Thank you for visiting nature.com. You are using a browser version with limited support for CSS. To obtain the best experience, we recommend you use a more up to date browser (or turn off compatibility mode in Internet Explorer). In the meantime, to ensure continued support, we are displaying the site without styles and JavaScript.

# Impact of wet-dry cycling on the phase behavior and compartmentalization properties of complex coacervates

## Abstract

Wet-dry cycling on the early Earth is thought to have facilitated production of molecular building blocks of life, but its impact on self-assembly and compartmentalization remains largely unexplored. Here, we investigate dehydration/rehydration of complex coacervates, which are membraneless compartments formed by phase separation of polyelectrolyte solutions. Solution compositions are identified for which tenfold water loss results in maintenance, disappearance, or appearance of coacervate droplets. Systems maintaining coacervates throughout the dehydration process are further evaluated to understand how their compartmentalization properties change with drying. Although added total RNA concentrations increase tenfold, RNA concentration within coacervates remains steady. Exterior RNA concentrations rise, and exchange rates for encapsulated versus free RNAs increase with dehydration. We explain these results in light of the phase diagram, with dehydration-driven ionic strength increase being particularly important in determining coacervate properties. This work shows that wet-dry cycling can alter the phase behavior and protocell-relevant functions of complex coacervates.

## Introduction

The potential of the wet-dry cycle to promote molecular complexity on the early Earth is increasingly supported by experiments1,2,3. Dehydration–rehydration periods are suggested to be driven not only by thermal evaporation but also by environmental phenomena, such as geyser activity, rainfall4,5, and salt deliquescence6. Even in the absence of catalysts, the wet-dry cycle has been shown to lower the thermodynamic barrier in the formation of polyacids7, esters1,2, oligopeptides8,9,10, nucleosides3, and polynucleotides11,12—molecular building blocks of life. Theoretical simulations have been proposed to explain the effects on reactivity13,14, while streamlined experimental setups are being explored for a better control of the process9,15. Despite the likelihood of prebiotic wet-dry cycling and its demonstrated benefits for polymerization reactions11,12,16, reports of its impact on molecular self-assembly and compartmentalization have thus far been restricted to lipid vesicles17,18,19.

Membraneless compartments, such as those produced by complex coacervation and other forms of liquid–liquid phase coexistence, are vigorously investigated for their potential to concentrate molecules and assist reactivity20,21,22,23,24,25. Complex coacervates result from associative charge-driven assembly of oppositely charged macromolecules26. The concentrated phase can form droplets when suspended in solution. With its crowded yet hydrated interior, it is a promising protocell candidate24,27 that can amass significant concentrations of (bio)molecules22,24,28 and host enzymatic reactions20,21,23,29,30. Extant cells benefit from related functions as coacervation is implicated in forming membraneless organelles29,31,32.

The impact of wet-dry cycling on complex coacervate compartments is yet to be explored. This process affects a key player in these systems, water, which has a central role in determining the structure and behavior of coacervates33. Beyond the hydrophilic or hydrophobic aspects of the constituents, which affect phase separation34, the coacervate salt content can also impact water retention35,36,37. The phase behavior of these systems can be described by diagrams such as ones that relate the polymer concentration in the mixture to that of the salt38,39. Choosing a composition is the same as selecting a location on the phase diagram. For specific applications, this choice is often empirical, usually done based on the desired outcome or function of the coacervate in the context of the study. However, these compartments are responsive to environmental variables, such as the ionic content of the solution33, pH40, temperature41,42, and different methods of preparation23,33,43, which alter inter and/or intramolecular interactions responsible for liquid–liquid phase separation. Using coacervate systems as models of protocells requires, therefore, taking into consideration the possible changes to the prebiotic environment around them. Beyond prebiotic research, understanding the impact of significant hydration fluctuations on coacervates is of interest to their different applications as adhesives44, in food systems45, and drug delivery46, as the properties of these materials are intimately related to their water content33.

Here, we examined the effects of wet-dry cycling on the composition, structure, and behavior of a model complex coacervate system. We chose to focus on understanding the impact on compartmentalization, one of the central functions of coacervates24,47. While previous studies have focused on how increases in either salt or polymer influence complex coacervates38,42, water loss during drying presents an unusual problem as it concentrates both salts and polymers simultaneously. We found that dehydrating a coacervate mixture decreases the potential of the polymer-rich phase to partition an RNA oligonucleotide, and enhances its diffusion. This was followed by experiments on mimics that had the same concentrations of the components during drying steps, which related the observations to the phase behavior of the complex coacervate.

## Results

### Drying and rehydration controls coacervate formation

To investigate the wet-dry cycling of complex coacervates (Fig. 1a), we chose a widely studied polyelectrolyte pair, the poly(diallyldimethylammonium) PDADMA/poly(acrylic acid) PAA system with around 53 repeating units for the polycation and on average 25 for the polyanion. To the macromolecules, sodium chloride, magnesium chloride, and HEPES buffer were added (see Supplementary Note 1 for details on choosing the system and environment). While wet-dry cycling can occur in various locations, our inspiration was the fresh water of a terrestrial pond (Supplementary Note 1)5. Samples were dried using a heatblock at 95 °C, a temperature chosen for quicker evaporation. Supplementary Note 2 and Supplementary Figs. 14 detail the drying process and setup, the measurement of the evaporation rate, and the nonimpact of the temperature on the existence of the coacervate. To limit the focus to polymer and salt effects while drying, initial HEPES and magnesium concentrations were fixed at 2.5 and 0.43 mM, respectively. The starting values were chosen as to sustain the pH and not have an impact on phase separation (see Supplementary Note 3, Supplementary Figs. 5 and 6 for details).

We began by mapping the phase diagram at 1:1 PDADMA:PAA to delimit the approximate boundary between the two-phase and one-phase regimes using a combination of turbidity measurements and optical microscopy (Fig. 1b, Supplementary Figs. 7 and 8). Several initial compositions, noted on the diagram as i (filled triangle), ii (filled square), iii (filled diamond), were chosen for the investigation. Concurrent increases in all solute concentrations as water evaporates were expected to yield different diagonal shifts in compositions on the phase diagram depending on the starting composition (see dashed lines in Fig. 1b). Dehydration by ~10-fold impacted phase behavior differently for the three initial compositions.

The further the composition was on the left of the turbidity graph in Fig. 1b, a wider range of the two-phase region, where droplets exist, would be afforded to travel rightward and upward on the diagram as the concentrations of NaCl and polymers increase with water evaporation. Open markers (i (open triangle), ii (open square), iii (open diamond)) show the expected final locations of the dried samples. As seen in Fig. 1c–i, an appropriate composition which sustained droplet formation over the whole range was: 5 mM monomer charge, 5 mM NaCl, 2.5 mM HEPES, 0.43 mM MgCl2 (Supplementary Note 4). This composition was used for most of the following experiments, unless otherwise stated. Choosing a more concentrated composition eventually caused a dissolution of the droplets as the mixture extended beyond the two-phase region of the plot (Fig. 1c-ii). Numerous studies have shown that coacervates dissolve when conditions are pushed beyond the two-phase region. This was observed micro- and macroscopically33,39, and has been driven actively through enzymatic reactions29,48. A less concentrated point provided coacervates that would start with low turbidity (small dispersed droplets), which increased with drying as droplets grew in volume (Fig. 1c-iii, Supplementary Fig. 8). In each of the three cases, the initial composition/morphology appeared to be regained once the sample was rehydrated with a volume of water equivalent to the starting point (Fig. 1c–i–iii), or gradually (Fig. 1c-iv). Coacervate aging for 24 h, without drying, did not appear to affect its morphology when resuspended (Supplementary Fig. 9). Dry samples were also imaged in different conditions (Supplementary Note 4, Supplementary Fig. 10). We note that changes to the overall sample composition alter the relative amounts and compositions of its polymer-rich phase and dilute phase;38 a simple schematic for how these changes are anticipated to impact a generic coacervate system is provided in Supplementary Fig. 11. Further analysis on these changes and their repercussions is presented below.

