Catastrophic arrhythmias and sudden cardiac death can occur with even a small imbalance between inward sodium currents and outward potassium currents, but mechanisms establishing this critical balance are not understood. Here, we show that mRNA transcripts encoding INa and IKr channels (SCN5A and hERG, respectively) are associated in defined complexes during protein translation. Using biochemical, electrophysiological and single-molecule fluorescence localization approaches, we find that roughly half the hERG translational complexes contain SCN5A transcripts. Moreover, the transcripts are regulated in a way that alters functional expression of both channels at the membrane. Association and coordinate regulation of transcripts in discrete ‘microtranslatomes’ represents a new paradigm controlling electrical activity in heart and other excitable tissues.https://doi.org/10.7554/eLife.52654.001
Signaling in excitable cells depends on the coordinated flow of inward and outward currents through a defined ensemble of ion channel species. This is especially true in heart, where the expression of many different ion channels controls the spread of excitation triggering the concerted contraction of the ventricular myocardium. Even small perturbations in the quantitative balance due to block or mutations affecting a single type of channel can initiate or perpetuate arrhythmias and lead to sudden death. Repolarization is a particularly vulnerable phase of the cardiac cycle, when imbalance of inward and outward currents can prolong action potential duration and trigger arrhythmias such as Torsades de Pointes (Roden, 2016). The genetic basis of such catastrophic arrhythmias is in many cases unknown; mechanisms coordinating expression of multiple ion channels may represent novel disease targets.
Cardiac IKr is critical for normal repolarization (Sanguinetti and Jurkiewicz, 1990) and is a major target of acquired and congenital long QT syndrome (Sanguinetti et al., 1995; Trudeau et al., 1995). IKr channels minimally comprise hERG1a and hERG1b subunits (Sale et al., 2008; Jones et al., 2004), which associate cotranslationally (Phartiyal et al., 2007) and preferentially form heteromultimers (McNally et al., 2017). Underlying heteromultimerization is the cotranslational association of hERG1a and 1b mRNA transcripts (Liu et al., 2016). Because current magnitude is greater in heteromeric hERG1a/1b vs. homomeric hERG1a channels, and loss of hERG1b is pro-arrhythmic (Sale et al., 2008; Jones et al., 2014), the mechanism of cotranslational assembly of hERG subunits is important in cardiac repolarization (Liu et al., 2016).
In this study we found that association of transcripts could occur not only between alternate hERG transcripts encoded by a single gene locus, but also between transcripts encoding entirely different ion channel types whose balance is critical to cardiac excitability. Indeed, we show that SCN5A, encoding the cardiac Nav1.5 sodium channel, associates with hERG transcripts as demonstrated by co-immunoprecipitation of nascent protein in heterologous expression systems, cardiomyocytes derived from human induced pluripotent stem cells, and native human myocardium. Single-molecule fluorescent in situ hybridization (smFISH) quantitatively reveals hERG and SCN5A transcript colocalization captured during protein translation. Targeting hERG transcripts for shRNA degradation coordinately reduces SCN5A transcript levels as well, along with native IKr and INa currents recorded from cardiomyocytes. Thus, cotranslational association and regulation of transcripts is a novel mechanism establishing and preserving a balance of IKr and INa in heart, where relative levels of these currents critically determine normal action potential production and coordinated electrical activity.
Using specific antibodies that target the N-terminus of hERG1a, we purified hERG1a protein from induced pluripotent stem cell-derived cardiomyocytes (iPSC-CMs) and human ventricle lysates and performed RT-PCR to identify associated transcripts (‘RNA-IP’; Figure 1A). As previously reported (Liu et al., 2016), both hERG1a and hERG1b transcripts co-immunoprecipitated with nascent hERG1a protein. Surprisingly, SCN5A transcripts encoding Nav1.5 channels also copurified with nascent hERG1a protein (Figure 1B and Figure 1—figure supplement 1). The interaction appears specific since neither ryanodine receptor RyR2 nor inward rectifier channel Kir2.1 (KCNJ2) transcripts copurified as part of this complex. The counterpart experiment using anti-Nav1.5 antibodies confirmed association of transcripts encoding hERG1a, hERG1b and Nav1.5, but not RyR2 (Figure 1B). Bead-only controls showed no signal, indicating specific interactions of antibodies with corresponding antigens. The association also occurred in HEK293 cells, where additional controls showed that the antibodies used did not interact nonspecifically with mRNA encoding the other ion channels or subunits (Figure 1—figure supplement 1). Interestingly, when lysates independently expressing hERG1a and Nav1.5 were mixed, hERG1a antibodies copurified only hERG1a mRNA, and Nav1.5 antibodies copurified only SCN5A mRNA, indicating that association of the two mRNAs requires their co-expression in situ. In addition, the interaction between hERG1a and SCN5A does not require the presence of hERG1b (Figure 1—figure supplement 1). This experiment demonstrates that transcripts encoding hERG1a, hERG1b and Nav1.5 physically interact within the cell and can be copurified using antibodies targeting either hERG1a or Nav1.5 nascent proteins. Their association with either encoded protein implies the transcripts associate during protein translation, or cotranslationally.
To independently confirm hERG1a and SCN5A transcript association, we performed single-molecule fluorescence in situ hybridization (smFISH) experiments in iPSC-CMs (Figure 2A). We used a combination of short DNA oligonucleotides (20 nucleotides), each labeled with a single fluorophore, that bind in series on the target mRNA and collectively are detected as a single fluorescent spot (Raj et al., 2008) (see Materials and methods). Probes for hERG1a and SCN5A mRNAs were designed with spectrally separable labels for simultaneous detection (Quasar 647 and 546 respectively; see Materials and methods and Figure 2—figure supplement 1 for probe validation, and Supplementary file 1 for list of probes) (Femino et al., 1998). Punctate signal for each mRNA species appeared singly and in clusters (Figure 2A–B). To evaluate mRNA copy number in each detected signal, we fitted the histogram of the total fluorescence intensity of smFISH signals with the sum of Gaussian functions and determined mean intensity of a single mRNA molecule for each species (Figure 2B; Figure 2—figure supplements 2–3). We found that approximately 25% of detected molecules exist singly, whereas about 20% occupy clusters containing six or more transcripts (Figure 2C). Both transcripts were observed throughout the cytoplasm with higher density within 5–10 μm from the nucleus (Figure 2A and D), consistent with the expected distribution of perinuclear endoplasmic reticulum where these mRNA molecules are translated into proteins. A GAPDH mRNA probe set served as a positive control for smFISH experiments (Stellaris validated control). In contrast with signals observed for hERG1a and SCN5A transcripts, GAPDH transcript clustered less, with 50% found as single molecules and <5% in clusters of 6 or more transcripts (Figure 2C). Moreover, GAPDH molecules distributed more homogeneously throughout the cytoplasm with higher density in the range of 10 to 20 μm from the nucleus (Figure 2D). We noted similar numbers of hERG1a and SCN5A transcripts per cell but fewer than those for GAPDH (Figure 2E). Thus, numbers and spatial distribution of hERG1a and SCN5A transcripts can be simultaneously resolved. Further work will be required to elucidate the significance or possible physiological role of differently sized mRNA clusters.
