstrated conclusions. Instead, these are now discussed explicitly as unresolved mechanistic questions requiring future molecular analysis. Nevertheless, the central methodological conclusion remains unchanged: stable selectable transgene expression, recovery of colony-derived transgenic lines, and reporter-positive Blastocystis ST7-B transformants can now be reproducibly obtained.
Reviewer #1 (Public review):
Summary:
This paper presents a toolkit for the transformation of Blastocystis. The authors have screened a number of selectable agents, promoters and reporter genes and present their findings. This resource will be of immense use to those in the Blastocystis field, as well as those seeking to establish transformation tools in other species where such tools do not yet exist. Establishing new transformation tools is extremely challenging, and the authors have done an excellent job.
Strengths:
The authors have carried out a systematic screen of promoters, reporter genes and selectable agents. They have screened numerous for each, and all the data is presented. It is good to see when things did not work as well as when things did, so this data set is extremely useful indeed.
Weaknesses:
The findings are reported by reporter gene assay (microscopy). No evidence is given using genetics. The authors claim that the DNA is maintained episomally. However, could it be possible that there is integration? No PCRS/RT-PCRs are shown (although it can safely be assumed that the DNA/RNA is present where the transformation was successful), nor are any Western blots. These would have been useful to show that the P2A ribosomal skipping had occurred, and that proteins were expressed individually rather than as a polyprotein.
We thank the reviewer for the positive assessment of the manuscript and for recognising both the technical difficulty and broader utility of establishing genetic tools in Blastocystis and other experimentally challenging microbial eukaryotes. We also appreciate the reviewer’s identification of the main evidential limitations in the original manuscript, particularly regarding vector maintenance and P2A-mediated protein separation.
First, regarding the question of vector topology and the interpretation of episomal maintenance.
We agree that the original manuscript presented episomal persistence too strongly relative to the evidence currently available. We have therefore revised the manuscript throughout to clarify that episomal maintenance should presently be regarded as a plausible working model rather than a directly demonstrated conclusion.
The transfection system used here was adapted from Li et al. (2019), including use of the pXS2-P<sub>Legumain</sub>-derived plasmid framework. Importantly, the construct used in the present study does not contain the original Trypanosoma brucei tubulin-targeting region associated with homologous integration in the original pXS2 system. Complete plasmid sequencing confirmed that the constructs function here as heterologous expression plasmids carrying Blastocystis ST7-B regulatory elements and transgenes. While this does not demonstrate episomal persistence, it also means that genomic integration cannot be inferred from the historical pXS2 vector architecture alone.
We further note that comparative genomic analyses by Gentekaki et al. (2017) suggest that Blastocystis lacks components of the canonical non-homologous end-joining (NHEJ) machinery, implying that homologous recombination is likely to represent the principal route for double-stranded DNA repair. Because the constructs used here did not contain Blastocystis homology arms, there is currently no obvious mechanism favouring targeted homologous integration. Nevertheless, we fully agree that genomic integration cannot presently be excluded.
To reflect this appropriately, the revised manuscript now explicitly separates the demonstrated functional outcomes from unresolved mechanistic questions concerning vector maintenance. We also identify several future approaches that would help distinguish episomal persistence from genomic integration, including outward-facing PCR, plasmid rescue followed by full plasmid sequencing, Southern blotting, FISH, selection-withdrawal experiments, and long-read sequencing approaches.
We have revised the manuscript throughout to remove statements implying demonstrated episomal maintenance and now present episomal persistence only as a plausible working interpretation.
In the Methods section under Cloning, the following text has been added:
Lines 202–206: “The constructs used in this study were derived from the pXS2-P<sub>Legumain</sub> vector described by Li et al. (2019), which adapted a heterologous expression-vector backbone for transient plasmid-based expression in Blastocystis ST7-B. Here, the same molecular backbone was used as a plasmid scaffold carrying Blastocystis-derived regulatory elements and transgenes.”
In the Discussion, the following text has been added/edited:
Lines 665–673: “The molecular maintenance state of the introduced constructs remains unresolved: episomal maintenance is a plausible working model, but genomic integration cannot be formally excluded. The constructs used here lack Blastocystis homology arms, and comparative genomic analyses suggest that Blastocystis lacks canonical non-homologous end-joining components (Gentekaki et al., 2017), making targeted integration by standard repair routes unlikely but not impossible. Direct assays such as outward-facing PCR, plasmid rescue followed by full plasmid sequencing, FISH, or selection-withdrawal experiments will be required to distinguish episomal persistence from integration.”
Second, regarding P2A-mediated protein separation.
We agree that Western blotting would provide the most direct biochemical assessment of P2A-mediated ribosomal skipping efficiency in Blastocystis ST7-B and would help determine the extent of any residual uncleaved fusion product. We have therefore revised the manuscript to avoid implying that complete protein-level separation was directly demonstrated.
The revised manuscript now states only what is directly supported by the current data: that P2A-containing bicistronic constructs supported antibiotic-selected recovery of transgenic lines together with detectable downstream reporter expression. The microscopy data therefore support functional downstream reporter expression, but do not by themselves exclude residual uncleaved fusion products.
We selected P2A because it is a compact and well-characterised peptide with high reported separation efficiency across multiple eukaryotic systems, including microbial eukaryotes. However, we agree that P2A performance can be context-dependent, and we now explicitly identify biochemical validation of P2A cleavage efficiency as an important future direction.
Importantly, these revisions do not alter the central methodological conclusion of the study, namely that selectable transgene expression, propagation of reporter-positive lines, and recovery of colony-derived Blastocystis ST7-B transformants can now be reproducibly achieved.