Together these results showed that it is possible to travel into and out of the two-phase region during drying, underscoring the importance of knowing the coordinates of each system, and supporting the predictability of the wet-dry cycle’s impact on the phase behavior of coacervates—a topic that will be further explored here. Next, we chose to focus on an aspect of coacervates that is inherent to their protocell and membraneless organelles applications: compartmentalization.

### Compartmentalization behavior of an RNA oligonucleotide during the wet-dry cycle

As the water evaporated and the total volume decreased during drying (Fig. 2a), the concentration of each component increased (Fig. 2b). We did not observe changes to the volume of coacervate formed, based on visual estimates (Supplementary Fig. 15b). To understand the changes to the coacervate as the water content decreased, partitioning of a short fluorescently-labeled RNA oligomer, a 15-mer oligouridylic acid U15, was performed, as RNA, with its versatility20,21,49, is thought to play a central role in prebiotic chemistry50. The labeled U15 partitioned strongly into the coacervate phase, with >30,000-fold greater local concentration inside than outside the droplets (Fig. 2c–d; with 0.02 µM U15 added globally before drying, 10 µM were measured inside the droplets and around 0.3 nM outside).

After each drying step, U15 was added in concentrations that matched the drying-induced increase in components concentration (Fig. 2c). As seen in Fig. 2d, the measured concentration of the fluorescent U15 in the coacervate phase stayed constant throughout the process, despite the increase in global U15 concentration during dehydration (see Fig. 2e, Supplementary Figs. 12 and 14). At the same time, U15 concentration in the dilute phase increased from less than 1 nM up to 12 nM (Supplementary Table 1). The partitioning coefficients, or partition ratio, K = U15coacervate phase/U15dilute phase, decreased from >30,000 to around 1000 (Fig. 2d). In another experiment, the oligomer was added at a constant concentration of U15 (0.02 µM). As seen in Supplementary Figs. 13 and 14, the partitioning coefficients were similar in the two experiments, regardless of the initial [U15] added (Supplementary Fig. 14e–f) and measured in the coacervate phase.

The correlation between K and the decreasing total volume followed a linear trend as the coacervate phase volume stayed constant (Supplementary Fig. 15). While the ratio of the dilute phase/coacervate phase volumes decreased, the preference of U15 to go into the polymer-rich phase decreased, even if more of the nucleic acid was available in the dilute phase (Supplementary Fig. 15, Supplementary Table 1). Zeta potential measurements ruled out the effect of the coacervate charge on partitioning (Supplementary Note 5, Supplementary Fig. 16). The observed decrease in partitioning suggests that the coacervate phase paradoxically could become more hydrated as the overall sample dehydrated, due to increasing polyelectrolyte and salt concentrations. This, along with an increase in charge screening would render the two phases more similar and reduce the strong preference of the U15 for the coacervate phase. Coacervate compartmentalization has been shown to exhibit a close relationship between partitioning and molecular mobility20,47. To further explore the RNA behavior, we investigated U15 diffusion within the coacervate.

Fluorescence recovery after photobleaching (FRAP) experiments were performed to investigate the movement of U15 between the coacervate droplets and the surrounding dilute solution (whole-droplet FRAP) and within the droplet itself (partial-droplet FRAP). Figure 3a, b depicts representative samples of these experiments showing the whole-droplet FRAP of the 160-min sample and the partial-droplet FRAP of the 80-min sample, respectively. Figure 3c, d shows the fluorescence recovery profiles within these samples. The apparent diffusion coefficients, obtained from the recovery halftime values (τ1/2) (which are also shown) and the photobleached areas radii, are shown in Fig. 3e, f for the whole-droplet and intradroplet FRAP experiments, respectively. We note that these data are most useful for comparing between similar datasets, and not between the two experiment types, to understand different dehydration states rather than as a means of quantifying true molecular diffusion51. The slow diffusion in the initial samples can be correlated with the high partitioning observed in these samples in Fig. 2. The photobleached U15 was almost immobilized within the droplets in these samples as the exchange rate with the surrounding solution was low.

RNA recovery within the whole droplet showed an increasing trend as the water was lost from the coacervate mixture (Fig. 3e). While the upper bound of apparent diffusion coefficients after tenfold dehydration was close to 0.2 µm2 s─1, these values are considerably lower than their expected diffusion in buffer of around 150–300 µm2 s─120,52. Values ranging between 0.005 and 1.9 µm2 s─1 were previously measured for various RNA 15-unit oligomers partitioned within a polyU/spermine coacervate47. The difference in the diffusion within the droplets was not as significant, merely doubling between the first and the last time point—spanning a decrease of 8 to 10-fold in sample volume (or similar increase in concentrations, Fig. 3f)—and rehydration recovered the initial values. This implied a ~2-fold decrease in the coacervate viscosity. The effect of slow whole-droplet recovery can be further seen in the example shown in Fig. 3b as, even though the photobleached region of the droplet recovered quickly from the supply of RNA in its immediate proximity, the whole-droplet fluorescence intensity slightly decreased as it took longer for this supply to be replenished from the dilute phase. This also emphasizes that the apparent diffusion coefficients are standardized to the size of the bleached area: even the highest whole-droplet diffusion coefficients correspond to a slower recovery than the slowest partial-droplet coefficients (whole droplet 160 min: 20 s, partial droplet 0 min: 2.7 s—gray bars in Fig. 3e, f). Repeating the exchange experiment with a constant concentration of U15, instead of increasing them like here, disproved the hypothesis that the increase in RNA mobility could be a concentration effect (see Supplementary Note 6, Supplementary Fig. 17, Supplementary Table 4).

### Mechanism of RNA partitioning and kinetics during drying

Combined, the partitioning and FRAP results lead to a better understanding of the observed nucleic acid compartmentalization behavior during dehydration. The strong accumulation of RNAs within the coacervate phase of related systems has been previously observed and attributed to electrostatic attraction, which can be coupled with displacement of polyanions within the network20,47,53. The partitioning values and the apparent diffusion coefficients are the consequence of the complex nucleic acid dynamics towards, outward from, and within the coacervate phase20. The dynamics, which are governed by charge screening, appear to be directly related to partitioning: the change in whole-droplet diffusion coefficient (~40-fold increase) was in the opposite direction, but similar magnitude, as the partitioning coefficient (~30-fold decrease). Hints of a strong correlation between fast whole-droplet recovery and low partitioning have been observed before20,47. Salt has been shown to decrease the entropy penalty for partitioning of charged polymers54. Elevated levels of charge screening cause the polymer to behave like an uncharged molecule which decreases its preference for one or the other phase54,55. Here, a general trend of this relationship was elucidated.

Furthermore, even though slower kinetics could be expected from an increase in polymer concentration, a simultaneous increase in hydration, which would cause a reverse effect, has been observed before with coacervates made of lysine and glutamic acid polymers38. This phenomenon, which has been ascribed to self-suppression of complex coacervates56, was implied for diagonal movements along the charge-equivalence line on the phase diagram38. While the repercussion of this phenomenon could be a slight decrease in coacervate volume, this can be counterbalanced by an increasing salt concentration, accompanied by an increase in water content38. Higher polymer concentrations have also been shown to promote compartmentalization in two-component systems with low salt concentrations54. This increases the mixing enthalpy and enhances partitioning, but also raises the water content of the coacervate phase38 which brings its hydration level somewhat closer to the dilute phase.