Although we observed a range in numbers of hERG1a and SCN5A mRNAs among iPSC-CMs (Figure 2E), regression analysis revealed clear correlation in their expression levels within a given cell (Figure 3 and Supplementary file 2). Plotted against each other, hERG1a and SCN5A mRNA numbers exhibited a coefficient of determination (R2) of 0.57 (p=0.00001; 41 cells; Figure 3A–B). In contrast, pairwise combinations of hERG1a and RyR2, hERG1a and GAPDH, or SCN5A and GAPDH exhibited much lower linear correlation (R2 = 0.22, p=0.017; R2 = 0.18, p=0.15; and R2 = 0.33, p=0.000134 respectively; n = 26, 13, and 28 cells respectively; Figure 3C–D, Figure 3—figure supplement 1A–B, and Supplementary file 2). Spearman coefficients revealed similar results as Pearson coefficients, where significant correlation is observed only between SCN5A and hERG1a (Supplementary file 2). These findings indicate a roughly constant ratio of hERG1a and SCN5A mRNA copies.
To determine potential hERG1a and SCN5A transcript association using smFISH, we measured proximity between the two signals using the centroid position, scored from touching to 67% (1 pixel) overlap (Figure 4A–B). To discern colocalization from random overlap, we calculated the expected number of particles that could associate based on chance only for the different association criteria. Two-tailed t tests with Bonferroni correction revealed association between hERG1a and SCN5A transcripts significantly greater than that expected by chance (see Materials and methods; P values summarized in Supplementary file 3; Figure 4B). Approximately 25% of each transcript population was associated with the other (Figure 4C). To test specificity of interaction between hERG1a and SCN5A transcripts, smFISH and pairwise comparisons were also performed with RyR2 and GAPDH transcripts, which revealed no significant association (Figure 4D–E; Supplementary file 3). These results show that association of hERG and SCN5A transcripts demonstrated in lysates can also be visualized in iPSC-CMs in situ, and provide strong evidence for the existence of a discrete mRNA complex comprising hERG1a and SCN5A transcripts.
To further explore whether colocalized mRNAs were part of a translational complex, we combined smFISH with immunofluorescence using hERG1a antibodies. We observed close association between hERG1a and SCN5A mRNAs and hERG1a protein significantly greater than that expected by chance (Figure 5A–B and Figure 5—figure supplement 1A–B). Interestingly, among the 16% of actively translated hERG1a mRNAs (i.e. those associated with hERG1a protein), 46% were also associated with SCN5A mRNAs (Figure 5C), indicating a 3-fold enrichment of their association in translational complexes. Analysis of the distribution of colocalized molecules revealed that 70% are located close to the nucleus (within 10 μm, Figure 5D).
We monitored association of hERG1a protein and transcript in the presence of puromycin, which releases translating ribosomes from mRNAs (Azzam and Algranati, 1973) (Figure 6A). We observed no change due to puromycin in the total number of respective mRNAs detected per cell (Figure 6B). As expected, puromycin reduced association between hERG1a mRNA and hERG1a protein (antibody) and the S6 ribosomal protein (Figure 6C). In addition, triple colocalization of hERG1a and SCN5A transcripts and either hERG1a protein or the ribosomal subunit S6 was robustly reduced (Figure 6D). These findings further support the conclusion that hERG1a and SCN5A associate cotranslationally.
We previously demonstrated that targeted knockdown of either hERG1a or 1b transcripts by specific short hairpin RNA (shRNA) caused a reduction of both transcripts not attributable to off-target effects in iPSC-CMs or HEK293 cells (Liu et al., 2016). To determine whether hERG and SCN5A transcripts are similarly subject to this co-knockdown effect, we evaluated expression levels by performing RT-qPCR experiments in iPSC-CMs. We found that hERG1a, hERG1b and SCN5A expression levels were all reduced by about 50% upon hERG1a silencing compared to the effects of a scrambled shRNA (Figure 7A, orange bars). RYR2 transcript levels were unaffected. We observed similar results using the specific hERG1b shRNA (Figure 7A, blue bars). Expressed independently in HEK293 cells, only hERG1a mRNA was affected by the 1a shRNA, and only hERG1b was affected by the 1b shRNA (Figure 7B). SCN5A was unaffected by either shRNA, indicating that the knockdown in iPSC-CMs was not due to off-target effects and levels of associated hERG1a and SCN5A are quantitatively coregulated. Similar results of approximately 40% co-knockdown of discrete hERG1a and SCN5A mRNA particles were obtained using smFISH (Figure 7—figure supplement 1). Even more than the total population of mRNA, the number of colocalized particles is decreased by approximately 55%, indicating that physically associated transcripts are subjected to co-knockdown (Figure 7—figure supplement 1C). Together these results indicate a coordinated and quantitative regulation of mRNAs encoding a complement of ion channels.
Figure 7—source data 1
Figure 7—source data 2
Figure 7—source data 3
Figure 7—source data 4
Figure 7—source data 5
To assess functional consequences of transcript coregulation, we recorded effects of hERG1b silencing on native currents in iPSC-CMs. Figure 7C shows the repolarizing current IKr in iPSC-CMs transfected with either hERG1b or scrambled shRNA. Steady state and peak tail IKr were decreased in hERG1b-silenced cells compared to cells transfected with scrambled shRNA (Figure 7D). IKr reduction was the result of a decrease in Gmax upon hERG1b-specific silencing with no modifications in the voltage dependence of activation (Figure 7E and Supplementary file 4). These results are in accordance to our previous studies reporting a reduction in IKr density upon hERG1b-specific silencing, and indicate that transcripts targeted by shRNA are those undergoing translation (Liu et al., 2016; Jones et al., 2014). To determine whether hERG1b silencing also affects translationally active SCN5A, we measured peak INa density in iPSC-CMs and detected significant reduction of about 60% when hERG1b was silenced, compared to control cells (Figure 7F–H). Peak Gmax was decreased but no alterations in voltage dependence of activation or inactivation were detected (Figure 7H and Supplementary files 4 and 5). Late INa, measured as the current integral from 50 to 800 ms from the beginning of the pulse (Glynn et al., 2015), was similarly reduced in magnitude (Figure 7I–K). This analysis indicates that coregulation via co-knockdown results in quantitatively similar alteration of INa,late and IKr, which operate together to regulate repolarization (Banyasz et al., 2011). Ito, which does not regulate action potential duration in larger mammals (Sun and Wang, 2005), is unaffected by hERG1b silencing (Figure 8A–D), suggesting the coregulation of INa and IKr reflects their coherent participation in repolarization.