Text inserted in the Results:
Lines 394–396: “The P2A peptide is expected to promote ribosomal skipping during translation, allowing two separate polypeptides to be produced from a single open reading frame.”
Lines 403–404: “However, protein-level separation was not directly tested, and the extent of any residual uncleaved fusion product remains unresolved.”
Text inserted in the Discussion:
Lines 619–629: “P2A was selected because it is a well-characterised peptide with high reported separation efficiency in human cell lines, zebrafish embryos, and mice (Kim et al., 2011). It also has precedent across microbial eukaryotes, including the protest Dictyostelium discoideum (Zhu et al., 2023), the fungi Aspergillus niger (Schuetze and Meyer, 2017) and Ustilago maydis (Müntjes et al., 2020), and the apicomplexan parasites Toxoplasma gondii (Markus et al., 2019) and Plasmodium falciparum (Dans et al., 2024). However, P2A performance is context-dependent, and the evidence presented here is functional rather than biochemical. P2A-containing constructs support antibiotic-selected recovery and downstream reporter expression in Blastocystis ST7-B, but ribosomal skipping efficiency and any residual uncleaved product will require direct protein-level validation.”
Reviewer #1 (Recommendations for the authors):
(1) Please could you show a Western blot to confirm if P2A has worked? It could be that the proteins are being expressed as a polyprotein.
We agree that Western blotting would provide the most direct biochemical assessment of P2A-mediated ribosomal skipping efficiency in Blastocystis ST7-B and would help determine the extent of any residual uncleaved fusion product. This is an important point, and we have revised the manuscript accordingly to avoid implying that complete protein-level separation was directly demonstrated.
The current study was designed as a first-generation functional genetic toolkit for Blastocystis ST7-B, focused primarily on establishing reproducible workflows for selectable transgene expression, reporter recovery, and propagation of transgenic lines in this experimentally challenging anaerobic microbial eukaryote. The toolkit is therefore validated here through functional outcomes, including antibiotic-selected survival, stable propagation through extended passaging (>15 passages) and cryopreservation, and detectable reporter fluorescence above wild-type autofluorescence.
P2A was selected because it is a compact and well-characterised peptide with high reported ribosomal skipping efficiency across multiple eukaryotic systems, including microbial eukaryotes, as discussed above. Nevertheless, we fully agree that direct biochemical validation would strengthen the mechanistic interpretation of the bicistronic system in Blastocystis ST7-B. We therefore now explicitly identify Western blot analysis, ideally using epitope-tagged upstream and downstream products, as an important future direction for quantitative assessment of P2A cleavage efficiency and any residual uncleaved fusion products.
Relevant manuscript revisions are described above under the general response to Reviewer 1.
(2) Something has gone wrong with figure formatting. Figure 2 is nearly illegible and I cannot read the text in section A. Sections B, C, and D have lost their labels and are fuzzy and surrounded by black. A similar issue affects Figure 3. Everything is just black with a few cells. It is illegible when printed.
We thank the reviewer for highlighting these presentation issues and agree that the submitted figure quality significantly impaired readability and interpretation. The problems appear to have arisen primarily during manuscript compilation and export, particularly affecting image resolution, contrast, and panel labelling in the review PDF.
To address this, Figures 2 and 3 have been completely reformatted and replaced with revised high-resolution versions. We have also improved typography, panel separation, colour scaling, and legend clarity throughout. In response to additional reviewer suggestions, individual data points have now been added to Figures 2B and 2C to improve transparency and interpretability of the underlying data distributions.
Figures 2 and 3 have been replaced with fully revised high-resolution versions with improved panel labelling, accessibility, typography, and figure legends.
(3) The data from Figure 2B would be better placed in Table 1 with a column for robust/moderate/intermediate/weak/very weak. This would be much easier for the reader.
We thank the reviewer for this helpful suggestion. We believe the comment refers to the promoter activity data shown in Figure 2A rather than the voltage optimisation data in Figure 2B. To improve readability and accessibility of these data, we have revised Figure 2A extensively to make the promoter activity tiers more legible and easier to interpret directly from the heat map and accompanying box plots.
We considered incorporating simplified activity classifications into Table 1. However, activity patterns were construct-specific rather than simply locus-specific. In several cases, multiple promoter fragments derived from the same locus produced substantially different reporter outputs, and activity did not scale monotonically with promoter fragment length. We therefore felt that assigning a single categorical activity label at the locus level would oversimplify the dataset and reduce the construct-level resolution that is central to the toolkit value of the study.
Instead, we addressed the reviewer’s concern by substantially improving the presentation and readability of Figure 2A, allowing readers to identify robust, moderate, intermediate, weak, and very weak expression constructs more directly while preserving the underlying construct-specific information.
Figure 2A has been revised to improve clarity, accessibility, and legibility of the promoter activity tiers, allowing construct-level expression classes to be interpreted more directly from the heat map and accompanying boxplots.
(4) How do you know if the constructs are maintained as episomes? Have you done an outward-facing PCR?
We agree that direct molecular evidence distinguishing episomal persistence from genomic integration is currently lacking, and we appreciate the reviewer highlighting this important limitation. We have therefore revised the manuscript throughout to avoid presenting episomal maintenance as a demonstrated conclusion and now describe it only as a plausible working interpretation based on the current evidence and vector design.
We have not performed outward-facing PCR in the present study. As discussed in the general response above, we now explicitly identify outward-facing PCR, plasmid rescue followed by full plasmid sequencing, selection-withdrawal assays, FISH, and long-read sequencing approaches as important future directions for resolving the molecular maintenance state of the constructs.