An expanded discussion on expected partitioning of polymers between the two phases and its impact on the observed behavior is included in the Supplementary Discussion 1 and Supplementary Fig. 18. As the polymer-rich phase becomes less concentrated in polymers, more hydrated, and more charge screened—in its approach to the critical point where the compositions of the two phases eventually become the same—the outcome is faster diffusion and lower preference of the guest molecule to one or the other phase. In general, the behavior of the U15 RNA used here can be interpreted as that of a polymer undergoing similar effects as the ones expected for other macromolecules. The decrease in the RNA partitioning is manifested by a constant concentration inside the polymer-rich phase accompanied by an increase in the dilute phase (see Supplementary Discussion 1). We next tested how the expected periodicity of wet-dry cycling would impact the compartmentalization behavior of the coacervates used here.

### Impact of repeating wet-dry cycles on coacervate compartmentalization

Multiple wet-dry cycles, which could last from few minutes to few hours, are usually employed to increase reaction yields and prove their robustness in extreme environmental variability1,2,12. We sought to expose the PDADMA/PAA coacervate compartments to multiple cycles to check whether they survive these conditions, and to understand the impact on their RNA partitioning. Repeatedly drying and rehydrating the coacervate was monitored by weighing the contents of the tubes (Fig. 4a). The solution pH remained the same during these steps, with a slight decrease observed after the first cycle (Supplementary Fig. 19). The concentration of U15, added at the same concentration after rehydrating all samples, was around 10 µM after five cycles (Fig. 4b, Supplementary Fig. 20). A slight increase was observed between the initial sample and the rehydrated ones, similar to the outcome of the single-cycle experiment in Fig. 2. While vortexing, then pipetting, was employed to resuspend the dry coacervate, this increase in [U15] within the coacervate could be related to some coacervate not being resuspended completely. This could also explain the slight drop in pH values after the first cycle as some HEPES would be stuck with the unsuspended coacervate. Supplementary Note 7 details the statistical analysis showing this difference; while the last cycle is also shown to be slightly different, the discrepancy is less significant. The partitioning coefficient did not vary significantly (Supplementary Note 7), indicating that the U15 amount in the supernatant was similar, around 1–2 nM, among samples (Fig. 4c, Supplementary Table 7). The FRAP experiments in Fig. 4d, e showed that the dynamics of U15 remained unchanged after cycling the samples between dry and wet states which demonstrated that the coacervate integrity and viscosity were regained after each rehydration step. It is worth noting that the apparent diffusion coefficients were close to the second time point in Fig. 2, in which the same concentrations of components as the starting ones in this experiment were reached. Overall, these experiments revealed the minimal impact of repeated cycles on the compartmentalization potential of complex coacervates.

### Comparing the dried samples with composition mimics

Thus far, we have discussed the effects of drying and rehydration on complex coacervates. While this process, and its impact on compartmentalization, were expected to be grounded in movements on the phase diagram (dashed lines in Fig. 1), we sought to validate whether these movements were indeed dictating the resulting behavior. Most experiments above follow a movement that has been theoretically described as traversing a charge-equivalence line38. If the implication is correct, we hypothesized that it should be possible to recreate the drying process by making samples with increasing concentrations of all components—composition mimics—with the same total volume. This experiment would also help us verify whether the cycling process affects the linear movement, for example by damaging reactants or through failure of reincorporating large amounts of the dry materials into the rehydrated coacervates. Mimics that contained the same polymer, salt, and buffer components were prepared with starting concentrations that would fall on the same expected line as the drying process (Fig. 5a).

These composition mimics samples were prepared at the same total volume as the initial sample in all the above experiments (500 µL, Fig. 5a). Figure 5 and Supplementary Fig. 22a show samples that were dyed with bromophenol blue and centrifuged to show the difference between dried coacervates and mimics. A visual calibration curve was prepared to estimate the volumes of the concentrated phase (Supplementary Fig. 22b). The total volume was obtained by conversion from net weights (Supplementary Fig. 23). The first sign that the coacervate mimics and the dried ones, while having different total volumes, were similar was the almost identical ratio of Vcoacervate/Vtotal (Fig. 5b). To check whether this similarity translated into the same compartmentalization behavior of coacervates, U15 partitioning and FRAP experiments were performed. Figure 5c–f shows that these partitioning and FRAP results were very similar between the dried samples and the mimics. While the starting values in Fig. 5d are slightly different, the trend in percentage decrease is almost identical (Supplementary Note 7, Supplementary Fig. 21). The pH of the mimics also stayed constant, following a similar trend to the dried samples (Supplementary Fig. 25). These comparisons emphasize the importance of the volume ratio of the coacervate to the total volume, rather than the volume itself, in determining its properties and behavior. We note that these volume fractions reflect changes in the composition of the coacervate and dilute phases, which define the observed effects on the RNA partitioning and diffusion (see Supplementary Discussion 1). Such an outcome gives confidence in results of experiments that are performed with minimal volumes when the materials are limited. The mimics experiment also demonstrated the predictability of the drying behavior from samples prepared from scratch.

To understand the impact of the observed movement through the phase diagram on the internal structure of the coacervate and its possible relationship to the compartmentalization behavior, we turned to small-angle X-ray scattering (SAXS). SAXS enabled us to investigate the conformation of polymers in solution over multiple length scales simultaneously. This technique has been applied to similar systems to understand the effects of increasing the concentration of one component—polymer or salt alone35,57. In general, as salt is added and electrostatic interactions are screened, polyelectrolyte chains decrease in effective charge density and more closely resemble neutral polymers in solution by SAXS35,37. In our case, we increase both polymer and salt concentrations, in addition to buffer and magnesium amounts, to mimic the impact of drying on the structural level (Fig. 5a). The aim of this experiment was to explore the molecular-level effects of this realistic environmental change. Samples with lower polymer and salt concentrations (below 50 mM for both) were omitted from the analysis as they did not scatter well because of the small volume of coacervate material. Samples with 50–100 mM concentrations scattered better and were qualitatively analyzed to obtain an idea of the coacervate network behavior along the same charge-equivalence line on the phase diagram (sample details are in Supplementary Table 10, dotted line in Fig. 5a).

All scattering profiles of analyzed samples had a slope of–2 at high-q (i.e., at the smallest length scale) which showed the behavior of a Gaussian chain exhibiting a random walk—an observation that has been reported for many other polymer coacervate systems in the literature35,37,57 (Fig. 6a, Supplementary Fig. 26a). At larger length scales (mid-q), the slope was shallow at the lower concentrations but showed an I(q) ~ q−1 dependency at higher concentrations. The latter indicates rod-like structures which, along with the increase in scattering seen at a length scale of 10–40 nm (obtained using an estimated direct conversion of 2π/q), could be attributed to the dense tubule diameters that have been observed in cryo-transmission electron microscopy measurements58,59. We also note that a small peak around 0.025 Å−1 in the 50 mM sample could be related to long-range electrostatic repulsion, as expected from a highly charged sample (see Supplementary Fig. 16). The upturn in the scattering at low-q could point to larger aggregates as all concentrations increase and along with them, the hydration level. Future investigations could probe this larger length scale further.

In the high-q region, a broad low-intensity peak around 0.3 Å−1 in the lower concentration samples appeared to shift to lower-q in the higher concentrations. Such a peak is widely reported in the literature to originate from a distinct polyelectrolyte correlation length, ξ, which is related to the interactions between the polymeric chains37,55,60. The intensity of the peak is sharp in concentrated polyelectrolyte solutions; in general this is highly dependent on the polymer concentration which, if increased, causes a shift to higher-q values (corresponding to smaller lengths or mesh sizes)55. However, its intensity drastically decreases in the presence of salt, which weakens the electrostatic repulsions between chains, or when the polyelectrolyte associates as part of a complex mixture, such as in complex coacervates35,37. With the help of the Unified fit, applied to one structural level61,62, the approximate size of this length was obtained (Fig. 6b, Supplementary Fig. 26b and Supplementary Table 11).

