Polysaccharide chemistry regulates kinetics of calcite nucleation through competition of interfacial energies
See allHide authors and affiliations
Edited by Bruce Watson, Rensselaer Polytechnic Institute, Troy, NY, and approved April 18, 2013 (received for review December 20, 2012)

Abstract
Calcified skeletons are produced within complex assemblages of proteins and polysaccharides whose roles in mineralization are not well understood. Here we quantify the kinetics of calcite nucleation onto a suite of high-purity polysaccharide (PS) substrates under controlled conditions. The energy barriers to nucleation are PS-specific by a systematic relationship to PS charge density and substrate structure that is rooted in minimization of the competing substrate–crystal and substrate–liquid interfacial energies. Chitosan presents a low-energy barrier to nucleation because its near-neutral charge favors formation of a substrate–crystal interface, thus reducing substrate interactions with water. Progressively higher barriers are measured for negatively charged alginates and heparin that favor contact with the solution over the formation of new substrate–crystal interfaces. The findings support a directing role for PS in biomineral formation and demonstrate that substrate–crystal interactions are one end-member in a larger continuum of competing forces that regulate heterogeneous crystal nucleation.
Efforts to decipher patterns of biomineralization have identified proteins and polysaccharides (PSs) as major components of the organic matrices associated with sites of calcification. In mollusks and other organisms including the red algae, coccolithophores, and foraminifera (1, 2) (Table 1), calcifying macromolecules are dominated by functional groups with an acidic character—proteins that are rich in carboxylated amino acids (14) and PSs that are highly sulfated and carboxylated (15, 16). Although a physical picture of these interactions is not well developed, this recurring affiliation of carboxylate and sulfate groups with zones of mineralization in organisms suggests specific roles for macromolecules in nucleation and growth. Early studies have led the biomineralization community to generally assume that charged proteins actively regulate mineralization. In contrast, PSs, such as the chitin found in the insoluble fraction of the mollusk shell, are thought to provide an inert scaffolding to support these proteins (17, 18).
Examples of polysaccharides found at sites of CaCO3 mineralization from diverse phyla
Recent studies challenge this assumption with qualitative evidence that PSs can also promote calcium carbonate (CaCO3) mineralization (19, 20) (Table 1). For example, specific orientations of chitin fibers with neutral functional groups promote the templating of CaCO3 in the lobster carapace (13, 21), crab cuticle (21), and nautilus shell (22). More generally, the monosaccharide sequences along PS chains can influence biological function and their interactions with proteins (23). This suggests PS chemistry and interactions with proteins could regulate patterns of mineralization.
Anecdotal observations from in vitro studies also support the thinking that PSs influence mineral formation, but their specific effects are unclear. For example, PSs with higher carboxyl and sulfate content promote either faster (24, 25) or slower (26, 27) rates of CaCO3 nucleation. Although these results seem inconsistent at first glance, the differences are likely attributable to the diverse experimental designs that were used across disciplines and, in some cases, with little control over chemical conditions. Although qualitative, insights from in vivo and in vitro studies provide evidence that the chemical structure of PSs can indeed control calcite nucleation. They also raise the question of whether there is an underlying relationship between homologies of mineralization and the functional group chemistry of monosaccharide sequences, and more generally, the chemistry and structure of macromolecules.
To test this idea, we designed an experimental study to quantify the underlying energetic controls on calcite nucleation. A suite of high-purity PSs with regular monomer sequences and simple functional group chemistry were chosen as model compounds for the complex PSs found in calcifying organisms (Fig. 1). Heparin is the most highly charged PS of the group with carboxyl and sulfate groups, whereas amine groups give chitosan a small net positive charge. Two alginates provided a test of how stereochemistry influences nucleation through different proportions of the stereoisomers mannuronic and guluronic acid.
Polysaccharide chemical structures illustrate the functional groups attached to 2-carbon (red) and 6-carbon (blue) of each ring. (A) De-N-sulfated heparin contains amine, acetylamine, carboxyl, and sulfate groups. R is 80% H and 20% COCH3. Ninety percent of carboxyl groups are in axial positions. (B and C) Alginates contain carboxyl groups with different proportions of guluronic acid monomer content. (D) Hyaluronate contains acetylamine and carboxyl groups. (E) Chitosan contains amine and acetylamine groups. (F) Cellulose, with only hydroxyl groups, was not used in study and is included for comparison.