We have demonstrated using diverse and independent approaches the association and coregulation of transcripts encoding ion channels that regulate excitability in cardiomyocytes. By co-immunoprecipitating mRNA transcripts along with their nascent proteins, we have shown that hERG and SCN5A transcripts associate natively in human ventricular myocardium and iPSC-CMs as well as when heterologously expressed in HEK293 cells. Using smFISH together with immunofluorescence in iPSC-CMs, we demonstrate that the ratio of hERG and SCN5A transcripts is approximately 1:1 despite a range of pool sizes from roughly 5 to 200 molecules per cell. These transcripts colocalize about 25% of the time, but when considering only those hERG transcripts undergoing translation, nearly 50% are associated with SCN5A. When hERG1a or hERG1b transcripts are targeted by shRNA, SCN5A levels are reduced by about the same amount. Both peak and late INa are correspondingly reduced. Reflecting their coherent roles in the process of cardiac repolarization, the term ‘microtranslatome’ captures the cotranslational properties of this discrete complex comprising functionally related mRNAs and their nascent proteins.
What is the functional role of cotranslational association of transcripts? Deutsch and colleagues showed that cotranslational interaction of nascent Kv1.3 N-termini facilitates proper tertiary and quaternary structure required for oligomerization (Tu and Deutsch, 1999; Robinson and Deutsch, 2005). Cotranslational heteromeric association of hERG1a and hERG1b subunits ensures cardiac IKr has the appropriate biophysical properties and magnitude shaping the normal ventricular action potential. Coordinated protein translation of different channel types could control relative numbers of ion channels involved in electrical signaling events. Such a balance is critical during repolarization, when alterations in IKr or late INa are known to cause arrhythmias associated with long QT syndrome or Brugada syndrome (Rook et al., 1999; Bezzina et al., 1999; Bennett et al., 1995). Indeed, during normal Phase 3 repolarization, non-equilibrium gating of sodium channels leads to recovery from inactivation and re-activation of currents substantially larger than the tiny steady-state late INa observed under voltage-clamp steps (Banyasz et al., 2011; Clancy et al., 2003). Our observation of roughly equivalent hERG1a and SCN5A mRNA levels squares with previous reports of fixed channel transcript ratios associated with certain identified crustacean neurons (Schulz et al., 2007; Schulz et al., 2006). Cotranslating mRNAs in a stoichiometric manner could buffer noise associated with transcription (Dar et al., 2012) and render a stable balance of channel protein underlying control of membrane potential.
These studies raise questions of the mechanism by which transcripts associate. Although hERG1a and hERG1b N-termini interact during translation (Phartiyal et al., 2007), association of transcripts does not rely on this interaction: alternate transcripts encoding the proteins interact even when translation of one of the proteins is prevented (Liu et al., 2016). In principle, transcripts could associate via complementary base pairing or by tertiary structural interactions as ligand and receptor. Alternatively, they could be linked by one or more RNA binding proteins (RBPs). Because the association and coregulation observed in native heart can be reproduced in HEK293 cells, the same or similar mechanisms are at work in the two systems. More work will be required to discern among possible mechanisms, and to determine the time course with respect to transcription, nuclear export and cytosolic localization of interacting transcripts.
A mechanism involving RBPs is appealing because it comports with the idea of the ‘RNA regulon,’ a term describing a complex of transcripts bound by one or more RBPs (Brown et al., 2001; Keene and Tenenbaum, 2002). RBPs in the yeast Puf family bind large collections of mRNAs to control their localization, stability, translation and decay (Gerber et al., 2004; García-Rodríguez et al., 2007). In mammalian systems, the Nova protein serves to coordinate expression of mRNAs encoding splicing proteins important in synaptic function (Ule et al., 2003). Presumably in both cases these proteins interact in multiple regulons (complexes) serving different or related roles. Mata and colleagues isolated individual mRNA species in yeast and showed they associate with other mRNAs encoding functionally related (but nonhomologous) proteins, along with mRNA encoding the RBP itself (Duncan and Mata, 2011). Moreover, these mRNAs encoded proteins that formed stable macromolecular complexes (Duncan and Mata, 2014). Taking it one step further, Cosker et al. (2016) showed that two mRNAs involved in cytoskeletal regulation bind the same RBP to form a single RNA granule, possibly analogous to the microtranslatome regulating key elements of excitability in the heart reported here.
A comprehensive analysis of the microtranslatome’s components will require RNA-seq at a level of multiplexing that ensures sufficient statistical power in the face of potentially reduced complexity of the RNA-IP samples. These efforts will necessarily be followed by validation through complementary approaches such as RNAi and smFISH to confirm their identity within the microtranslatome.
One of the more curious findings of our study is the coordinate knockdown of different mRNAs in the complex by shRNAs targeted to only one of the mRNA species. The mechanism by which multiple mRNA species may be simultaneously regulated is not clear. shRNAs silence gene expression by producing an antisense (guide) strand that directs the RNA-induced silencing complex (RISC) to cleave, or suppress translation of, the target mRNA (Petersen et al., 2006; Maroney et al., 2006). Since hERG shRNA has no off-target effect on SCN5A mRNA expressed heterologously in HEK293 cells, we assume there is insufficient complementarity for a direct action. Perhaps by proximity to RISC, translation of the nontargeted mRNA is also disrupted, but to our knowledge no current evidence is available to support this idea. A transcriptional feedback mechanism seems unlikely given that co-knockdown can occur with plasmids transiently expressed from engineered promoters and not integrated into the genome of HEK293 cells. It is also important to note that it is unknown whether SCN5A is the only sodium channel transcript coregulated by hERG knockdown. In principle, transcripts encoding other sodium channels implicated in late INa, such as Nav1.8 (Yang et al., 2012; Macri et al., 2018), could also be affected, as could transcripts encoding auxiliary subunits associated with Nav1.5 (Isom et al., 1994).