The increase in the size of the correlation length, from around 7 to around 10.5 Å, pointed to the noteworthy influence of salt screening on the structure of this complex coacervate during the simultaneous increase of both polymer and salt concentrations. The observation along this line in the phase diagram supports the partitioning and diffusion behavior of the U15 seen above, as salt screening appeared to be the key player in these results. Also, a less polymer-dense network deduced from the mid-q region, and the increase in ξ, implied a more hydrated coacervate phase.

### Changing the directions of compositional change

While changes in starting compositions caused a predictable control over the formation and disassembly of the coacervate (Fig. 1), we next explored the effects of more systematic variations over the guest RNA, using more mimics. As the mimics experiments above focused on moving along a charge-equivalence line, we examined the impact of traversing other linear directions within the phase diagram on the coacervate compartmentalization capacity, by changing the starting concentration of one component. Figure 5 showed that the drying behavior can be predicted from such samples. Therefore, to mimic drying here, samples were prepared with various salt concentrations for a fixed range of polymer concentrations (Fig. 7a, Supplementary Fig. 27). The opposite—changing the polymer concentrations with fixed [salt]—was also investigated (Supplementary Fig. 28). The initial U15 added in these experiments was increased with the polymer concentration, to mirror the drying effect. In Fig. 7, it increased from 0.02 to 0.2 µM in the variable salt concentrations mimics.

Varying the salt concentrations around a starting value of 5 mM with a fixed range of polymer concentrations starting at 5 mM did not affect the concentration of U15 partitioned inside the coacervate, consistent with what was observed in the drying experiment (Supplementary Fig. 27b). Salt was varied in a linear fashion, similar to drying samples, with values ranging between 2.5 and 25 mM in the lower concentrated samples and between 10 and 100 mM in the higher concentrations. In the same samples, the partitioning coefficient decreased with increasing salt concentrations towards the upper section of the range (Fig. 7b), which directly validated the impact of salt screening on the partitioning behavior. Similar experiments performed with varying polymer concentrations in a fixed salt range had an impact on the U15 concentrations inside the coacervate phase which decreased, but the trend in partitioning was again similar to, but slightly shallower than, the salt experiment (Supplementary Fig. 28). The mechanism of partitioning above and SAXS results pointed to an increase in hydration with more polymers, accompanied by a changing volume fraction, which would explain the effect on the U15 concentration inside the coacervate phase.

The whole-droplet FRAP response in the experiments where the concentration of salt was varied showed an increasing apparent diffusion coefficient, similar to the drying experiment. Among the samples that had the same polymer concentrations, the highest concentration of salt exhibited the fastest kinetics (Fig. 7c). The difference in the lower salt concentration samples (2.5–25 mM NaCl) was not as distinct. The effect of salt screening on polyelectrolyte diffusion has been shown to be nonlinear63. Interestingly, the samples that had different polymer concentrations for the same salt concentrations also showed increasing whole-droplet diffusion trends (Supplementary Fig. 28, Supplementary Table 14). The universal correlation between faster kinetics and lower partitioning in these experiments mirrored drying experiments. As for partial-droplet FRAP, the increase in kinetics was again less pronounced (Supplementary Figs. 27c and 28e, Supplementary Tables 13, 15), revealing how it was harder to affect the internal viscosity of the coacervate by changing the concentrations in this range. This pointed, again, to the importance of whole-droplet exchange, over internal viscosity, in determining exchange kinetics with the surroundings.

## Discussion

The experiments in this paper point to an intriguing richness in phase behavior and physical properties of PDADMA/PAA complex coacervates as they dry and rehydrate, and to how these changes can be understood using the phase diagram. The experiments with mimics successfully linked the wet-dry cycling process to movements on the phase diagram. They also provided structural insights on the expanding polymeric network as this distinctive linear compositional change occurred, and predicted the effects of varying the direction of these movements. Based on the generality of the ionic strength and (de)hydration effects underlying these behaviors, we anticipate that similar wet-dry cycling response may be possible for other complex coacervate systems.

Repeated wet-dry cycles did not seem to impact the integrity and dynamic response of the coacervate. During a single cycle, the transition between different hydration states did not significantly affect the local concentration of RNA inside the coacervate droplets over a 10-fold decrease in overall sample volume and concomitant increase in total concentrations of RNA and other components. Hence, the coacervate phase essentially buffers the local RNA concentration during large environmental changes, even while it changes substantially outside the droplets. From a coacervate perspective, our analysis emphasizes that changes in the overall system do not necessarily correlate with proportional changes in the composition of each phase, and can be understood through the phase diagram. From a protocell perspective, this very primitive form of proto-homeostasis might be beneficial for early cellular function. At the same time, changes in RNA exchange between the coacervate droplets and the exterior continuous phase, and in the relative amounts of nucleic acid inside versus outside the compartment, were substantial. As has been discussed by Jia et al., high exchange rates could hinder evolution of RNA as its segregation within individual compartments is short-lived64. However, RNA exchange rates between coacervate and continuous phases, and ultimately between coacervate droplets, can be controlled by manipulating the interaction strength of the compartment’s charged components53 or preparing coacervates with microfluidics65. The present work suggests that considering the trajectories of such systems through composition space during hydration cycling, afforded by an environmental process, can provide an additional mode of control in which populations of membraneless compartments cycle between states with higher and lower inter-droplet RNA exchange.

Furthermore, controlling the drying rate would allow a balance over the duration where high partitioning is obtained versus that during which fast kinetics are predominant, depending on the requirements of the experiment. It is thought-provoking to consider that the composition (as well as macromolecules and salt types) and drying method of various ponds on an early Earth could have led to a large number of dehydration processes, providing access to compositionally and functionally different coacervate populations, even if the available components were limited. Considering several recent reports that discuss the potential of coacervates to modulate the reactivity of ribozymes and other enzymes20,21,53, the changes observed here are expected to result in a wide array of reactivity profiles within the concentrated phase. As such, it is important to keep in mind that an optimal composition for a certain function of complex coacervates could be ideal for a limited range of concentrations (of both polymer and buffer molecules). For better or worse, this range is easily changeable in a transient natural system, as we show here. Outside the scope of origins of life research, the conditions imposed on coacervates by wet-dry cycling could be of interest to their use in other fields. For example, this study demonstrates that their cargo-carrying and -release capacities could be predictable depending on the level of hydration, a feature that would be of interest in the area of drug design and in vivo delivery, particularly for gene therapy and gene editing applications.

Finally, we note that the similarity between the dehydrated samples and their composition mimics encourages future work not only via the obvious convenience of using mimics in place of dehydrated samples, but also in the conceptual differences between them. While the parameters examined in the experiments above collapsed to one behavior, it is fascinating to consider the directionality of these two sets of samples: the dried samples are moving towards a state of complete dehydration; the mimics are traversing the phase diagram towards a single-phase highly hydrated system. Nonetheless, they behave similarly: while the mixture dries, the coacervate phase acts like a more hydrated entity. The wet sample, depending on the starting composition, could start with a polymer-rich phase in a kinetically trapped state, e.g., with encapsulated RNAs unable to diffuse freely. As the solution dries, the coacervate phase becomes more liquid-like, allowing the RNA molecules to diffuse more freely before further drying traps it again in a solid form. Such progression has been observed before by groups exploring the different morphologies of polyelectrolyte complex coacervates33,66, and requires further analysis. The implications on the protocell-behavior of coacervate are intriguing. On one hand they show the striking role of the coacervate-to-total-volume ratio in determining the composition and phase behavior of the compartment. On the other hand, they raise questions as to whether there exists a divergence point in the behaviors among the two types of samples and the reliance of such a point on the composition and hydration state of each component.