The revised manuscript now clearly separates the demonstrated functional outcomes, including selectable transgene expression, recovery of colony-derived transgenic lines, and stable reporter-positive propagation under selection, from the unresolved mechanistic question of vector topology.
This issue has been addressed throughout the revised manuscript, including in the Methods and Discussion sections, where episomal maintenance is now presented as a plausible but unconfirmed interpretation rather than a demonstrated conclusion.
Minor Comments
Line 66: is this one to two billion individuals with Blastocystis, or one to two billion Blastocystis cells per gut?
The intended meaning was colonised individuals globally. We agree that the original phrasing was ambiguous and have corrected it for clarity.
Lines 66–67 revised to: “…microorganisms in the human gut, and is estimated to colonise approximately one to two billion people globally (Scanlan and Stensvold, 2013).”
Line 148: Supplier of IMDM?
The supplier information was already present in the original manuscript as IMDM L0191 (Biowest).
No additional manuscript change required.
Line 157: Who annotated the dataset, the 2017 paper or the present study?
The dataset annotation derives from Armengaud et al. (2017). We agree that the original wording was unclear and have revised this section substantially to improve clarity regarding the rationale and workflow used for promoter and terminator candidate selection.
“The relevant Methods section has been extensively revised for clarity and expanded detail” (Lines 156–189).
Line 166: Who predicted the 3′ UTR, the 2017 paper?
This information derives from the NCBI annotation associated with the Blastocystis ST7-B genome based on Denoeud et al. (2011). This has now been clarified in the Methods section.
Clarified in revised Methods section.
Line 237: How long did it take in days?
Approximately 2 days.
Line 270 revised to: “…turned yellow without drug treatment, usually within 2 days post-transfection.”
Line 325: Typo, missing gap between Figure and 1A.
Corrected in revised manuscript.
Reviewer #2 (Public review):
This manuscript presents a substantial technical advance for the genetic manipulation of Blastocystis by establishing an integrated workflow for stable episomal transgenesis, antibiotic selection, clonal recovery, and reporter-based imaging in the ST7-B subtype. The study is particularly valuable because it combines multiple previously fragmented approaches into a coherent and practically applicable toolkit, including endogenous regulatory elements, optimized electroporation conditions, selectable markers, and anaerobic compatible fluorescent reporters. This methodological work greatly expands the molecular toolbox and future studies focused on both basic and infection biology can now build on the ability to express and localize proteins in fixed as well as live cells.
The microscopy data are convincing and clearly demonstrate functional reporter expression and successful recovery of stable transgenic lines. Nevertheless, because this is primarily a methodological paper, the study would be further strengthened by the inclusion of Western blot validation of reporter expression and bicistronic constructs. In particular, biochemical analysis of the P2A-containing constructs would help assess the efficiency of ribosomal skipping and exclude the possible presence of uncleaved fusion proteins, thereby providing stronger support for the interpretation of the imaging data and the functionality of the expression system.
We thank the reviewer for this thoughtful and positive assessment of the manuscript and for recognising the value of integrating previously fragmented approaches into a coherent and practically usable genetic toolkit for Blastocystis ST7-B. We particularly appreciate the reviewer’s recognition that the system expands the currently available molecular toolbox for both cell biological and infection-related studies in this experimentally challenging anaerobic microbial eukaryote.
We also appreciate the reviewer’s comments regarding biochemical validation of the P2A-containing bicistronic constructs. We agree that Western blot analysis would strengthen the mechanistic interpretation of the reporter system by directly assessing ribosomal skipping efficiency and the possible presence of residual uncleaved fusion products. In response, we have revised the manuscript throughout to ensure that the conclusions remain appropriately evidence-based and do not imply that complete protein-level separation was directly demonstrated.
The revised manuscript now explicitly distinguishes the demonstrated functional outcomes, including selectable transgene expression, stable propagation of reporter-positive lines, and detectable downstream reporter expression, from unresolved mechanistic questions concerning P2A cleavage efficiency and vector maintenance state. We now also identify biochemical validation of P2A-mediated protein separation as an important future direction for further refinement of the system.
Relevant manuscript revisions addressing these points are described above under the response to Reviewer 1.
Reviewer #2 (Recommendations for the authors):
The quality of images could be better. The figures lacked resolution — possibly a conversion artefact.
We agree that the figure quality in the submitted review PDF significantly reduced readability and visual interpretation. The issues appear to have arisen primarily during manuscript compilation and export, particularly affecting image resolution, typography, panel labelling, and contrast rendering.
To address this, Figures 2 and 3 have been completely reformatted and replaced with revised high-resolution versions. We have also improved panel separation, typography, colour scaling, contrast settings, and figure legends to improve accessibility and interpretability both on screen and in print. In addition, the export workflow and file formatting have been updated to improve compatibility with journal production requirements and reduce the likelihood of compression-related rendering artefacts during manuscript compilation.
Figures 2 and 3 have been replaced with revised high-resolution versions with improved typography, panel labelling, contrast settings, and accessibility.
Reviewer #3 (Public review):
Summary:
The primary objective of this study was to establish a practical and functional framework for the propagation of stable transgenic cell lines of Blastocystis, a common animal gut microeukaryote. Although the work focused on Blastocystis ST7-B, a subtype with relatively low prevalence in humans, this choice is justified by its association with more frequent negative health effects. Beyond their relevance to the medical field, the methodological advances described here have the potential to also expand cell biology studies of this anaerobic organism, including its unusual mitochondria and redox metabolism.