Whether disrupting the integrity of these complexes gives rise to some of the many arrhythmias not attributable to mutations in ion channel genes per se remains to be determined. Although the coregulation of inward INa and outward IKr shown in this study may suggest a compensatory mechanism, in a previous study we showed that selective knockdown of hERG1b prolongs action potential duration and enhances variability, both cellular markers of proarrhythmia (Jones et al., 2014). Perhaps in the absence of co-regulation the effects would be more deleterious. Jalife and colleagues have introduced the concept of the ‘channelosome,’ a macromolecular protein complex mediating a physiological action. Interestingly, Nav1.5 and Kir2.1, which regulates resting and diastolic membrane potential, exhibit compensatory changes when the levels of either are genetically manipulated (Milstein et al., 2012). In this case, the effect seems to be on stability of the nontargeted channel proteins, which form a complex together with SAP97, and not on mRNA levels (Matamoros et al., 2016). We do not yet know whether the complex of transcripts we have studied encodes a similarly stable macromolecular complex, or perhaps ensures appropriate ratios of channels distributed independently at the membrane. Based on current evidence, we propose that the microtranslatome of associated transcripts is a novel mechanism governing the quantitative expression of multiple ion channel types and thus the balance of excitability in the cardiomyocyte.
HEK293 cells were purchased from ATCC and cultured under standard conditions (37°C, 5% CO2) in DMEM medium (Gibco) supplemented with 10% Fetal Bovine Serum (FBS, Gibco). iPSC-CMs (iCell, Cellular Dynamics International) were plated and cultured following manufacturer’s instructions. A certificate of analysis including purity and identity, sterility, mycoplasma absence, plating efficiency and viability is provided with each vial. We performed additional mycoplasma testing after plating in the laboratory. ShRNA sequences specific for hERG1a 5’-GCGCAGCGGCTTGCTCAACTCCACCTCGG-3’ and its control 5’-GCACTACCAGAGCTAACTCAGATAGTACT-3’ were provided by Origene into a pGFP-V-RS vector. shRNA specific for hERG1b 5’-CCACAACCACCCTGGCTTCAT-3’ and its respective control were purchased from Sigma-Aldrich. For heterologous expression, hERG1a (NM_000238) and hERG1b (NM_172057) sequences were cloned into pcDNA3.1. Transient transfections were performed using 2.5 µl/ml Lipofectamin 2000 (Thermofisher) with 2 µg/ml plasmid. Cells were collected for further analysis 48 hr after transfection. When needed, a second transfection was performed 24 hr after the first one with either hERG1a or hERG1b shRNA and the corresponding scrambled shRNA as a control. Cells were then collected for experiments 48 hr after last transfection.
Rabbit anti-hERG1a (#12889 from Cell Signaling, 1:100), rabbit anti-hERG1b (#ALX-215–051 from Enzo, 1:100), rabbit anti-pan hERG (#ALX-215–049 from Enzo, 1:3000), rabbit anti NaV1.5 (#ASC-005 from Alomone or #D9J7S from Cell signaling, 1:500), were used for immunofluorescence, western blot or RNA-IP experiments. Alexa 647 goat anti-rabbit, Alexa 488 goat anti-rabbit or Alexa 488 donkey anti-mouse were employed for indirect immunofluorescence or immunoblotting experiments (Thermofisher; 1:1000).
RNA isolation and purification were achieved using TriZol reagent (Life Technologies) and RNeasy Mini Kit (Qiagen). RT-qPCR experiments were performed using a TaqMan Gene Expression Assay (Life Technologies) and mRNA expression levels were calculated using the 2-ΔΔCt cycle threshold method. All data were normalized to mRNA level of β-actin housekeeping genes. Because iPSC-CMs are subject to inherent biological variability, we used a standardization procedure to normalize the independent biological replicates as previously described (Willems et al., 2008). Briefly, a log transformation of the normalized relative expression gene level was performed, followed by mean centering and autoscaling of the data set. Results are expressed as average and 95% confidence intervals. Primers were purchased from Invitrogen (hERG1a: Hs00165120_m1; hERG1b: Hs04234675_m1; SCN5A: Hs00165693_m1; RYR2: Hs00892883_m1; and β-actin: Hs01060665_g1).
For immunofluorescence studies, iPSC-CMs were grown on gelatin-coated coverslips, rinsed in PBS three times and fixed in 4% paraformaldehyde for 10 min at room temperature. Following fixation, cells were incubated 1 hr at room temperature with a solution containing 0.5% triton X-100 for permeabilization and 1% bovine serum albumin along with 10% serum (secondary antibodies species) diluted in PBS to saturate samples and limit nonspecific binding. Cells were then processed for indirect immunofluorescence using a combination of primary and secondary antibodies (see antibodies section above). Cells were washed three times with PBS, incubated with DAPI to counterstain nuclei and mounted with Vectafield mounting medium.
FISH was performed using Stellaris probe sets, which comprised up to 48 oligonucleotides designed to selectively bind in series the targeted transcripts. Probes were designed using the StellarisTM Probe Designer by LGC Biosearch Technologies with the following parameters: masking level: 5, oligo length: 20 nucleotides, and minimum spacing length: two nucleotides. Oligonucleotides were labeled with TAMRA or Quasar 670 dyes for detection of SCN5A and hERG respectively. 48 oligonucleotides were designed for SCN5A, RyR2 and GAPDH and 35 for the specific N-terminal sequence of hERG1a. Sequences for all probes are provided in Supplementary Table 1. FISH was performed on iPSC-CMs according the manufacturer’s protocol. Briefly, fixation was performed by adding paraformaldehyde to a final concentration of 4% (32% solution, EM grade; Electron Microscopy Science) followed by a hybridization step for at least 4 hr at 37°C in a buffer containing a final concentration of 125 nM probes and 10% formamide (Stellaris hybridization buffer). Cells were washed for 30 min (Stellaris washing buffer A) before incubation for 30 min at 37°C with DAPI to counterstain the nuclei. A final washing step was performed (Stellaris washing buffer B) and coverglasses were mounted onto the slide with Vectashield mounting medium.
