Protein crystallography is the predominate technique used to determine the three-dimensional structure of biological macromolecules. High-resolution three-dimensional structures provide information that is used to determine the function of proteins and other biomolecules and for drug discovery in cases where proteins play a role in different disorders or diseases. Growing high-quality crystals of these biomolecules enhances the ability to obtain X-ray data at a high resolution, thereby enabling more accurate three-dimensional structure determinations. Data and information obtained from crystallographic investigations are important for macromolecular engineering to optimize biomolecules for various applications in biomedical research. Macromolecular transport in crystallization processes has been shown to directly affect crystal quality (García-Ruiz et al., 2016; McPherson et al., 1999; Vekilov, 1999). Gravity-dependent flow effects, including convection and sedimentation, affect the crystal growth processes on earth (Lee and Chernov, 2002; Otálora et al., 2001; Wilcox, 1983). Density-driven solution convection might be expected to force molecules to rapidly flow past the growing crystal, thus bringing impurities such as inorganic and organic particles and macromolecular aggregates to growing crystal surfaces (Lee and Chernov, 2002). Different concentrations at different parts of a crystal created with the flow patterns may lead to nonuniform growth conditions (DeLucas et al., 1986; Wilcox, 1983). Sedimentation is another gravity-dependent effect that significantly alters the crystal growth process on earth. Depending on the density of the growing crystals versus the solution density, crystals growing in a 1G environment migrate to the top, bottom, or wall of a crystallization container (Carotenuto et al., 2002; DeLucas et al., 1986). Thus, sedimentation creates crystal accumulation on the surface, bottom, or wall of a crystallization container, which may interrupt further crystal growth (DeLucas et al., 1986; García-Ruiz et al., 2001a; Wilcox, 1983). Diffusion-controlled crystal growth processes in the absence of convection (and the elimination of the sedimentation effect) may be beneficial for crystal quality. Therefore, the microgravity environment appears to be ideally suited for growing crystals with improved quality (Kuranova et al., 2011; McPherson et al., 1999; Snell et al., 1997). In this context, it is important to investigate the effect of crystal growth rates versus crystal quality and size.
The first reported protein crystallization experiments in microgravity, performed in 1984, described the growth of lysozyme and b-galactosidase crystals on Spacelab-1 (Littke and John, 1984). Since then in subsequent space shuttle missions, unmanned satellite missions, on the Russian space station and on the International Space Station (ISS), more than 100 different proteins have been crystallized under microgravity conditions (DeLucas et al., 1986; Krauspenhaar et al., 2002; Snell et al., 1997; Timofeev et al., 2012a; Vallazza et al., 2002). In 1989, Asano et al. performed a series of crystal growth experiments for bovine pancreatic ribonuclease S under microgravity conditions using the COSIMA 2 system (Asano et al., 1992; Plaas-Link and Cornier, 1988). The microgravity-grown ribonuclease S single crystals revealed improved diffraction resolution compared to ground-grown crystals of equal size (Asano et al., 1992). In another experiment, crystals of uridine phosphorylase from Shewanella oneidensis MR-1 revealed improved quality for microgravity-grown crystals compared to 1g controls (Safonova et al., 2012). However, some crystallization experiments performed under microgravity conditions showed no significant improvement in crystal quality (Hilgenfeld et al., 1992; Strong et al., 1992).
Macromolecule purity is a major parameter in the crystal growth process such that removal of impurities and elimination of macromolecular heterogeneity improve the probability of growing higher quality crystals (Giege et al., 1986; McPherson et al., 1999; Vekilov and Rosenberger 1996). Crystal defects often originate from incorporation of molecular aggregates and other impurities into the lattice of a growing crystal (Adawy et al., 2015; Giege et al., 1986; McPherson et al., 1999; Vekilov and Rosenberger 1996). Hen egg-white lysozyme (HEWL) has been crystallized in the presence of HEWL dimers on earth and under microgravity conditions to investigate the effect of impurity incorporation into a growing crystal. It was observed that the HEWL crystals grown under microgravity conditions contain 4.5 times less HEWL dimers than control experiments performed on earth (Carter et al., 1999). Another experiment demonstrated that the presence of chicken egg-white lysozyme dimers in the crystallization solutions in microgravity reduced crystal size, increased mosaicity, and reduced the signal-to-noise ratio of the X-ray data (Snell et al., 2001). Yet in another investigation, no significant difference in impurity incorporation between microgravity and ground crystals was observed (Snell et al., 2001). To further explore the effect of macromolecular transport phenomena in crystallization processes, experiments on the ISS were performed. For this investigation, Plasmodium falciparum glutathione S-transferase (PfGST) (Liebau et al., 2002; Perbandt et al., 2015) and HEWL were crystallized in the presence of varying amounts of fluorescently labeled protein aggregate.