## Methods

### Materials

Poly(diallyldimethylammonium chloride), PDADMAC, was obtained from Polysciences, Inc. (molecular weight, MW ~8500 g mol−1), and poly(acrylic acid), PAA, was obtained from Sigma–Aldrich (average MW ~1800 g mol−1). Sodium chloride (NaCl, ≥99.5%), 4-(2-hydroxyethyl)piperazine-1-ethanesulfonic acid sodium salt (HEPES, ≥99.5%), and magnesium chloride hexahydrate (MgCl2.6H2O) were all purchased from Sigma–Aldrich. Polymer stock solutions were prepared in water with a final weight percent of around 10–11% for PDADMA and around 5% for PAA. The pH of the stock solutions was adjusted to ~7.5 using sodium hydroxide (NaOH, EMD, ≥97.0%). The oligonucleic acid U15, a uridylic acid 15-mer, was obtained from Integrated DNA Technologies and was labeled on the 5’-end with Alexa Fluor 647. The U15 oligomer was dissolved in nuclease-free water (Ambion), aliquoted, and stored at −20 °C. Micro cover glasses (no. 1.5, 24 × 30 mm, VWR) were used to image samples. Silicon spacers (Electron Microscopy Sciences), with 9 mm internal diameter and 2 mm depth, were sandwiched between two cover glasses for imaging. All polymer solutions and coacervates were prepared using HPLC grade water (Ricca Chemical Company). Unless otherwise stated, coacervate solutions were prepared, dried, and rehydrated in polypropylene microcentrifuge tubes (VWR).

To improve the imaging of coacervate droplets by preventing their coalescence on the surface, the slides were functionalized with oligoethylene glycol moieties to reduce interactions with coacervate components. This was done by incubating them in a 0.3% solution of N-(triethoxysilylpropyl)-o-polyethylene oxide urethane (95%, Gelest, Inc.) in anhydrous toluene (99.8%, EMD Millipore Corporation) for 4 h. The treatment was preceded with a cleaning step that consisted of soaking the slides in a saturated solution of potassium hydroxide (≥85%, Sigma–Aldrich) in isopropanol (90%, Ricca Chemical Company) for 30 min followed by water rinsing and drying at 70 °C. After the oligoethylene glycol functionalization step, the slides were thoroughly washed with toluene, ethanol (190 proof, Koptec), and water, respectively, with a final drying step at 70 °C overnight.

### Coacervate preparation, drying, and addition of U15

Coacervates were prepared by mixing specific volumes of HPLC grade water with the appropriate volumes of MgCl2 (0.216 M), HEPES (0.942 M), and NaCl (1.0 M) stock solutions, followed by adding PAA and PDADMA, respectively, to reach the desired final polymer concentrations. All components concentrations are mentioned in the Results section and figures as they were adjusted to suit the goal of each experiment. The concentrations of polyelectrolyte stock solutions were around 0.6–0.8 M (all with respect to the monomer or single charge) depending on the trial, and 1.6–1.8 M in certain turbidity phase diagram experiments that required higher polymer concentrations. The charge ratio was kept at 1:1 by equalizing the final concentrations with respect to the monomers. The addition of the polycation (last added component) caused the solution to become visibly turbid, a sign of coacervation. Solutions were mixed by pipetting gently with a 1000 or 200 µL pipette, depending on the total volume. The tubes were vortexed before and after the addition of the polyanion, then quickly spun (3 s) to collect any liquid on the walls or the cap. After the addition of the polycation, the tubes and their contents were weighed again to obtain the initial weight of the coacervate solution. Samples were then quickly pipette-mixed to uniformly disperse the coacervate, spun down for few seconds, and placed in a preheated heatblock for drying.

Drying of coacervate solutions was performed using a Digital Heatblock (VWR). The microcentrifuge tubes containing the coacervates were placed in the heatblock after preheating it to the chosen temperature (95 °C). The internal temperatures of the block (and tubes) surfaces were verified using a thermometer (Traceable, VWR) equipped with a type K thermocouple. These measurements showed that the temperature at the bottom of the tubes reached the surrounding value of 95 °C after around 2 min and 30 s. All samples were prepared in triplicates and different samples were prepared for each time point (0, 40, 80, 120, 160 min, and a sample that was fully dried for a total time of 4 h 40 min to be used for rehydration)—and all heated simultaneously. The t = 0 samples were prepared at the same time as the others but not heated. The tubes were placed in the block with the lid open to allow water evaporation.

At each time point, a set of triplicates (positioned at different locations of the block to avoid errors from temperature variability) was capped, removed, and allowed to cool down to room temperature before weighing. All empty tubes were weighed initially and after sample preparation, before heating and after heating, using a digital balance (Mettler Toledo) to ensure uniformity of treatment among experiments. The ambient room temperature and humidity were recorded every 5 min during the drying experiments using a Bluetooth Datalogging Temperature and Humidity Meter (TraceableGO, VWR), with no noticeable effect of both parameters on the outcome of drying. As the coacervate would have settled at the end of each drying period (or after leaving the samples for a day or two for triplicate analysis), a 200-µL pipette was used to resuspend it before the addition of the U15 oligomer for confocal microscopy experiments. Measuring the pH of the turbid coacervates or the supernatant solutions was done using a pH meter (SevenExcellence, Mettler Toledo) equipped with an Ultra-Micro-ISM pH electrode (Mettler Toledo) for small-volume samples.

The U15 aliquot was heat-shocked at 95 °C for around 60–90 s, allowed to return to room temperature, and vortexed before the addition of the adequate amount to the resuspended coacervate samples, followed by pipetting to allow even dispersion. The heat shock is performed to disrupt any aggregates and misfolds due to cold storage of the RNA aliquot (at −20 °C). While such artifacts are not expected in simple homo-oligomers, we wanted to avoid any potential interference with the compartmentalization behavior. This order allowed to check the new state of the coacervate and prevent RNA hydrolysis. As the diffusion of the RNA was shown to be slow in some samples (low [polymer], [salt]), the addition of the fluorescently tagged U15 to the coacervate was followed by incubating the solutions in the dark for around 4 h to allow equilibration, and avoid light damage to the fluorophore. This was followed by mixing the samples again with a pipette and placing the desired amount of coacervate (usually 10 µL) on oligoethylene glycol-functionalized slides. After covering the samples with a nontreated slide sandwiching a silicon spacer, they were allowed to sit for at least one hour while other, faster diffusing samples, were imaged. It was apparent that some slow-diffusing droplets had higher U15 concentrations at the beginning which could be caused by the RNA loading the coacervate phase that it encountered first more. Because of the relatively faster diffusion of U15 within all these droplets (see intradroplet FRAP results), no local inhomogeneity (or aggregation) was observed. The incubation steps led to uniform fluorescence in slow-diffusing samples (which otherwise exhibited differing levels of fluorescence among droplets) and were not necessary for samples which showed faster dynamics.

### Turbidity measurements

To establish their phase diagram, the turbidity of coacervate solutions was measured with an Infinite M1000 Pro instrument (Tecan) using the i-control microplate reader software (version 1.11). PDADMA/PAA coacervates were prepared at 1:1 charge ratio with different concentrations of polymers (with respect to monomer concentration) and NaCl. HEPES and MgCl2 concentrations were kept at 25 mM and 4.3 mM for all these samples. All solutions were prepared in a 96-well plate (Flat bottom, Nunclon Delta transparent, ThermoFisher) with a total volume of 250 µL each. Multiple reads of absorbance per well were performed and the average was calculated for each sample. After correcting for background absorbance, the percent transmittance was calculated, as (10Absorbance at 500 nm) × 100, followed by the turbidity, as 100 − %Transmittance.