Digital images were acquired using a 63X objective on a Leica DMi8 AFC Inverted wide-field fluorescence microscope. Z-sections were acquired at 200 nm intervals. Image pixel size: XY, 106.3 nm. Image post-treatments were performed using ImageJ software (NIH). Briefly, a maximum projection was performed before background subtraction and images were filtered using a Gaussian blur filter to improve the signal/noise ratio and facilitate spot detection. Spot detection and colocalization was performed using the plugin ComDet on ImageJ (Chang et al., 2006; Hoffman et al., 2001).
FISHQUANT was used as a second method for spot detection and gave similar values. Briefly, background was substracted using a Laplacian of Gaussian (LoG) and spots were fit to a three-dimensional (3D) Gaussian to determine the coordinates of the mRNA molecules. Intensity and width of the 3D Gaussian were thresholded to exclude non-specific signal (Raj et al., 2008; Femino et al., 1998).
To evaluate the number of mRNA molecules, the total fluorescence intensity of smFISH signals was fitted with the sum of Gaussian functions (see equation below) to determine the mean intensity of a single mRNA.
For the purpose of our statistical calculations, we assumed that the protein and mRNA signals were circular. The following formulas were used to calculate the expected number of mRNAs (Em) that would interact based on chance alone for each association criteria:
where Nm1 is the total number of mRNA in one channel, Nm2 is the total number of mRNA in the second channel, r is the average radius of mRNA spots (in nm), I is the intersection between particles (nm2, and A is the total area of the region analyzed (in nm2. As the distance between particles is increased, the number of expected associated mRNAs will increase since more mRNAs will be considered associated. We used criteria with different stringency in the first set of experiments (from 1 pixel to four pixels distance between spots) and considered the two pixels distance between spots physiologically relevant for triple association analysis and co-knockdown experiments.
To test the significance of triple associations between hERG1a mRNA, SCN5A mRNA and hERG1a protein, the following formula was used:
where Np is the total number of proteins, Em is the expected number of mRNA that would interact based on chance alone as calculated above. For each association criteria, the intersection between particles was calculated using the following equation:
mRNA numbers were plotted against each other from different combinations of smFISH signals as scatter plots. Then Pearson’s and Spearman’s correlation coefficients were evaluated to assess correlation between considered mRNA species.
The following equation was used to calculate Pearson’s coefficient R and determine the coefficient of determination R2 from the mRNA pairs :
where is the covariance of the values and is the difference between the standard deviation of the values. Significance was determine using a F test.
The Spearman’s coefficient ρ was determined on ranked values Xi and Yi using the following equation:
where is the covariance of the rank values and is the difference between the standard deviation of the ranked values. Significance was determine using two-tailed probability test.
Ribonucleoprotein (RNP) complexes were isolated with a RiboCluster Profiler TM RIP-Assay Kit (Medical and Biological Sciences) using protein-specific antibodies and Ab-immobilized A/G agarose beads. After formation of the RNP/beads complex, we used guanidine hydrochloride solution to dissociate beads from RNP complexes. Finally, target RNAs were analyzed using RT-PCR.
Patch clamp under whole-cell configuration was used to record all ionic currents. IKr and INa,late were recorded at physiological temperatures (37°C), while INa was recorded at room temperature (22°C) using an Axon 200B amplifier and Clampex Software (Molecular Devices). Glass pipettes with a resistance of 2.5–5 MΩ measured with physiological solutions (below) were pulled using an automatic P-97 Micropipette Puller system (Sutter Instruments).
To record steady state and tail IKr, cells were continuously perfused with an external solution containing (in mM): NaCl 150, KCl 5.4, CaCl2 1.8, MgCl2 1, Glucose 15, HEPES 15, Na-pyruvate 1, and the pH was adjusted to 7.4 with NaOH. Pipettes were filled with an internal solution containing (in mM): NaCl 5, KCl 150, CaCl2 2, EGTA 5, HEPES 10, Mg-ATP 5, and the pH was adjusted to 7.3 with NaOH. The voltage protocol for IKr was completed at physiological temperature (37°C) and determined as an E-4031 (2 μM) sensitive current. Cells were recorded using a holding potential of −50 mV, followed by a pulse at −40 mV to inactivate sodium channels, then 3 s depolarizing steps (from −50 to +30 mV in 10 mV increments) to activate hERG channels and finally to −40 mV for 6 s. Steady-state IKr was measured as the 5 ms average current at the end of the depolarizing steps. Tail currents were measured following the return to −40 mV.
To record INa, cells were perfused with an external solution containing (in mM): NaCl 50, Tetraethylammonium (TEA) methanesulfonate 90, CaCl2 2, MgCl2 1, Glucose 10, HEPES 10, Na-pyruvate 1, Nifedipine 10 μM, and pH adjusted to 7.4 with TEA-OH. Micropipettes were filled with an internal solution containing (in mM): NaCl 10, CaCl2 2, CsCl 135, EGTA 5, HEPES 10, Mg-ATP 5, and pH was adjusted to 7.3 with CsOH.
INa activation was investigated by applying pulses between −140 and +20 mV in 10 mV increments from a holding potential of −120 mV. To measure inactivation of sodium channels, conditioning pulses from −140 to +20 mV in 10 mV increments were applied from a holding potential of −120 mV following by a test pulse to −20 mV.
To record INa,late, cells were perfused with an external solution containing (in mM): NaCl 140, CsCl 5.4, CaCl2 1.8, MgCl2 2, HEPES 5, Nifedipine 10 μM, and pH was adjusted to 7.3 with NaOH. Pipette were filled with an internal solution containing (in mM): NaCl 5, CsCl 133, Mg-ATP 2, TEA 20, EGTA 10, HEPES 5, and pH was adjusted to 7.33 with CsOH. INa,late was measured by applying an 800 ms single pulse to −30 mV from a holding potential of −120 mV. Late INa was measured as the current integral from 50 to 800 ms from the beginning of the pulse.
To record Ito, cells were continuously perfused with an external solution containing (in mM): NaCl 150, KCl 5.4, CaCl2 1.8, MgCl2 1, Glucose 15, HEPES 15, Na-pyruvate 1, E4031 2, CdCl2 0.5 and the pH was adjusted to 7.4 with NaOH. Pipettes were filled with an internal solution containing (in mM): NaCl 5, KCl 150, CaCl2 2, EGTA 5, HEPES 10, Mg-ATP 5, and the pH was adjusted to 7.3 with NaOH.
Both activation (for IKr, Ito and INa) and inactivation (for INa) were fitted to Boltzmann equations (Equations (1) and (2), respectively) and voltage dependence parameters were obtained.