Materials and Methods
Recombinant Expression and Purification of the ProteinsPfGST from Plasmodium falciparum was expressed and purified as previously reported (Liebau et al., 2002; Perbandt et al., 2015) with few modifications. The recombinant PfGST was expressed in E. coli BL21 cells in overnight cultures at 19°C. The cells were harvested by centrifugation and resuspended in 1´ phosphate-buffered saline (PBS) buffer (pH 7.4). The cell suspension was sonicated, and the cell debris was removed by centrifugation at 17.000´g at 4°C for 1 h. The recombinant PfGST was purified applying glutathione affinity chromatography; additionally, PfGST tetramer was separated by gel filtration on a Superdex HiLoad 26/600 column (GE Healthcare). Monomeric hen egg lysozyme (HEWL) was obtained by subjecting commercially obtained protein (Biomedicals LLC) to size exclusion chromatography (Yarra-2000 column). To produce stable aggregates, the purified monomeric protein was subjected to crosslinking by using glutaraldehyde as the crosslinking agent. The fused protein was then reapplied to the size exclusion column to separate dimeric lysozyme from remaining monomeric protein.
Dispersity Analysis of the Protein Multimeric States
The dispersity and particle radius distribution of PfGST dimer (30 mg mL−1) and tetramer (10 mg mL−1) were determined and analyzed at room temperature by dynamic light scattering (DLS) applying the DLS system SpectroLightÔ 300 (Xtal Concepts GmbH, Hamburg, Germany). Time-resolved DLS measurements of hydrodynamic radius verified the monodispersity of PfGST dimer with RH = 3.7 ± 0.1 nm and tetramer with RH = 5.7 ± 0.1 nm solutions, respectively. To produce stable aggregates of HEWL, monomeric protein was subjected to crosslinking as described before and subsequently run over a size exclusion column to separate remaining monomer from dimers and higher aggregates. The purified and stable dimer was then fluorescently labeled as described in the following.
Fluorescent Labeling of Protein Aggregates
To investigate the amount of impurity incorporated into growing crystals, stable fluorescently labeled protein aggregates were prepared and subsequently added at different percent concentrations to nonlabeled monomeric protein suspensions. The PfGST tetramer and lysozyme dimer, acting as impurities in the crystallization experiments, were labeled with the fluorescent dyes Alexa Fluor® 488 TFP ester and Alexa Fluor® 594 NHS ester, respectively. The Alexa Fluor® 488 TFP ester (C39H44F4N4O11S2, MW = 884.9 Da) and Alexa Fluor® 594 NHS ester (C39H37N3O13S2, MW = 819.8 Da) were obtained from Thermo Fisher Scientific (Life Technologies). The Alexa Fluor® 488 TFP ester (5 mg) was dissolved in 0.5 mL of dimethyl sulfoxide. The reactive dye solution (80 μL) was slowly added to the stirring PfGST tetramer solution (10 mg/ml in PBS). The reaction was incubated for 1 h at room temperature with continuous stirring. The labeled tetramer was separated from free dye using a Sephadex® G-25 prepacked gel filtration column. The column was first equilibrated with PBS buffer and then loaded with a reaction mixture and eluted with PBS buffer solution. Labeling degree (DOL) of tetramer was calculated using following calculations:
The calculated DOL was approximately 4. The protein-dye conjugate was concentrated to 10 mg/ml final concentration using Millipore Amicon® ultra-centrifugal concentrators (Merck Millipore). For lysozyme aggregate labeling, a solution of buffered lysozyme dimer at 2 mg/mL was mixed with Alexa Fluor® 594 NHS ester at 22°C and incubated for 1 h. Unbound dye was removed via spin concentration (500 μL 30 MW cutoff spin concentrator).