Strengths:
Prior to this work, genetic tools for Blastocystis were very limited, relying on a single strong promoter-terminator combination. The authors successfully expanded the available promoter set across a range of expression strengths by testing two dozen variants in luciferase-based assays. Critically, they developed an integrated workflow from a modular transgenic construct design, to an expanded inventory of molecular components (promoters, reporters), optimized DNA delivery, stepwise antibiotic resistance-mediated clonal selection and propagation, and to reporter validation. The evaluation of several anaerobiosis-compatible labeling strategies for live (and fixed) cell optical imaging will be particularly useful, with the SNAP-tag system appearing especially promising for Blastocystis.
Weaknesses:
The presented data generally provide solid support for the conclusions that the work reached, but clarification of reasoning and several inconsistencies, as well as amendments to the visual presentation of the data, would be highly beneficial, as detailed below.
(1) Episomal persistence of the construct:
The manuscript repeatedly assumes, including in its title, that constructs persist in Blastocystis in their episomal form, but no direct evidence is provided. Although this interpretation is plausible, it should be identified more clearly as provisional. Nuclear genomic integration (e.g., via NHEJ) remains a possible explanation unless supporting evidence or rationale is provided to exclude it. Testing whether the phenotype persists without drug-mediated selection in the generated transgenic cell lines would help strengthen the case for episomal maintenance.
We thank the reviewer for this important point and agree that the original manuscript presented episomal persistence too strongly relative to the currently available evidence. In particular, we agree that the title and several sections of the manuscript implied a level of mechanistic certainty that was not directly demonstrated.
We have therefore revised the manuscript throughout to clarify that episomal maintenance should presently be regarded as a plausible working interpretation rather than a demonstrated conclusion. The revised text now explicitly distinguishes the demonstrated functional outcomes, including selectable transgene expression, recovery and propagation of colony-derived transgenic lines, and stable reporter-positive maintenance under selection, from the unresolved mechanistic question of vector topology.
As discussed in our response to Reviewer 1, the constructs used here do not contain Blastocystis homology arms, and comparative genomic analyses suggest that Blastocystis lacks canonical non-homologous end-joining components, making targeted integration by standard repair routes less strongly supported mechanistically, although genomic integration cannot presently be excluded.
We agree that selection-withdrawal experiments would provide useful additional evidence regarding construct persistence and have now explicitly identified such assays, together with outward-facing PCR, plasmid rescue, FISH, and long-read sequencing approaches, as important future directions for resolving the molecular maintenance state of the transgenes.
The manuscript has been revised throughout to remove wording implying demonstrated episomal maintenance. Episomal persistence is now discussed only as a plausible working interpretation pending direct molecular validation.
(2) Promoters and terminators:
(2.1) There is a discrepancy between the claimed number of loci (14), from which promoters used to drive luciferase expression were derived, and those detailed as having been actually generated in Table 1 (11). This inconsistency should be corrected or explained, as it creates uncertainty around the accuracy of the dataset.
We thank the reviewer for this careful reading and for identifying this inconsistency. We agree that the distinction between candidate loci and successfully generated promoter constructs was not sufficiently clear in the original manuscript and could create uncertainty regarding the dataset.
The original candidate set comprised 14 loci selected for promoter and terminator discovery. However, only 11 loci yielded successfully cloned and experimentally tested promoter constructs. The remaining three loci were retained in Table 1 for completeness and transparency, as repeated cloning attempts were unsuccessful despite two independent efforts.
We have revised the manuscript to make this distinction explicit and to clarify that the reported NanoLuc benchmarking experiments were ultimately performed using constructs derived from 11 successfully cloned loci.
Lines 361–364: “To expand the available regulatory parts, we screened 23 NanoLuc reporter constructs containing putative endogenous promoter–terminator pairs from 11 of 14 candidate loci; three loci could not be cloned after two independent attempts and are indicated in Table 1.”
(2.2) Based on the presented evidence, constructs benchmarked in bioluminescence assays differed only in their promoter composition. Although terminator selection is mentioned in the Methods section, no additional details are provided; for instance, Table 1 and Figure 2 only list 23 promoters in total. Figure 2A likewise shows only promoter-dependent variation. If the terminator was held constant (LeguP1?), this should be stated explicitly. The authors may then consider revising the wording of having tested “23 promoter-terminator pairs” to better reflect that only promoters varied.
We thank the reviewer for the opportunity to clarify this point. We agree that the original presentation may have created the impression that promoter and terminator regions were independently varied and benchmarked, whereas the experimental design was primarily focused on construct-level comparison of endogenous regulatory modules.
As described in the Methods, each construct contained a candidate endogenous upstream promoter region together with the corresponding endogenous downstream terminator region derived from the same locus. For consistency and to keep the cloning and screening strategy experimentally tractable, a fixed 500 bp downstream terminator fragment was used for each locus rather than systematically varying terminator length or independently testing terminator activity.
We therefore retain the description “endogenous promoter–terminator pairs,” since each construct contains both endogenous upstream and downstream regulatory regions from the same genomic locus. However, we agree that the assay was not designed to independently dissect promoter versus terminator contributions to reporter output. We have revised the manuscript accordingly to make this distinction explicit and avoid ambiguity regarding the scope of the benchmarking analysis.
Lines 365–368: “Each construct paired a candidate upstream promoter region with the corresponding downstream terminator region from the same locus, defined here as the native 500 bp sequence immediately downstream of the stop codon. Where multiple promoter lengths were tested for the same locus, the terminator fragment was kept constant (Table 1; Figure 1A).”