All data generated or analysed during this study are included in the manuscript and supporting files. Source data files have been provided for all figures.
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Cardiac IKr channels minimally comprise hERG 1a and 1b subunitsThe Journal of Biological Chemistry 279:44690–44694.https://doi.org/10.1074/jbc.M408344200
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Heteromeric assembly of human ether-à-go-go-related gene (hERG) 1a/1b channels occurs cotranslationally via N-terminal interactionsJournal of Biological Chemistry 282:9874–9882.https://doi.org/10.1074/jbc.M610875200
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Two components of cardiac delayed rectifier K+ current. differential sensitivity to block by class III antiarrhythmic agentsThe Journal of General Physiology 96:195–215.https://doi.org/10.1085/jgp.96.1.195
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Richard AldrichSenior and Reviewing Editor; The University of Texas at Austin, United States
In the interests of transparency, eLife publishes the most substantive revision requests and the accompanying author responses.
The paper demonstrates a regulatory mechanism for maintaining the homeostatic "balance" between sodium and potassium channels in heart tissue, where imbalance can lead to dangerous arrhythmias. Transcripts of ERG potassium and Nav1.5 sodium channels are colocalized and cotranslated, which helps maintain a safe ratio of the depolarizing sodium and the hyperpolarizing potassium channels.
Decision letter after peer review:
The previous reviews from another journal have been considered and evaluated along with the manuscript by an expert Reviewing Editor, who has the following comments:
"On one hand, I think the reviewers did an excellent job and identified shortcomings preventing the ability to come to clear and definite conclusions, but on the other hand, the work, as one of the reviewers noted, is thought provoking and as such does it really need to dot every “i” and cross every “t”? I think if the authors would point out in the Discussion that for technical reasons, they were unable to do the RNAseq and similarly for the other really technically difficult points, it would be okay. They are being very honest in what they have confidence in and what not, more than I can say for many other papers. So, I would accept it with minor revisions, especially in discussion to qualify their conclusions, and let people make up their own minds. It is fun to read something a little bit different."https://doi.org/10.7554/eLife.52654.051
We have submitted our revised manuscript entitled “A microtranslatome coordinately regulates sodium and potassium currents in the heart” for review at eLife. We have provided reviews and responses from another journal to assist in eLife’s consideration of our manuscript for publication.
This manuscript describes for the first time the cotranslational association and coregulation of mRNA transcripts encoding different ion channels species. The balance of ion currents that generate electrical impulse is essential for proper function in excitable cells. The observation that transcripts associate and are coregulated via a “microtranslatome” may represent a general mechanism by which cells coordinate expression and thus activity of functionally related proteins. Thus the primary audience will be those interested in a new mechanism by which multiple conductances are coordinately regulated at the level of protein translation. We received the editorial suggestion from Dr Aldrich to acknowledge the difficulty of conducting RNA-seq analysis as part of this study and have now revised the manuscript to include the following text in the Discussion: “A comprehensive analysis of the microtranslatome’s components will require RNA-seq at a level of multiplexing that ensures sufficient statistical power in the face of potentially reduced complexity of the RNA-IP samples. These efforts will necessarily be followed by validation through complementary approaches such as RNAi and smFISH to confirm their identity within the microtranslatome.”
[Editors' note: we include below the reviews that the authors received from another journal, along with the authors’ responses.]
We appreciate the opportunity to improve our manuscript per the critiques of the reviewers and editor. A major concern by the reviewers and reiterated by the editor was whether the association of transcripts was cotranslational. As described below we have carried out experiments using puromycin showing dissociation of the complexes and providing a third line of support for the cotranslational basis of hERG1a and SCN5A transcript association. Despite our best attempts not all the suggestions were fulfilled, as detailed below, but we hope you agree that the manuscript has been significantly improved as a result of the key experiments completed.
1) Please note that we do not think that identifying proteins within the 'translatome' through mass spectrometry as suggested by reviewer 1 (point 2) is necessary. However we do feel that attempting to identify the RNA content through non-biased sequencing (RIP-Seq or similar approach rather than just targeted PCR) would significantly increase confidence in the original result. Given that the conditions for immunoprecipitation have already been worked out, this should be quite feasible within the timeframe of a regular revision, and we therefore consider this demand within the scope of the current manuscript.
RNA-seq analysis has been a vexing aspect of this project. We carried out a detailed study that produced confusing (and expensive) results. Upon attempting to repeat the study, a new campus core with greater bioinformatics and study design expertise than the company we originally used suggested that our results were likely hampered by random variation that arises with libraries of reduced complexity, such as those expected of our microtranslatome complex. To carry out the experiment again will require many more replicates to mitigate this problem and will be extremely expensive. We believe that with the addition of the puromycin perturbation our results demonstrating the presence of the hERG mRNA in the complex via RT-PCR, smFISH, and co-knockdown are now quite compelling.
2) Addressing reviewer 1's point 4 experimentally will also be necessary.
We agree and please see our response under reviewer 1, point 4.
3) In regard to reviewer 2's comments, we agree that several of the experiments lack adequate controls, which should be remediated. We also agree with this reviewer that evidence the association occurs co-translationally is currently lacking and must be provided.
As described below, we have carried out experiments with puromycin to disrupt the interaction between the ribosomes and mRNA, and report in Figure 6 the results that the antibody and smFISH signals are dissociated as would be expected from a cotranslational complex.
This is a well-written, thought-provoking and novel study with potential for significant impact to the field. I only have a few comments.
1) It seems to me that with not much additional effort the investigators can describe more than two transcripts in these complexes. Could it be possible to run an RNA-seq on the precipitates to know what else, in addition to the two transcripts described, is present?
We have identified other elements in the precipitate using a candidate approach and are sorting out whether they are components of the same or different microtranslatomes. This is a challenging task that requires multiplexed co-knockdowns and smFISH experiments with each component. We are currently approaching this challenge as a different project that is the thesis project of one of my students, who has just begun these experiments. Also, as mentioned above, RNA-seq of the microtranslatome, which we attempted, produced confusing results and will require a more sophisticated and expensive approach than is required with, e.g., a whole-cell or tissue sample. Even if we did obtain a list of other interacting mRNAs we hope the reviewer will agree that the level of work required to prioritize the candidates and validate their association with the complex will require much work beyond the scope of the current project.
2) Similar to the comment above: A proteomic analysis of these precipitates would identify other proteins whose transcripts may also be present (as per the RNA-seq experiment suggested above) as well as (and perhaps more importantly) which known RNA-binding proteins are present in the complex that may be acting to form the complex.