Capillary Protein/Precipitant Filling and Sealing Procedure for Crystallization
Crystallization experiments were performed using the counter/ liquid–liquid diffusion technique in capillaries of 100 mm length, 3 mm width, and 0.3 mm inner diameter (VitroCom). The capillaries were filled with 37 μL of precipitant and 37 μL of protein solution (doped with different percentages of fluorescently labelled protein aggregate using syringes (Hamilton)). Lysozyme was prepared in 0.1 M NaOAc (pH 4.6) solution with the precipitant solution consisting of 1 M NaCl and 0.1 M NaOAc (pH 4.6). A sample of PfGST dimer and tetramer was prepared in 0.1 M NaHPO4 (pH 6.7) solution. The precipitant solution for PfGST consisted of 2.8 M AmSO4, 0.1 M NaHPO4 and 15% glycerol (pH 6.7). The length and width of all flight and ground control capillaries were measured to confirm that they were within stated limits. Capillaries were visually examined before filling to ensure that there are no visual defects, e.g. cracks and jagged ends. One capillary end was filled with Apiezon N cryogrease (Apiezon) using a plastic 25 mL syringe with a rubber or silicon tube that attached the syringe with the other end fit snugly over the capillary. Grease was extruded approximately 3–5 mm into the capillary end. All protein and precipitant solutions were degassed using “house” vacuum prior to use for the flight and ground control experiments. The capillary was filled with protein using a glass syringe (Hamilton) with a needle small enough to fit within the width of the capillary (i.e. < 0.3 mm width). This was followed by layering the precipitant solution against the protein solution and filling the capillary to approximately 3 mm from the other end of the capillary. After completely filling the capillary with protein and precipitant solution, the opposing end was filled with Apiezon N grease using a plastic 25 mL syringe with the same rubber/silicone tube as described previously. Five-minute drying Double Bubble epoxy (Hardman) was prepared, and each end of the capillary was dipped into the epoxy to a depth of approximately 2–3 mm and the capillary inspected to determine that the ends were completely sealed. The sealed capillary was then placed on a clay mount to dry for at least 5 min. The sealed capillary was inspected using a dissecting microscope (at approximately 15´–25´ magnification). The sealed capillaries were placed into a specially constructed cassette (ZIN Technologies) that allowed capillaries lie flat in cassette channels. After eight capillaries were positioned in the cassette, the top clamp (with the six washers previously placed in the screw holes) was carefully aligned and screws fastened using a hex wrench. To insure the capillaries were not damaged, the cassette top (clamp) was removed and the capillaries are visually inspected for possible cracks. If the capillaries were not damaged, the cassette top with the six washers (previously placed in the screw holes) was carefully aligned and refastened using a hex wrench. The capillary cassette was placed into a Bitran bag and then Bubble bag followed by immediate placement of the “bagged” cassette into a walk-in -20°C ± 2.0°C freezer overnight. The capillaries were reinspected for cracks after the overnight freezing process. Following the “slow freezing” of the “bagged” cassettes in the -20°C freezer, the bags were immediately placed into a -80°C ± 20°C freezer and maintained in a frozen state until on-orbit activation and observation in the Light Microscopy Module (LMM).
Two series of experiments were performed on ISS, one during 26.02.2017 to 10.03.2017 and a second during 16.06.2017 to 23.06.2017. The cassettes were launched aboard SpaceX (SpX-10) in cold stowage at -80°C. Upon reaching the ISS, the cassettes were transferred to ISS cold stowage (-80°C) while awaiting science operations. The cassettes were removed from cold stowage, thawed, and installed onto the LMM petri plate using Velcro. The LMM petri plate was installed in the LMM base adapter and the LMM prepared for powered science operations. The initial protein crystallization experiments, LMM Biophysics-1, were performed using the ISS LMM at a temperature of 20–23°C. Powered operations began as soon as practical after installation was completed
with initiation of the crystal search phase occurring within 4 h of cassette installation. The growth of crystals was monitored for several days. Crystal images were recorded with 2.5´, 10´ objectives. To investigate crystal growth rate and the fluorescence of crystals, Texas Red and FITC fluorescence filters were used.