This design allowed construct-level benchmarking of paired promoter–terminator modules but did not test promoter strength or terminator activity independently.
(2.3) Promoter benchmarking was done with a plasmid lacking a selection marker, so it is unclear how the maintenance of the luciferase construct was ensured. Without selection, the observed reporter intensity could reflect differential or stochastic plasmid retention rather than promoter strength alone. The luminescence assay was performed 16-18 hours after transfection, but the rationale for this particular timeframe should be explained. In this context, the authors should explicitly state whether the experiments shown in Fig.2A represent biological triplicates or technical triplicates from a single transfection.
We thank the reviewer for these important methodological points. We agree that the original manuscript did not sufficiently clarify the transient nature of the NanoLuc benchmarking assay or the rationale underlying the assay design and timing.
The promoter benchmarking assay was designed as an early transient-expression screen adapted from the NanoLuc-based workflow of Li et al. (2019), with modifications, rather than as a stable-maintenance assay. No selectable marker was included because the objective was to compare relative early reporter output across constructs shortly after DNA delivery, before prolonged culture effects became dominant.
The 16–18 h post-electroporation time point was selected based on the NanoLuc expression kinetics reported by Li et al. (2019) and empirical optimisation during assay development. This window allowed robust transient reporter detection while limiting confounding effects arising from prolonged plasmid loss, differential outgrowth, variable recovery, or later culture-level changes.
We agree that, in the absence of selection, the observed NanoLuc signal cannot be interpreted as an absolute measure of promoter strength independent of DNA uptake efficiency, early plasmid retention, or post-transfection recovery dynamics. We have therefore revised the manuscript to clarify that Figure 2A reports relative transient reporter output under standardized early post-transfection conditions rather than isolated promoter activity alone.
We now also explicitly state that the data shown in Figure 2A derive from three independent electroporation experiments per construct, each assayed in technical duplicate.
Lines 241–248: “Promoter–terminator activity was assessed 16–18 h after electroporation using a transient NanoLuc assay adapted from Li et al. (2019), with modifications. This early time point was selected to capture reporter output within the transient-expression window after DNA delivery, before prolonged plasmid loss, differential outgrowth, or culture-level changes could dominate the readout. Because the constructs did not contain a selectable marker, the measured NanoLuc signal reflects early transient reporter output rather than promoter strength independent of DNA uptake, early plasmid retention, or post-transfection recovery.”
Additional clarification added to Figure 2 legend stating that measurements derive from three independent electroporation experiments, each assayed in technical duplicate.
(3) Figure 2:
(3.1) Several aspects of the current design may lead to ambiguity for the reader. The boxplots are colour-coded, but it is unclear whether the colours carry meaning or are purely decorative. Because the data are already spatially separated into bins, additional random colouring is redundant and may suggest distinctions that are not intended. In addition, part A of Figure 2 is split into two panels, with the scale for the left panel shown in the right panel and some of the boxplot colours falling in the range of the scale, but not in line with their counterparts in the left panel. Because the colour use is not consistent, it is difficult to tell whether the same scale should be applied to both panels or how it should be interpreted.
(3.2) The left panel of part A uses a diverging blue-white-red colour scheme, which is most appropriate when the midpoint represents a meaningful central value such as zero. Because the values shown in this graph are only positive, a non-diverging 2-colour scale or a colour palette such as 'viridis' would make the plot easier to interpret.
(3.3) A black background should be avoided: 'B' and 'C' labels are invisible, and it draws attention to a distracting design feature rather than the data themselves.
We thank the reviewer for these detailed comments regarding figure design and visual interpretation. We agree that the original presentation of Figure 2 introduced unnecessary visual ambiguity through inconsistent colour usage, the use of a diverging colour scale for strictly positive values, and poor readability associated with the dark background and low-resolution export.
In response, Figure 2 has been extensively redesigned to improve clarity, accessibility, and interpretability. The previous blue–white–red diverging heatmap has been replaced with a sequential colour palette appropriate for positive-only expression data. Boxplot colouring has also been simplified and harmonised with the heatmap scheme to avoid implying unsupported categorical distinctions. In addition, panel organisation, typography, scaling, and legend structure have all been revised to improve readability and reduce ambiguity regarding interpretation of the plotted values.
We also agree that the black background distracted from the data presentation and impaired visibility of panel labels and image boundaries. The revised figures therefore use white backgrounds together with clearer panel separation and improved label visibility throughout.
Figure 2 has been completely reformatted using a sequential colour scale in panel A, simplified and harmonised boxplot colouring, larger typography, improved panel separation, revised legends, and white backgrounds throughout. Corrected high-resolution source figures have been provided.
(4) Figure 3:
(4.1) Individual snapshots should be separated more clearly, either by using a white background or by adding visible borders to make the overall composition clearer. As currently displayed, some boundaries between fluorescent channels resemble image artifacts rather than intentional panel divisions.
We thank the reviewer for this helpful comment regarding figure composition and panel separation. We agree that the original presentation made it difficult to distinguish intentional panel boundaries from imaging artefacts, particularly in the low-resolution review PDF generated during manuscript compilation.
To improve clarity, Figure 3 has been reformatted using white backgrounds, clearer panel spacing, and more explicit separation between individual snapshots and imaging channels. High-resolution source images have also been provided to ensure that fluorescence patterns, image boundaries, and panel organisation remain clearly interpretable both on screen and in print.
Figure 3 has been reformatted with improved panel separation, white backgrounds, clearer image boundaries, and revised high-resolution source figures.