Temperature-dependent turbidity was measured using an OLIS 8453 diode-array UV-visible spectrometer equipped with a Peltier temperature-controlled cell holder where up to six cuvettes containing the solutions could be placed. A SpectralWorks software was used to set up the measurements and temperature. While it was possible to scan the absorbance as the temperature was varied automatically, a decrease in turbidity was observed and ascribed to some evaporation of samples during the long measurement. For that reason, fresh 1:1 PDADMA:PAA coacervate samples were prepared in duplicates for each time point, and allowed to sit at the specific temperature for 10–12 min before the measurement. Coacervate samples prepared in water alone and in buffer (50 mM NaCl, 25 mM HEPES, 4.3 mM MgCl2) were measured this way at temperatures that ranged between 5 and 95 °C.

### Zeta potential measurements

The zeta potential of coacervate samples was measured using a Malvern Zetasizer Nano Series (Nano ZS, Malvern Panalytical). Coacervates were prepared with a total volume of 1 mL in the addition order described above, and transferred to a folded capillary zeta cell (Malvern) for the measurement. Data recording and analysis was done on the Zetasizer Software 7.10 from Malvern. A Leica Auto Abbe refractometer was used to obtain the refractive index of the buffer solutions.

### Imaging samples without fluorescence labeling

Transmitted light imaging of samples to support the turbidity analysis of the phase diagram and the initial drying experiments was performed using a Nikon Eclipse TE200 inverted microscope equipped with an Image-Pro Plus 7.0 software. Samples were sandwiched between an oligoethylene glycol-functionalized slide at the bottom and a normal microscope slide on top with a silicon spacer, which were placed on top of a Nikon Plan APO ×100/1.40 oil objective. Images were analyzed using the ImageJ software.

### Partitioning and fluorescence recovery after photobleaching (FRAP)

Imaging of coacervate samples containing fluorescent probes was performed on a Leica TCS SP5 laser scanning confocal inverted microscope. All images were acquired with an HCX PL APO ×63.0/1.40–0.60 oil CS UV objective on a LAS AF software (both from Leica), and data analysis was performed on a LAS AF Lite software (ver. 2.6). While images were acquired at different zoom factors, a zoom of 3.0 was used to measure the fluorescent emission from droplets for partitioning experiments as well as to establish a calibration curve for the Alexa 647-tagged U15. For all imaging experiments, including the calibration curve, the excitation was at 633 nm, the excitation beam splitter was chosen as TD 488/543/633, and the emission bandwidth of the photomultiplier tube was set to 650–695 nm. All partitioning experiments were performed in duplicates or triplicates and 3 images of at least 5 droplets were analyzed for each trial (each result was usually an average of 15 droplets per trial ×2 or 3).

To obtain the partitioning coefficient K (ratio of U15 concentration in coacervate phase/concentration in dilute phase ratio), the samples were centrifuged (Centrifuge 5415 R, Eppendorf) at 13,200 rpm (16,100 × g) for 15 min, and around 200 µL of the supernatant was transferred to a new tube for fluorimetry measurements. For samples that were dried further and did not contain enough supernatant volume for the analysis in the 160-µL cuvette, a specific volume of the supernatant was diluted in water and the results were corrected to adjust for the dilution factor. A Fluorolog instrument (Horiba Scientific) was used to measure the fluorescence emission from the supernatant at 665 nm for the Alexa 647-U15 probe. Excitation was at 633 nm, like in the confocal measurements and multiple scans (at least 10) were averaged for each trial to obtain the final results. A calibration curve was established using the same settings, and was used to convert counts to concentration.

FRAP experiments were performed on the same confocal instrument with all the lasers turned on (543, 633 nm, and the Argon laser at 20%). While imaging was still performed using the same settings mentioned above, the bleaching was performed at 100% 458, 476, 488, 514, 543, and 633 nm laser power. Partial regions of droplets (1 µm diameter) or the whole droplet (5–9 µm diameter, depending on the coacervate composition) were selected as regions of interest (ROI). Depending on the experiment, pre-bleaching imaging and bleaching were set to 5 or 10 frames. In fast diffusing samples, bidirectional scanning was performed to capture as much data as possible at the beginning of the post-bleach imaging. Post-bleach time and frames were adjusted to match the diffusion within each sample. All experiments were performed in duplicates or triplicates (with measurements of at least nine internal regions for partial-droplet analysis and six droplets for whole-droplet analysis). When experiments that required larger amounts of U15 were performed in duplicates, the number of droplets and internal regions were increased to match the same number of trials done in triplicates.

Because of loss of fluorescence during multi-frame post-bleach measurements, the fluorescence was normalized to obtain the FN(t) as was described before47,64, using:

$$F_N\left( t \right) = \frac{{\left[ {S_{(t)} - B_{(t)}} \right]\left[ {R_{(0)} - B_{\left( 0 \right)}} \right]}}{{\left[ {R_{(t)} - B_{(t)}} \right]\left[ {S_{(0)} - B_{\left( 0 \right)}} \right]}}$$
(1)

where S(t) was the average measured fluorescence recovery postbleaching of the bleached ROI, R(t) the average fluorescence intensity of a reference ROI that was either a similarly-sized whole droplet in the same frame for whole-droplet experiments or a 1-µm nonbleached region within the same droplet for intradroplet experiments, B(t) the average background fluorescence of a randomly chosen region postbleaching. As for background fluorescence, B(0) was the background reference obtained as the average of five images measured separately with all the lasers turned off, S(0) was the average of the prebleach fluorescence for the specific bleached ROI, and R(0) was the average prebleach fluorescence of the reference ROI.

Data fitting was performed using an OriginPro 8.5 software according to the following equation:

$$F_N\left( t \right) = A\left[ {1 - \exp \left( { - \frac{t}{\tau }} \right)} \right] + C$$
(2)

where A is the mobile fraction of the fluorescence probe, C the y-intercept of the FN(t) fluorescence intensity recovery curve, and τ the fluorescence recovery time constant specific to each experiment, which could be used to obtain the halftime (τ1/2) of fluorescence recovery:

$$\tau _{1/2} = \tau {\mathrm{ln}}(2)$$
(3)

The halftime can then be used, along with the radius (r) of the specific bleached ROI, to obtain the apparent 2D diffusion coefficient, according to67:

$$D_{{\mathrm{app}}} = \frac{{0.88\,r^2}}{{4\tau _{1/2}}}$$
(4)

where 0.88 is a constant used for calculating diffusion for circular beams.

### Small-angle X-ray scattering (SAXS)

SAXS experiments were conducted at beamline 12-ID-B of the Advanced Photon Source at Argonne National Laboratory (Lemont, IL USA). Measurements were collected with 14 keV X-rays at a sample-to-detector distance of 4 m (q-range = 0.002–0.5 Å−1, equivalent to 1.2–310 nm length scale, with displayed region of interest corresponding to 1.25–63 nm) at 25 °C. The prepared coacervate samples were transferred into 2 mm quartz capillaries (Charles Supper Company, Natick, MA USA) and centrifuged at 5000 × g for 10 min, resulting in two coexisting phases. The capillaries were sealed with epoxy glue and stored at room temperature for at least 24 h prior to measurement. During the SAXS experiments, the capillaries were positioned in holding racks so that the coacervate phase was in the path of the beam to obtain scattering from the centrifuged coacervate. After collecting each sample, the path of the beam was moved vertically to check the supernatant phase against the respective aqueous background. The signal from this background, which is mostly water, was later subtracted from the coacervate phase signal. The exposure time of the samples was limited to 0.1 s. All two-dimensional data were converted to one-dimensional intensity profiles and processed using the Irena package62 for Igor Pro.

### Statistical analysis

The means and standard deviations are shown within the figures with additional details in the captions. We employed a single-factor ANOVA test to measure the differences between cycled samples and mimics samples. Where the results would not allow such a test, a two-tailed t-test was used. The results of these tests are available in the Supplementary Note 7.

## Data availability

All the data are available within the paper and its Supplementary Information file. Relevant data can be provided by the corresponding author upon request.

## References

1. 1.

Forsythe, J. G. et al. Ester-mediated amide bond formation driven by wet-dry cycles: a possible path to polypeptides on the prebiotic earth. Angew. Chem. Int. Ed. 54, 9871–9875 (2015).