Confocal Fluorescence Imaging Experiments
To investigate the incorporation of impurities into growing crystals for each protein, confocal fluorescence imaging experiments were performed. Crystal fluorescence images of both proteins were recorded on ISS using the LMM microscope, 2.5´ and 10´ objectives. Fluorescence imaging experiments on ground were performed using a Zeiss LSM 710 confocal laser scanning microscope (Carl Zeiss Microscopy). The capillaries were scanned with a 10´ magnification lens. To investigate the fluorescence of PfGST crystals, an FITC (excitation 475–495 nm; emission 515–545 nm) filter was used, and for lysozyme crystals, a Texas Red (excitation 540–580 nm; emission 590–630 nm) filter was used.
The image-analysis software ImageJ (developed at the National Institute of Mental Health, Maryland, USA) was then used to determine the size of crystals at different positions in the capillaries. The statistical analyses were performed using Origin (OriginLab Corporation) data analysis and graphing software tools as well as Microsoft Excel statistical tools (Microsoft Office 365 ProPlus, Microsoft Corporation). A two-tailed, unpaired t-test (Student’s t-test) was used to determine significant difference in mean values between different crystal groups within a 99% confidence interval.
Crystallization in Microgravity
The flight cassettes were installed on the LMM microscope after sample thawing to perform crystallization experiments. Grown lysozyme crystals showed nearly similar morphologies in each capillary and were photodocumented in the LMM (Figure 2A)PfGST needle-like crystals were observed (Figure 2B) Furthermore, crystals of different sizes at different capillary areas were observed for both proteins.
The length of the major axis for lysozyme and PfGST crystals smaller in size was measured to be 150–200 mm and 150–320 mm, respectively, and for crystals larger in size was measured to be 450–560 mm and 500–780 mm, respectively (Figure 2A and B)
Crystal Growth in Microgravity
Time-lapse images for different capillary areas were recorded to investigate crystal growth rates for lysozyme (Figure 3) and PfGST (Figure 4) crystals in microgravity. At the time points t = 253 min and t = 612 min, nucleation and subsequent growth of lysozyme crystals were not observed (Figure 3). However, at time points t = 1416 min, t = 3214 min, and t = 8725 min, growth of lysozyme crystals was observed and their growth rates were photo-documented (Figure 3).
PfGST crystals were first observed at the time point t=3266 min after sample thawing (Figure 4). The PfGST crystal dimensions and amount of crystals varied for several observed areas in capillary (Figure 4). The growth rate values as well as the dimensions (length of major axis) of lysozyme and PfGST crystals for different areas along the capillary were determined. The growth rate values for the n = 15 lysozyme and n = 6 PfGST crystals were determined.