(4.2) In parts B-D, the legend should explain more clearly what each image shows, and the figure itself would benefit from annotations. There seem to be three sub-panels in each 'condition' of part B (as well as C and D): while the middle and rightmost panel can be easily inferred to represent the fluorescent protein and bright-field image, what the leftmost panels represent is not specified. If DAPI was used to dye DNA, an explanation why mostly multiple labelled regions are visible should be provided.
We thank the reviewer for these helpful suggestions regarding figure annotation and legend clarity. We agree that the original presentation did not sufficiently explain the composition of the imaging panels, particularly under the low-resolution conditions of the review PDF.
To improve interpretability, the revised Figure 3 now includes clearer panel organisation, improved annotations, and expanded figure legends explicitly identifying the individual imaging channels and staining conditions shown in each subpanel. The leftmost panels in parts B–D are now more clearly identified in both the figure and legend, together with the corresponding fluorescence or staining conditions used in each experiment.
As mentioned in the Methods sections we used Hoechst 33342 to visualise DNA; but we agree that the Hoechst 33342-labelled structures required additional clarification. The revised legend section now explains that multiple Hoechst 33342-positive regions are commonly observed because Blastocystis cells can contain multiple nuclei depending on cell stage and subtype-specific morphology.
In addition, high-resolution source images have been provided to ensure that fluorescent signals, panel boundaries, and imaging features remain clearly interpretable both on screen and in print.
Figure 3 legends and annotations have been revised to clarify imaging channels, staining conditions, and panel organisation. The figure caption was also edited to include: “DNA was visualised using Hoechst 33342. Most cells contained two nuclei, and smaller Hoechst 33342-positive signals consistent with mitochondrial DNA were also observed in some instances.”
(4.3) Cell morphology and appearance differ markedly between UnaG/smURFP and SNAP-tag images, which should be explained. A microscope issue is mentioned in the main text, but if that was the cause, the authors should consider replacing the images, as the current distortions complicate interpretation.
We thank the reviewer for this important observation and agree that the apparent morphological differences between the UnaG/smURFP and SNAP-tag panels required additional clarification.
The images shown for the different reporter systems were acquired under different imaging conditions and microscope configurations following an instrument-related issue during part of the imaging workflow, as noted in the Methods section. As a result, direct visual comparison of cell morphology between reporter systems is not appropriate. The primary purpose of these panels is instead to demonstrate reporter detectability, live-cell labelling capability, and the characteristic fluorescence patterns obtained with the different anaerobiosis-compatible reporter systems.
In particular, the SNAP-tag panels were included to demonstrate successful live-cell labelling without permeabilisation together with the expected increase in fluorescence signal at higher substrate concentrations, rather than to support quantitative comparison of cell morphology across imaging conditions.
We considered replacing the affected images. However, equivalent replacement datasets acquired under directly comparable conditions are not currently available. We have therefore retained the original images but revised the figure legend to clarify the intended interpretation and limitations of these panels explicitly.
Figure 3 legend revised to include:
“Because images for the different reporter systems were acquired under different imaging conditions, they are presented to demonstrate reporter detectability and labelling pattern and should not be used for quantitative comparison of cell morphology across reporter systems.”
Reviewer #3 (Recommendations for the authors):
The reader may find the current order confusing starting with construct design before testing which drug to use for selection. The narrative would work better if it started with antibiotic selection as the first logical step for generating stable cell lines.
We thank the reviewer for this thoughtful suggestion regarding narrative structure and agree that multiple organisational strategies are possible for presenting a methodological workflow of this type.
We considered reorganising the Results section to begin with antibiotic selection and drug sensitivity profiling. However, we ultimately retained the overall structure because the manuscript is organised as a toolkit-development framework rather than as a strictly chronological experimental protocol. The Results therefore begin with regulatory-element discovery and construct design, which form the conceptual and experimental foundation of the toolkit, before progressing to DNA delivery optimisation, drug sensitivity profiling, clonal recovery, and reporter validation.
We felt that this structure most clearly reflects the dependency relationships within the system: regulatory elements are required before constructs can be assembled, constructs are required before electroporation conditions can be evaluated, and selectable constructs are required before stable selection and clonal recovery can be meaningfully assessed.
(2) The text states that the screen 'focused on the 1,000 most abundant proteins to establish a preliminary library capable of supporting varying levels of transcription.' Since the genome has ~6,000 protein-coding genes, the top 1,000 cover the most abundant proteins — not a wide expression range.
We thank the reviewer for this important clarification. We agree that the original wording could incorrectly imply that the screen was intended to sample broadly across the full transcriptional range of the Blastocystis genome. This was not the case, and we have revised the manuscript accordingly.
Our strategy was instead designed to enrich for candidate loci with a higher prior likelihood of supporting detectable transgene expression. Because no genome-wide promoter map, transcription start site dataset, or experimentally validated regulatory annotation was available for Blastocystis ST7-B at the inception of this work, we used the abundance-ranked Blastocystis ST4-WR1 proteomic dataset of Armengaud et al. (2017) as a practical starting point for candidate discovery.
Importantly, the Blastocystis ST4-WR1 proteome is highly skewed, with 193 proteins contributing approximately 50% of the detected proteome and the 13 most abundant proteins contributing approximately 10% (Armengaud et al., 2017). We therefore selected the top 1,000 proteins not as a representation of the genome-wide expression range, but as a proteomics-guided enrichment strategy to identify loci more likely to contain active endogenous regulatory regions suitable for initial toolkit development.