We agree with the reviewer that the results from a proteomic analysis will be extremely important, but as the editor suggested, this experiment is beyond the scope of the current study. Indeed, this is currently the sole project of a postdoctoral fellow in the lab. Again, validation of each protein component, such as RNA binding proteins, will require a tremendous effort to demonstrate their functional roles.
3) And from both points above: I am not too keen on the term “excitotranslatome.” It unnecessarily limits the relevance of the findings to the context of electrical excitability. These complexes may cover more than just one function. Yet again, this is only an opinion (the authors discovered them so of course, they should be free to name them…)
We agree with this viewpoint and now term the complex a “microtranslatome.” We have changed the title accordingly to: “A microtranslatome coordinately regulates sodium and potassium currents in the heart.”
4) Some of the speculation in the Discussion section would presume that the co-translation also leads to equivalent amounts of functional channels. It would be interesting to prove the latter. Do current amplitudes correlate on a cell-by-cell bases? Are these proteins (HERG and Nav1.5) co-localizing at the cell membrane? If you were to do a macropatch of the cell surface, would you be able to record both channels under the same small patch?
Whether the channel expression is quantitatively correlated is an important test of our central hypothesis and we thank the reviewer for this suggestion. We recorded IKr and INa current amplitudes simultaneously in the same cell as shown in Author response image 1. We did not uncover a strong correlation between IKr and peak INa current densities on a cell-by-cell basis (R2=0.28), but we have little confidence in the outcome of this experiment because IKr is extremely small relative to the noise and thus difficult to reliably quantify on a cell-by-cell basis. In the future we hope to quantify these currents in native, mature cardiomyocytes in which the currents are larger and correlations between IKr and late INa can be made.
The assessment of protein colocalization at the cell membrane would have been an interesting complement to confirm this correlation. Unfortunately, despite much effort put towards identifying antibodies produced in different species required for colocalization in immunofluorescence experiments, none gave sufficiently specific signals for hERG or NaV1.5 proteins. Work along this line continues in the lab.
Macropatch would be an elegant approach to identify a functional proximity of IKr and INa channels. Unfortunately, while sodium current is big enough to be recorded in macropatch configuration in iPSC-CMs, the same is not true for IKr, which is only 4-5 pA/pF in whole-cell configuration.
Other minor comments:
Figure 1: Isolated examples are presented. A measure of reproducibility should be provided. This applies particularly to the human LV and the iPSC-CM samples: How many different hearts investigated? How many clones of hIPSC-CMs? How many repeats?
Thank you for noticing this oversight. We purchased iPSC-CMs from Cellular Dynamics International (CDI) and those cells are derived from a single clone. They are reliable and consistent between batches, but multiple clones are unavailable. We now state the N for independent experiments for iPSC-CMs and human LV in the Figure 1 legend.
“In a series of 35 or 48…” What does the 35 or 48 refer to?
These values refer to the number of probes in sequence used for the smFISH experiments. These values have been removed from the text and clarified in the Materials and methods to avoid confusion.
Figures 2-3: Same as Figure 1: number of repeats? N values?
The n values have been added for each experiment directly on the graph or in the legend for each figure.
Figure 3: It would be interesting to see the complementary plot: SCN5A versus RyR2.
These probes were ordered with the same fluorophore in the original study and were therefore not distinguishable under the microscope. Unfortunately, we overlooked this suggestion until very recently and to avoid further delay we hope that the reviewer will agree that although this is interesting, it is not absolutely necessary to complete the study.
Figures 4B and 4E: Are the units in the X axis correct (micrometers)?
Thank you for this careful observation. This error has been corrected in the figure.
In this manuscript, the authors study the co-translational assembly of mRNAs that encode two different ion channels (INa and IKr) that are encoded by SCN5A and hERG in iPSC cardio myocytes. The association of the two mRNAs is first shown by RIP experiments and then further evaluated by smFISH and smFISH+IF for the hERG1a protein. Interestingly, RNAi knockdown of hERG1 mRNA also results in a depletion of SCN51 mRNA suggesting a connection between the stabilities of their transcripts by their association. The authors also show test the physiological consequence of this co-depletion by electrophysiology measurements.
In general, the work is interesting and addresses an important question in the field. The work would benefit from several controls in order to strengthen their assertion that these affects are occurring via co-translation.
The authors thank the reviewer for the expression of enthusiasm regarding the work’s significance. We recognize the primary concern is whether the phenomena and effects observed are cotranslational and will address this concern among the other comments as well.
1) Figure 1B is very dense and difficult to interpret. It would be better to separate out results from iPSC-CMs and HEK ectopic-expression. It is also not clear why RyR2 was also not overexpressed in HEK cells. The negative data for KCNJ2 can probably be moved to supplemental as well as IgG control data. Are these interactions puromycin-sensitive? I think this is a key control that is missing throughout the manuscript and should be performed for all of the smFISH studies as well.
We have revised the gel per the reviewer’s suggestion and included the previous, more complete gel in the supplement for those wanting to see all the controls within a single experiment. The RYR2 was not expressed heterologously because we were unable to express the available construct and therefore relied on natively expressed RYR2 in heart and iPSC-CMs, but we did not feel this affected the conclusion that the RYR2 is not a component of the microtranslatome. Having a negative control (KCNJ2) throughout the experiment is important to show that the IP is specific, so we kept this in Figure 1.
We have carried out experiments using puromycin and now show in Figure 6 that the association of hERG1a and SCN5A mRNAs with hERG protein is robustly reduced by the treatment, providing another line of support for the cotranslational association of the transcripts.
2) It is not clear what is the importance of these clusters as they are not mentioned again? Are the clustered puro-sensitive? Do they require active translation to form or is that just clustering on the ER somehow? Have the authors considered mild-digitonin extraction to remove cytosolic mRNAs and to leave behind ER- localized ones as described here (PMID: 23271194)?
Please see response to point 4 below.
3) GAPDH is not a good control for their experiments since it encodes a cytosolic protein that does not translate to high levels on the ER. The RyR2 transcript is much better since it encodes also encodes a membrane protein. I would either remove all GAPDH data or move to supplemental since its comparison is almost meaningless for what they want to show.
We value the information provided by the GAPDH signal precisely because it represents a transcript with a completely different type of distribution; not only is it distributed differently from the channel transcripts, but it is also abundant, in contrast to the rarer channel transcripts. In addition, the GAPDH probes are validated by Stellaris, adding another measure of certainty regarding signal identification.