According to the experimental results, the average growth rate (1.9 ± 0.23 mm/h) for lysozyme crystals with the length of major axis < 350 mm was significantly lower (statistical t-test: p < 0.01) than the average growth rate (2.6 ± 0.24 mm/h) for crystals with the length of major axis > 350 mm (Figure 5A) The average growth rate (2.4 ± 0.28 mm/h) for PfGST crystals with the length of major axis < 200 mm was significantly higher (Student’s t-test: p < 0.01) than the average growth rate (1.2 ± 0.13 mm/h1) for crystals with the length of major axis 300,400 mm (Figure 5B) The distribution of crystal size values (length of major axis) for lysozyme and PfGST crystals along the capillary was observed. The crystal size for both proteins at different positions in the capillaries was measured and comparatively statistically analyzed. The area in the capillary was measured from the end of capillary (i.e. the protein). Temporarily, the length of major axis values for the n = 39 lysozyme and n = 61 PfGST crystals was measured. The average dimensions (length of major axis) of lysozyme crystals were calculated in two areas from the capillary end, 13–25 mm and 25–44 mm with crystal sizes 277 ± 27 mm and 495 ± 47 mm, respectively. The average size of lysozyme crystals was significantly lower (Student’s t-test: p < 0.01) for the capillary area between 13 and 25 mm than the average size for the capillary area between 25 and 44 mm (Figure 5C)
The average size of PfGST crystals was calculated in the four areas from the capillary end, 26–29 mm, 29–35 mm, 35–41 mm, and 41–44 mm, with crystal sizes 158 ± 30 mm, 380 ± 54 mm, 770 ± 55 mm, and 571 ± 54 mm, respectively. A significant difference for the average crystal sizes from all four capillary areas (Student’s t-test: p < 0.01) was observed. Significance for the area 26–29 mm and 29–35 mm (p < 0.01), significance for the area 26–29 mm and 35–41 mm (p < 0.01), significance for the area 26–29 mm and 41–44 mm (p < 0.01), significance for the area 29–35 mm and 35–41 mm (p < 0.01), significance for the area 29–35 mm and 41–44 mm (p < 0.01), and significance for the area 35–41 mm and 41–44 mm (p < 0.01) are indicated (Figure 5D)
Impurity Incorporation into Growing Crystals in Microgravity
To investigate the incorporation of impurities into growing crystals for each protein, fluorescently labeled protein aggregates were prepared that simulated protein aggregate impurities in solution. For crystallization experiments in microgravity, samples with different protein aggregate ratios were prepared.
The LMM fluorescence micrograph of a capillary sample containing PfGST dimer and additionally fluorescently labeled PfGST aggregates (95.5:0.5 total ratio) shows the presence of fluorescence (white) in PfGST crystals grown in microgravity (Figure 6A) Initial crystallization experiments showed that fluorescently labeled PfGST aggregates are not crystallizing under same conditions as PfGST dimers. Since samples returned to the Earth, confocal images of crystals in the capillaries were recorded and photodocumented. The PfGST and lysozyme crystals grown in microgravity in the presence of fluorescence-labeled protein aggregates show the presence of fluorescence, green for PfGST crystals (Figure 6B) and red for lysozyme crystals (Figure 6C)
Since 1984, protein crystallization experiments have been conducted in microgravity to obtain crystals of higher X-ray diffraction quality (DeLucas et al., 1986; Kundrot et al., 2001; Littke and John, 1984; McPherson et al., 1999; Snell et al., 1997). It is assumed that a convection-free, diffusion-controlled environment will support growth of crystals of higher quality, which can be achieved using microgravity. The capillary counter diffusion method is an efficient technique to investigate diffusion-limited mass transport phenomena in macromolecular crystallization (García-Ruiz et al., 2001b; García-Ruiz, 2003).
This investigation addresses the following hypothesis:
Improved quality of microgravity-grown protein crystals is the result of two macromolecular characteristics that exist in a buoyancy-free, diffusion-dominated solution
- –slower crystal growth rates, due to slower protein transport to the growing crystal surface and
- –predilection of growing crystals to incorporate protein monomers versus higher protein aggregates due to differences in transport rates
Experiments were performed in microgravity and in laboratory controls to compare the effect of diffusional mass transport on crystal growth rate, crystal size, and impurity incorporation. The results for both proteins, lysozyme and PfGST, reveals growth of crystals with different sizes at different positions along the capillary (Figures 2A and B and 5C and D) The concentration variations of the protein–precipitant solution along the length of the capillary influence the interaction of protein precipitation. In addition, the diffusive macromolecular mass transport leads to a supersaturation gradient along the capillary resulting in crystals of different size ranges along the length of the capillary (García-Ruiz, 2003; García-Ruiz et al., 2016). This is due to a gradient of crystallization conditions produced along the capillary. Changes in the average size of the lysozyme crystals were only observed in two areas within the capillary. Crystals grown between 25 and 44 mm along the capillary (from the capillary end) are on average significantly larger compared to crystals grown in the area between 13 and 25 mm (Figure 5C) Analogous to the lysozyme crystallization results, changes in the average sizes of the PfGST crystals were observed such that the average sizes of PfGST crystals increased in the capillary area from 26 to 41 mm from the capillary end (also it started to decrease again in the area from 41 to 44 mm along the capillary; Figure 5D) As the counter diffusion method is based on mixing protein and precipitate solution by diffusion in opposite directions, it is assumed that lysozyme molecules diffuse an order of magnitude more slowly than the precipitant. This is caused by the fact that proteins reveal lower diffusion coefficient values in liquid environments compared to the diffusion coefficient values of the small molecule (salt ions) precipitant (Brune and Kim, 1993; Tyn and Gusek, 1990). Therefore, the concentration of precipitant in a capillary containing lysozyme increases at a faster rate than the concentration reduction of lysozyme in the same area of the capillary. In this context, the concentration of lysozyme in the area of the capillary initially containing the precipitant increases at a slower rate than the reduction of concentration of the precipitant in the same area of the capillary. This process produces an initial supersaturation wave in the protein area/side of the capillary, subsequently generating nucleation events and crystal growth (García-Ruiz et al., 2001b). This explains the observed growth of lysozyme and PfGST crystals in the initial protein area within the capillaries. It is supposed that nucleation and subsequent crystal growth occur at high protein and precipitant concentration values (at the interface between the protein and precipitant) and also at a high value of supersaturation and nucleation degree (Otálora et al., 2009). The supersaturation degree and the diffusion coefficient values change along the capillary over time, generating additional nucleation events. The supersaturation rate decreases with time, and the nucleation process and crystal growth occur at slower rates (Otálora et al., 2009; García-Ruiz et al., 2016). This effect of diffusional mass transport on nucleation and crystal growth is responsible for the observation of different crystal dimensions and different average growth rates for crystals in different positions along the capillary (Figures 2 and 5). Presumably within the diffusional gradients, crystal dimensions change proportionally to changes in nucleation and growth rates of crystals. As a result, the process whereby a gradient of precipitant concentrations naturally results in a position in the capillary with specific nucleation and growth rates that produce larger and improved crystal quality. For lysozyme, the estimated position with certain conditions optimal for the crystallization corresponded to the area 25–44 mm from the capillary end (Figure 5C) The size distribution of PfGST crystals presented in Figure 5D shows that the on average, the largest crystals were grown in the area 35–41 mm. It is assumed that in this area, conditions optimal for crystallization were originated over time by the diffusion-controlled macromolecular mass transport.
In previously reported studies, crystallization experiments were performed to investigate the relation between impurity incorporation and protein crystal growth process (Adawy et al., 2015; Carter et al., 1999; Snell et al., 2001). Our study involves fluorescently labeled protein aggregates to represent the impurities in the growth solution. The PfGST protein solution contained 0.5% of fluorescently labeled PfGST aggregates (Figure 6A) The analyzed data with respect to impurity incorporation into growing crystals are displayed in Figure 6. The LMM fluorescence micrograph and the confocal microscopy images of PfGST and lysozyme crystals show the presence of fluorescence in crystals. These initial data indicate that the crystals incorporated notable quantities of fluorescently labeled impurities.
In summary, the manuscript reports that comparative crystallization experiments using the ISS LMM facility were successfully performed in microgravity using an innovative capillary counter diffusion technique. Future studies will involve a statistical analysis of the percentage incorporation of impurities (via quantitative analysis of total fluorescence/crystal volume) incorporated into microgravity versus unit gravity grown crystals. This future research will address hypothesis 2: the diffusion-limited crystal growth environment producing a self-purifying process may dominate due to slower transport rates for larger aggregates in a diffusion-limited environment. This hypothesis assumes that crystal growth in microgravity benefits from a principally purer solution (less aggregate incorporation) than crystals in the presence of convective forces (Carter et al., 1999; McPherson et al., 1999).
The authors would like to thank all the people who have been involved in the SpaceX SpX-10 mission. The authors would like to thank all the crew members of ISS expedition 50 and 52. The authors would also like to thank all the participants (i.a. Zin Technologies) of Biophysics—1 project. This research has been supported by the NASA (Grant No. 80NSSC18K0013) and Deutsche Luft und Raumfahrt Agentur (DLR) (Grant No. 50WB1423). The authors also acknowledge UAB High Resolution Imaging Service Center, Shelby 135c, Confocal/Light Microscopy Core at the University of Alabama at Birmingham.
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