2. 2.

Mamajanov, I. et al. Ester formation and hydrolysis during wet-dry cycles: generation of far-from-equilibrium polymers in a model prebiotic reaction. Macromolecules 47, 1334–1343 (2014).

3. 3.

Becker, S. et al. Wet-dry cycles enable the parallel origin of canonical and non-canonical nucleosides by continuous synthesis. Nat. Commun. 9, 163 (2018).

4. 4.

Damer, B. & Deamer, D. Coupled phases and combinatorial selection in fluctuating hydrothermal pools: a scenario to guide experimental approaches to the origin of cellular life. Life 5, 872–887 (2015).

5. 5.

Mulkidjanian, A. Y., Bychkov, A. Y., Dibrova, D. V., Galperin, M. Y. & Koonin, E. V. Origin of first cells at terrestrial, anoxic geothermal fields. Proc. Natl Acad. Sci. USA 109, E821–E830 (2012).

6. 6.

Campbell, T. D. et al. Prebiotic condensation through wet-dry cycling regulated by deliquescence. Nat. Commun. 10, 4508 (2019).

7. 7.

Weber, A. L. Thermal synthesis and hydrolysis of polyglyceric acid. Orig. Life Evol. Biosph. 19, 7–19 (1989).

8. 8.

Lahav, N., White, D. & Chang, S. Peptide formation in prebiotic era—-thermal condensation of glycine in fluctuating clay environments. Science 201, 67–69 (1978).

9. 9.

Rodriguez-Garcia, M. et al. Formation of oligopeptides in high yield under simple programmable conditions. Nat. Commun. 6, 8385 (2015).

10. 10.

Fox, S. W. & Harada, K. Thermal copolymerization of amino acids to a product resembling protein. Science 128, 1214–1214 (1958).

11. 11.

Rajamani, S. et al. Lipid-assisted synthesis of RNA-like polymers from mononucleotides. Orig. Life Evol. Biosph. 38, 57–74 (2008).

12. 12.

Da Silva, L., Maurel, M. C. & Deamer, D. Salt-promoted synthesis of RNA-like molecules in simulated hydrothermal conditions. J. Mol. Evol. 80, 86–97 (2015).

13. 13.

Ross, D. S. & Deamer, D. Dry/wet cycling and the thermodynamics and kinetics of prebiotic polymer synthesis. Life 6, 28 (2016).

14. 14.

Higgs, P. G. The effect of limited diffusion and wet–dry cycling on reversible polymerization reactions: implications for prebiotic synthesis of nucleic acids. Life 6, 24 (2016).

15. 15.

Fox, S., Pleyer, H. L. & Strasdeit, H. An automated apparatus for he simulation of prebiotic wet-dry cycles under strictly anaerobic conditions. Int. J. Astrobiol. 18, 60–72 (2019).

16. 16.

Verlander, M. S., Lohrmann, R. & Orgel, L. E. Catalysts for self-polymerization of adenosine cyclic 2’, 3’-phosphate. J. Mol. Evol. 2, 303–316 (1973).

17. 17.

Damer, B. & Deamer, D. The hot spring hypothesis for an origin of life. Astrobiology 20, 429–452 (2020).

18. 18.

Joshi, M. P., Samanta, A., Tripathy, G. R. & Rajamani, S. Formation and stability of prebiotically relevant vesicular systems in terrestrial geothermal environments. Life 7, 51 (2017).

19. 19.

Deamer, D. W. & Barchfeld, G. L. Encapsulation of macromolecules by lipid vesicles under simulated prebiotic conditions. J. Mol. Evol. 18, 203–206 (1982).

20. 20.

Drobot, B. et al. Compartmentalised RNA catalysis in membrane-free coacervate protocells. Nat. Commun. 9, 3643 (2018).

21. 21.

Poudyal, R. R. et al. Template-directed RNA polymerization and enhanced ribozyme catalysis inside membraneless compartments formed by coacervates. Nat. Commun. 10, 490 (2019).

22. 22.

Frankel, E. A., Bevilacqua, P. C. & Keating, C. D. Polyamine/nucleotide coacervates provide strong compartmentalization of Mg2+, nucleotides, and RNA. Langmuir 32, 2041–2049 (2016).

23. 23.

Deng, N. N. & Huck, W. T. S. Microfluidic formation of monodisperse coacervate organelles in liposomes. Angew. Chem. Int. Ed. 56, 9736–9740 (2017).

24. 24.

Koga, S., Williams, D. S., Perriman, A. W. & Mann, S. Peptide-nucleotide microdroplets as a step towards a membrane-free protocell model. Nat. Chem. 3, 720–724 (2011).

25. 25.

McCall, P. M. et al. Partitioning and enhanced self-assembly of actin in polypeptide coacervates. Biophys. J. 114, 1636–1645 (2018).

26. 26.

de Jong, B. & Kruyt, H. R. Coacervation. Proc. R. Acad. Amsterdam 32, 849–856 (1929).

27. 27.

Keating, C. D. Aqueous phase separation as a possible route to compartmentalization of biological molecules. Acc. Chem. Res. 45, 2114–2124 (2012).

28. 28.

Tang, T. Y. D., van Swaay, D., deMello, A., Anderson, J. L. R. & Mann, S. In vitro gene expression within membrane-free coacervate protocells. Chem. Commun. 51, 11429–11432 (2015).

29. 29.

Aumiller, W. M. & Keating, C. D. Phosphorylation-mediated RNA/peptide complex coacervation as a model for intracellular liquid organelles. Nat. Chem. 8, 129–137 (2016).

30. 30.

Yin, Y. D. et al. Non-equilibrium behaviour in coacervate-based protocells under electric-field-induced excitation. Nat. Commun. 7, 10658 (2016).

31. 31.

Nott, T. J., Craggs, T. D. & Baldwin, A. J. Membraneless organelles can melt nucleic acid duplexes and act as biomolecular filters. Nat. Chem. 8, 570–576. (2016).

32. 32.

Banani, S. F., Lee, H. O., Hyman, A. A. & Rosen, M. K. Biomolecular condensates: organizers of cellular biochemistry. Nat. Rev. Mol. Cell Biol. 18, 285–298 (2017).

33. 33.

Wang, Q. F. & Schlenoff, J. B. The polyelectrolyte complex/coacervate continuum. Macromolecules 47, 3108–3116 (2014).

34. 34.

Fu, J., Fares, H. M. & Schlenoff, J. B. Ion-pairing strength in polyelectrolyte complexes. Macromolecules 50, 1066–1074 (2017).

35. 35.

Marciel, A. B., Srivastava, S. & Tirrell, M. V. Structure and rheology of polyelectrolyte complex coacervates. Soft Matter 14, 2454–2464 (2018).

36. 36.

Zhang, Y. P. et al. Molecular origin of the glass transition in polyelectrolyte assemblies. ACS Cent. Sci. 4, 638–644 (2018).

37. 37.

Fares, H. M. et al. Scattering neutrons along the polyelectrolyte complex/coacervate continuum. Macromolecules 51, 4945–4955 (2018).

38. 38.

Li, L. et al. Phase behavior and salt partitioning in polyelectrolyte complex coacervates. Macromolecules 51, 2988–2995 (2018).

39. 39.

Chang, L. W. et al. Sequence and entropy-based control of complex coacervates. Nat. Commun. 8, 1273 (2017).

40. 40.

Kaibara, K., Okazaki, T., Bohidar, H. B. & Dubin, P. L. pH-induced coacervation in complexes of bovine serum albumin and cationic polyelectrolytes. Biomacromolecules 1, 100–107 (2000).

41. 41.

Simon, J. R., Carroll, N. J., Rubinstein, M., Chilkoti, A. & Lopez, G. P. Programming molecular self-assembly of intrinsically disordered proteins containing sequences of low complexity. Nat. Chem. 9, 509–515 (2017).