We have revised the relevant Methods section substantially to clarify both the rationale and the workflow used for candidate selection, homolog identification, and promoter/terminator definition.
The Methods section (Lines 156–189) has been extensively revised to clarify the rationale underlying candidate regulatory-element selection. The revised text now explicitly states that the strategy was designed to enrich for likely active loci for toolkit development rather than to systematically survey the full range of promoter strengths across the Blastocystis genome.
Additional methodological detail has also been added regarding:
Use of the Armengaud et al. (2017) proteomic and proteogenomic datasets,
Homolog identification in Blastocystis ST7-B,
Locus selection criteria,
Promoter boundary definition,
And operational definition of candidate terminator regions.
(3) The Methods contain an inconsistency: cells were left in 0.5 mL, then 1 mL was added, but then only 0.5 mL is apparently used for transfection. What happened to the 1 mL?
We thank the reviewer for identifying this ambiguity in the transfection workflow description. The apparent inconsistency arose because the protocol description moved from bulk cell resuspension to preparation of individual electroporation reactions without explicitly stating how the intermediate suspension was used.
After washing, approximately 0.5 mL of cytomix buffer remained above the pellet, and 1 mL of complete cytomix buffer was then added to generate an approximately 1.5 mL cell suspension. Cells were counted from this pooled suspension, after which the volume corresponding to 5 × 10<sup>7</sup> cells was transferred into each individual electroporation reaction. Following addition of DNA, each electroporation reaction was adjusted to a final volume of 500 µL with complete cytomix buffer. The remaining cell suspension was retained for additional transfections or control reactions.
We agree that the original wording could be misinterpreted and have revised the Methods section to clarify the sequential handling steps more explicitly.
Lines 225-229 revised to read: “The resulting approximately 1.5 mL pooled cell suspension was used for total viable cell counting using a hemacytometer.”
“After counting, the volume corresponding to 5 x 10<sup>7</sup> cells was transferred to each electroporation reaction and combined with 25 µg of plasmid DNA. The total electroporation volume was adjusted to 500 µL with complete cytomix buffer.”
(4) Figures 2 and 3 are too low-resolution for the font size used and for clearly viewing the microscopy images.
We thank the reviewer for highlighting these readability issues. As noted in our responses above regarding Figures 2 and 3, the low-resolution appearance primarily resulted from manuscript compilation and PDF export artefacts affecting typography, image rendering, and panel clarity in the review version.
To address this, Figures 2 and 3 have been completely reformatted and replaced with revised high-resolution versions featuring improved typography, panel labelling, contrast, accessibility, and image clarity for both on-screen viewing and print reproduction.
Revised high-resolution versions of Figures 2 and 3 have been provided as described above. No additional manuscript changes were required beyond the figure revisions already outlined.
(5) Figure 4 is confusing because the left and right panels appear inconsistent, with much higher concentrations required for growth inhibition in the culture-based assay than the resazurin assay indicated. The rationale for the resazurin assay should be explained, and the complete growth inhibition (CGI) concentration should be highlighted in the right panel.
We thank the reviewer for highlighting this potential source of confusion. We agree that the distinction between the two assay endpoints was not sufficiently emphasised in the original figure presentation and legend.
The apparent discrepancy arises because the two assays measure different biological endpoints under different assay conditions. The resazurin assay was used to estimate IC<sub>50</sub> values, corresponding to the concentration at which metabolic activity was reduced by approximately 50% under the assay conditions. In contrast, the small-culture assay was designed to determine complete growth inhibition (CGI), defined operationally as the concentration at which no detectable culture outgrowth occurred after incubation, using phenol red acidification as a culture-level readout.
Because these assays measure partial metabolic inhibition versus complete suppression of detectable culture outgrowth, the corresponding concentration ranges are not expected to coincide directly. The higher concentrations observed in the right-hand panels therefore reflect the more stringent endpoint associated with complete growth inhibition rather than inconsistency between the assays.
We agree that this distinction should have been explained more clearly in the original manuscript. We have therefore substantially revised the Figure 4 legend to clarify the rationale underlying both assays, explicitly distinguish IC<sub>50</sub> and CGI endpoints, and explain how the CGI values were used to guide subsequent antibiotic selection conditions for Blastocystis ST7-B transformants. The CGI transition range has also been made more visually explicit in the revised figure presentation.
Figure 4 caption revised to: “Antibiotic potency and selection-window determination in Blastocystis ST7-B. Dose–response curves for puromycin, trimethoprim, and WR99210 were estimated from a resazurin-based viability assay (n = 3 independent replicates per drug per concentration). Points show mean ± SD, and the insets list the estimated IC50 values with R<sup>2</sup>-values > 0.75 for all fitted curves. The IC<sub>50</sub> estimates represent the drug concentrations that reduced resazurin-based metabolic activity by 50% under the assay conditions.”
Right panels: “small-culture complete growth inhibition assay using 1 × 10<sup>7</sup> WT Blastocystis ST7-B cells per culture, assayed in triplicate across a wide range of concentrations. Cultures were incubated for 2 days, and outgrowth was assessed using phenol red acidification of the medium as a culture-level readout, with yellow indicating growth and red indicating no detectable growth. The yellow-to-red transition was used to estimate the concentration required for complete growth inhibition and to guide the subsequent antibiotic selection strategy for Blastocystis ST7-B transformants.”
“IC<sub>50</sub> and CGI represent distinct assay endpoints: the former measures partial reduction in metabolic activity, whereas the latter identifies the concentration at which no detectable culture outgrowth occurs under the small-culture assay conditions.”