4) The authors show that about 25% of transcripts co-localize. Is this different for single or clustered transcripts?
We carried out an analysis of all transcripts expressed in cells and found no major change in distribution in clusters with puromycin treatment (Author response image 2A). When considering colocalized transcripts specifically, we found that colocalized hERG1a and SCN5A mRNAs are preferentially found in pairs of single molecules (32% and 36% of hERG1a and SCN5A transcripts respectively) or organized in clusters of 6 or more molecules (27% and 23% for hERG1a and SCN5A mRNAs respectively; Author response image 2B and C). Interestingly, puromycin treatment shifted these proportions towards association in clusters of 6 or more molecules suggesting that ribosomes are involved in the association of transcripts found as single molecule. We could speculate on the significance of this finding, but feel these observations raise many more questions than they answer and plan to use these findings as the basis for a new study. We now note in the manuscript that “Further work will be required to elucidate the significance or possible physiological role of differently sized mRNA clusters” so as to acknowledge the unanswered question.
Given the similar transcripts numbers, I do not understand the different expected co-localization numbers in Supplementary file 2. I would assume that the other parameters are identical.
The reviewer is right about the numbers of transcripts being similar for hERG and SCN5A mRNAs, but the parameter being modified is how much overlap there is between colocalized particles. Thus, the 1 pixel distance between center of mass (67% of the two spots overlapping) will consider a smaller number of particles as colocalized than 4 pixels (when spots touch each other). We modified the Materials and methods in order to clarify this point.
5) As it is not clear if the protein detected is nascent on polysomes or mature, I think it is not very strong evidence that this occurring co-translational. Is this sensitive to puro?
Evidence that transcripts associate cotranslationally has been clarified in the manuscript and can be summarized as follows: 1) The co-purification of transcripts with protein in the RNA-IP experiments implying that they are undergoing translation; 2) the co-knockdown of transcripts undergoing translation (as shown by quantitative RT-PCR and patch clamp analysis of currents); and 3) new data provided in Figure 6 showing a reduction of association of transcripts with hERG1a protein in the presence of puromycin.
6) This analysis would be more interesting with smFISH. Are they degrading the mRNAs that co-localize or do not co-localize or both? This might help them distinguish between possible models for this co-depletion.
We carried out the co-knockdown experiment using smFISH as suggested by the reviewer and it is now presented in Figure 7—figure supplement 1 and described in the manuscript. We observed that numbers of hERG1a and SCN5A mRNAs are decreased upon hERG1b-specific silencing (Figure 7—figure supplement 1B) as is the number of colocalized particles (Figure 7—figure supplement 1C). This observation supports the existence of a mechanism that controls the relative quantity of those two transcripts, as stated in the manuscript.
1) Please define iPSC-CM the first time it is used.
This has been added to the manuscript.
2) Figure 4B and E – distance should be in nm.
This has been corrected.https://doi.org/10.7554/eLife.52654.052
- Gail A Robertson
- Erick B Rios-Pérez
- Jennifer J Knickelbine
The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.
Research reported in this publication was supported by the National Heart, Lung and Blood Institute of the National Institutes of Health R01HL131403. The authors thank Dr. Peter Mohler of the Dorothy Davis Heart and Lung Institute for heart samples and Drs. Barry Ganetzky of the University of Wisconsin-Madison, Andrew Harris of the Rutgers New Jersey Medical School and Drs. Cynthia Czajkowski and Baron Chanda of the University of Wisconsin School of Medicine and Public Health for comments on an earlier version of the manuscript.
- Richard Aldrich, The University of Texas at Austin, United States
© 2019, Eichel et al.
This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.
In the adult Drosophila midgut, basal intestinal stem cells give rise to enteroblasts that integrate into the epithelium as they differentiate into enterocytes. Integrating enteroblasts must generate a new apical domain and break through the septate junctions between neighbouring enterocytes, while maintaining barrier function. We observe that enteroblasts form an apical membrane initiation site (AMIS) when they reach the septate junction between the enterocytes. Cadherin clears from the apical surface and an apical space appears between above the enteroblast. New septate junctions then form laterally with the enterocytes and the AMIS develops into an apical domain below the enterocyte septate junction. The enteroblast therefore forms a pre-assembled apical compartment before it has a free apical surface in contact with the gut lumen. Finally, the enterocyte septate junction disassembles and the enteroblast/pre-enterocyte reaches the gut lumen with a fully-formed brush border. The process of enteroblast integration resembles lumen formation in mammalian epithelial cysts, highlighting the similarities between the fly midgut and mammalian epithelia.
Major genomic deletions in independent eukaryotic lineages have led to repeated ancestral loss of biosynthesis pathways for nine of the twenty canonical amino acids1. While the evolutionary forces driving these polyphyletic deletion events are not well understood, the consequence is that extant metazoans are unable to produce nine essential amino acids (EAAs). Previous studies have highlighted that EAA biosynthesis tends to be more energetically costly2,3, raising the possibility that these pathways were lost from organisms with access to abundant EAAs in the environment4,5. It is unclear whether present-day metazoans can reaccept these pathways to resurrect biosynthetic capabilities that were lost long ago or whether evolution has rendered EAA pathways incompatible with metazoan metabolism. Here, we report progress on a large-scale synthetic genomics effort to reestablish EAA biosynthetic functionality in mammalian cells. We designed codon-optimized biosynthesis pathways based on genes mined from Escherichia coli. These pathways were de novo synthesized in 3 kilobase chunks, assembled in yeasto and genomically integrated into a Chinese Hamster Ovary (CHO) cell line. One synthetic pathway produced valine at a sufficient level for cell viability and proliferation, and thus represents a successful example of metazoan EAA biosynthesis restoration. This prototrophic CHO line grows in valine-free medium, and metabolomics using labeled precursors verified de novo biosynthesis of valine. RNA-seq profiling of the valine prototrophic CHO line showed that the synthetic pathway minimally disrupted the cellular transcriptome. Furthermore, valine prototrophic cells exhibited transcriptional signatures associated with rescue from nutritional starvation. 13C-tracing revealed build-up of pathway intermediate 2,3-dihydroxy-3-isovalerate in these cells. Increasing the dosage of downstream ilvD boosted pathway performance and allowed for long-term propagation of second-generation cells in valine-free medium at a consistent doubling time of 3.2 days. This work demonstrates that mammalian metabolism is amenable to restoration of ancient core pathways, paving a path for genome-scale efforts to synthetically restore metabolic functions to the metazoan lineage.