42. 42.

Chollakup, R., Smitthipong, W., Eisenbach, C. D. & Tirrell, M. Phase behavior and coacervation of aqueous poly(acrylic acid)-poly(allylamine) solutions. Macromolecules 43, 2518–2528 (2010).

43. 43.

Voets, I. K., de Keizer, A. & Stuart, M. A. C. Complex coacervate core micelles. Adv. Colloid Interface 147-48, 300–318 (2009).

44. 44.

Stewart, R. J., Wang, C. S. & Shao, H. Complex coacervates as a foundation for synthetic underwater adhesives. Adv. Colloid Interface 167, 85–93 (2011).

45. 45.

Schmitt, C. & Turgeon, S. L. Protein/polysaccharide complexes and coacervates in food systems. Adv. Colloid Interface 167, 63–70 (2011).

46. 46.

Johnson, N. R. & Wang, Y. D. Coacervate delivery systems for proteins and small molecule drugs. Expert Opin. Drug Deliv. 11, 1829–1832 (2014).

47. 47.

Aumiller, W. M., Cakmak, F. P., Davis, B. W. & Keating, C. D. RNA-based coacervates as a model for membraneless organelles: formation, properties, and interfacial liposome assembly. Langmuir 32, 10042–10053 (2016).

48. 48.

Nakashima, K. K., Baaij, J. F. & Spruijt, E. Reversible generation of coacervate droplets in an enzymatic network. Soft Matter 14, 361–367 (2018).

49. 49.

Hud, N. V., Cafferty, B. J., Krishnamurthy, R. & Williams, L. D. The origin of RNA and “My Grandfather’s Axe”. Chem. Biol. 20, 466–474 (2013).

50. 50.

Gilbert, W. Origin of life—the RNA world. Nature 319, 618–618 (1986).

51. 51.

Taylor, N. O., Wei, M. T., Stone, H. A. & Brangwynne, C. P. Quantifying dynamics in phase-separated condensates using fluorescence recovery after photobleaching. Biophys. J. 117, 1285–1300 (2019).

52. 52.

Yeh, I. C. & Hummer, G. Diffusion and electrophoretic mobility of single-stranded RNA from molecular dynamics simulations. Biophys. J. 86, 681–689 (2004).

53. 53.

Poudyal, R. R., Keating, C. D. & Bevilacqua, P. C. Polyanion-assisted ribozyme catalysis inside complex coacervates. ACS Chem. Biol. 14, 1243–1248 (2019).

54. 54.

Johansson, H. O., Feitosa, E. & Pessoa, A. Phase diagrams of the aqueous two-phase systems of poly(ethylene glycol)/sodium polyacrylate/salts. Polymers (Basel) 3, 587–601 (2011).

55. 55.

Muthukumar, M. 50th anniversary perspective: a perspective on polyelectrolyte solutions. Macromolecules 50, 9528–9560 (2017).

56. 56.

Veis, A., Bodor, E. & Mussell, S. Molecular weight fractionation and self-suppression of complex coacervation. Biopolymers 5, 37–59 (1967).

57. 57.

Spruijt, E. et al. Structure and dynamics of polyelectrolyte complex coacervates studied by scattering of neutrons, X-rays, and light. Macromolecules 46, 4596–4605 (2013).

58. 58.

Hwang, D. S. et al. Viscosity and interfacial properties in a mussel-inspired adhesive coacervate. Soft Matter 6, 3232–3236 (2010).

59. 59.

Jho, Y., Yoo, H. Y., Lin, Y. X., Han, S. & Hwang, D. S. Molecular and structural basis of lowinterfacial energy of complex coacervates in water. Adv. Colloid Interface 239, 61–73 (2017).

60. 60.

Nierlich, M., Boué, F., Lapp, A. & Oberthur, R. Characteristic lengths and the structure of salt free polyelectrolyte solutions—a small-angle neutron-scattering study. Colloid Polym. Sci. 263, 955–964 (1985).

61. 61.

Beaucage, G. Approximations leading to a unified exponential power-law approach to small-angle scattering. J. Appl Crystallogr. 28, 717–728 (1995).

62. 62.

Ilavsky, J. & Jemian, P. R. Irena: tool suite for modeling and analysis of small-angle scattering. J. Appl. Crystallogr. 42, 347–353 (2009).

63. 63.

Fares, H. M. & Schlenoff, J. B. Diffusion of sites versus polymers in polyelectrolyte complexes and multilayers. J. Am. Chem. Soc. 139, 14656–14667 (2017).

64. 64.

Jia, T. Z., Hentrich, C. & Szostak, J. W. Rapid RNA exchange in aqueous two-phase system and coacervate droplets. Orig. Life Evol. Biosph. 44, 1–12 (2014).

65. 65.

van Swaay, D., Tang, T. Y. D., Mann, S. & de Mello, A. Microfluidic formation of membrane-free aqueous coacervate droplets in water. Angew. Chem. Int. Ed. 54, 8398–8401 (2015).

66. 66.

Priftis, D. & Tirrell, M. Phase behaviour and complex coacervation of aqueous polypeptide solutions. Soft Matter 8, 9396–9405 (2012).

67. 67.

Axelrod, D., Koppel, D. E., Schlessinger, J., Elson, E. & Webb, W. W. Mobility measurement by analysis of fluorescence photobleaching recovery kinetics. Biophys. J. 16, 1055–1069 (1976).

## Acknowledgements

H.M.F.’s research was supported by an appointment to the NASA Postdoctoral Program with the NASA Astrobiology Program, administered by Universities Space Research Association under contract with NASA. J.M.T. acknowledges support from the NIST-CHiMaD Postdoctoral Fellowship, which is supported by assistant award 70NANB19H005 from U.S. Department of Commerce, National Institute of Standards and Technology as part of the Center for Hierarchical Materials Design (CHiMaD); CHiMaD supports polyelectrolyte complexation research at the University of Chicago, including financial support of A.E.M. This work was supported by a grant from the NASA Exobiology program (80NSSC17K0034). This research used resources of the Advanced Photon Source, a U.S. Department of Energy (DOE) Office of Science User Facility operated for the DOE Office of Science by Argonne National Laboratory under Contract No. DE-AC02-06CH11357. Xiaobing Zuo, PhD, is gratefully acknowledged for his assistance in the scattering experiments.

## Author information

Authors

### Contributions

H.M.F. and C.D.K. conceived and designed the experiments, analyzed the data, and wrote the paper. H.M.F. performed the wet-dry cycling and mimics experiments, including coacervate preparation, turbidity, microscopy, zeta potential, partitioning, FRAP, and fluorimetry measurements. A.E.M. and J.M.T. prepared samples and conducted the scattering experiments and assisted with the SAXS analysis and interpretation. H.M.F., A.E.M., J.M.T., M.V.T., and C.D.K. read, discussed, and edited the manuscript.

### Corresponding author

Correspondence to Christine D. Keating.

## Ethics declarations

### Competing interests

The authors declare no competing interests.

Peer review information Nature Communications thanks David Deamer, Marleen Kamperman and the other, anonymous, reviewer(s) for their contribution to the peer review of this work. Peer reviewer reports are available.

Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

## Rights and permissions

Reprints and Permissions

Fares, H.M., Marras, A.E., Ting, J.M. et al. Impact of wet-dry cycling on the phase behavior and compartmentalization properties of complex coacervates. Nat Commun 11, 5423 (2020). https://doi.org/10.1038/s41467-020-19184-z

• Accepted:

• Published:

• ### Connecting primitive phase separation to biotechnology, synthetic biology, and engineering

• Tony Z Jia
• , Po-Hsiang Wang
• , Tatsuya Niwa
•  & Irena Mamajanov

Journal of Biosciences (2021)