(6) In Figure 3B, the unexpected UnaG fluorescence pattern could be due to protein sequestration because the protein is mildly toxic to the cell. This should be discussed in addition to the reasons already provided.
We thank the reviewer for this thoughtful suggestion and agree that protein sequestration or reporter-associated cellular stress represent plausible alternative interpretations of the observed UnaG fluorescence pattern.
We considered the possibility of UnaG-associated toxicity during interpretation of these data. However, under the conditions tested, we did not observe clear evidence of a substantial toxic effect: UnaG-expressing Blastocystis ST7-B cells could be recovered as stable lines, maintained under antibiotic selection, and propagated through continued culture. We therefore felt that direct attribution of the observed fluorescence pattern to reporter toxicity would currently remain speculative.
At present, we consider the biochemical properties of the UnaG system itself to provide a more parsimonious explanation for the observed localisation pattern. In particular, unconjugated bilirubin is highly hydrophobic and would be expected to partition preferentially into lipid-rich cellular environments. This interpretation is consistent with the lipid-rich peripheral and intracellular structures previously reported in Blastocystis ST7-B (Liao et al., 2023).
We have therefore revised the Discussion to acknowledge that the observed UnaG fluorescence pattern may reflect a combination of reporter-specific biochemical behaviour, bilirubin partitioning, local intracellular environment, or possible sequestration phenomena. At the same time, we avoid assigning toxicity as a demonstrated mechanism in the absence of direct measurements of cell fitness, reporter abundance, or bilirubin distribution. Such experiments would be required to evaluate this possibility rigorously.
Lines 642-648: “Consistent with this, lipid-rich peripheral and intracellular structures have been reported in Blastocystis ST7-B, potentially providing favourable microenvironments for BR partitioning and contributing to the punctate UnaG fluorescence pattern (Liao et al., 2023). An alternative possibility is that the observed signal pattern reflects reporter sequestration or reporter-associated cellular stress. However, because UnaG-expressing lines were recovered, maintained under selection, and propagated through continued culture, toxicity remains a possible but untested explanation rather than a demonstrated mechanism.”
Minor Comments
Figure 2: Parts B and C should also show individual datapoints for better reader assessment.
We agree that inclusion of individual data points improves transparency and interpretability of the underlying data distributions.
Individual data points have now been overlaid on the boxplots in Figures 2B and 2C.
Figure 3A: Separate channels (fluorescence, bright-field, merge) should be shown rather than only the merge. The current overlay is difficult to interpret, especially for colour-blind readers.
We appreciate the reviewer’s concern regarding accessibility and interpretability. We considered separating the fluorescence, bright-field, and merged channels for Figure 3A. However, this panel was intended primarily as an overview demonstrating reporter detectability within the bicistronic construct context, while the detailed fluorescence distribution is explored more extensively in the subsequent UnaG panels. We therefore retained the merged presentation for Figure 3A. Importantly, the image is not dependent on red–green discrimination, as it combines a greyscale bright-field background with a high-contrast green/cyan fluorescence signal that remains distinguishable through brightness and contrast differences. In addition, colour-blind-friendly lookup tables (LUTs) were used throughout the revised figure set.
To further improve accessibility, the original red annotation arrow has been replaced with a colour-blind-friendly annotation colour.
Briefly define system components (P2A, UnaG, smURFP, SNAP-tag) and add an abbreviation list.
We agree that brief contextual definitions improve accessibility for readers less familiar with these reporter systems. Rather than adding a separate abbreviation list, we have added short explanatory descriptions at the points where these components are first introduced in the manuscript.
Lines 394–396: “The P2A peptide is expected to promote ribosomal skipping during translation, allowing two separate polypeptides to be produced from a single open reading frame.” Line 515–516: “UnaG, a bilirubin-binding fluorescent protein originally isolated from the muscle of the Japanese eel (Kumagai et al., 2013)…” Line 527: “smURFP (small ultra-red fluorescent protein)…”
Abstract: “among the most prevalent microbial eukaryote” should be “eukaryotes”.
Corrected in revised manuscript.
Conclusion (2nd sentence): unclear what “endogenous regulatory part discovery” means.
We agree that this phrase required clarification. The intended meaning was the identification and benchmarking of native Blastocystis ST7-B promoter and terminator elements for construct design and toolkit development. We have clarified this directly in the revised Conclusion section.
Lines 682–683 revised to: “By bringing endogenous regulatory part discovery, namely the identification of native promoter and terminator elements, …”
Author contributions: “critical advise” should be “advice”.
Corrected in revised manuscript.
Again, we thank the reviewers for their careful evaluation, constructive criticism, and thoughtful feedback on the manuscript. The review process has substantially strengthened the manuscript by helping us clarify the distinction between what is directly demonstrated experimentally and what remains mechanistically unresolved.
The central methodological conclusions of the study remain unchanged: the toolkit enables selectable transgene expression, recovery of colony-derived lines, and propagation of reporter-positive transgenic Blastocystis ST7-B lines, extending genetic accessibility in this organism substantially beyond the previous transient transfection framework.
At the same time, the revised manuscript now more explicitly acknowledges important unresolved mechanistic questions, including vector topology, P2A-mediated protein separation efficiency, and persistence in the absence of selection. These are now discussed transparently together with the future experimental approaches that will be required to address them directly.
We believe the revised manuscript now presents a clearer, more rigorous, and more accessible description of a practical genetic toolkit for Blastocystis ST7-B and hope that the revisions and clarifications satisfactorily address the reviewers’ concerns.