Using a flow-through method that controlled for solution chemistry (28) we quantified the number of crystallites that formed on each type of PS substrate. These were prepared by electrodeposition onto gold using established methods. Rate measurements assumed that each nucleus that achieved a critical radius subsequently continued to grow into an observable crystallite. The number of crystals per square millimeter was counted in a sequence of time-lapsed images to determine nucleation rates (Fig. 2 A–D, Insets) across a series of solution supersaturations, σ, defined bywhere ai is the activity of species i and Ksp is the equilibrium solubility constant (10−8.48 for pure calcite at 25 °C). The σ varied from 4.83 to 5.63 at a constant solution pH of 10.8 ± 0.1, [Ca2+]/[CO32−] of 1.0, temperature of 25.0 ± 0.5 °C, and total ionic strength of 0.007–0.013 M. Despite the high supersaturations that exceeded the solubility of amorphous CaCO3, only calcite crystallites formed under these conditions, as identified by their rhombohedral morphologies and consistent with previous work (28).
Calcite steady-state nucleation rates obey classical nucleation theory (Eq. 2) and show PS-specific dependence on B, a proxy for the thermodynamic barrier to nucleation. Data are quantified from slopes of experimental rate data shown in insets. (A) Heparin, B = 376 ± 60; (B) LG alginate (red circles), B = 390 ± 11 and HG alginate (blue circles), B = 294 ± 45; (C) hyaluronate, B = 253 ± 58; and (D) chitosan, B = 121 ± 22. SEs of ln(Jo) are smaller than the diameter of symbols. (E) Trends in A–D extrapolated to (1) large and (2) small supersaturations predicts reversal in relative order of nucleation rates.
Results and Discussion
The number of calcite crystallites that nucleated and grew on the PS substrates was proportional to the driving force, σ, of the reactant solution (Fig. 2 A–D, Insets). Rates were also PS-specific, with the highest and lowest number densities measured for heparin and chitosan, respectively (Fig. 2 A and D).
To quantify the thermodynamic basis for these differences, we evaluated the linear portion of the nuclei versus time data using classical nucleation theory (29, 30) (SI Text, section S1). The linear form of the general nucleation expression states that the flux of new nuclei onto a substrate is described bywhere Jo is the steady-state rate of heterogeneous nucleation (m−2⋅s−1); A is dependent upon kinetic factors that include rates of ion desolvation, attachment, and detachment; and slope, B, is given by
where F is a nucleus shape factor, ω is the molecular volume of calcite, kB is the Boltzmann constant, T is temperature, and γnet is the net surface free energy of the crystal–substrate–liquid system (mJ⋅m−2). Assuming that ω is relatively constant, the experimental variable within B is γnet for a constant T. Because B is a proxy for the thermodynamic barrier to the nucleation (SI Text, section S1), its dependence upon γnet represents the contribution of surface energies to the energy barrier. Eq. 2 gives a good fit to the rate data and shows that at the highest supersaturations substrates rich with carboxyl and sulfate functional groups (Fig. 2 A–C) promote the fastest nucleation rates, whereas the slowest rates occur on chitosan surfaces (Fig. 2D).
By evaluating the slopes of these trends, we find that values of B are PS-specific. The highest slopes, and thus the highest energy barriers to nucleation, are correlated with the charge-dense substrates [low-guluronic-acid (LG) alginate and heparin]. In contrast, nucleation onto chitosan substrates shows the lowest slope. Because B is directly proportional to surface energy cubed (Eq. 3), we can deduce that a low value of B is correlated with a low net surface energy. Our estimate of a low γnet for chitosan is consistent with the surface energy values reported in a previous nucleation study (31). Comparisons of the two alginates show the form with high guluronic acid (HG) content has a smaller thermodynamic barrier to nucleation than LG alginate.
To decipher the physical basis for nucleation barriers estimated for each PS, we first examine the dependence of B on net charge. The expected charge per monosaccharide is estimated using reported acid dissociation constants of the functional groups for each PS and chemical characterizations by the vendor (SI Text, section S2 and Table S1). For our experimental conditions (final pH of the mixed solutions, 10.8 ± 0.1), carboxyl and sulfate functional groups are negatively charged, whereas hydroxyl, acetylamine, and amine groups have a neutral or slightly positive net charge. PSs with mixed functional group chemistry are assigned an average charge.
By correlating the average monosaccharide charge of each PS with B, we find a direct relationship (Fig. 3A). Heparin and the alginates, which derive a higher negative charge from carboxyl groups, are correlated with greater B values and, therefore, greater thermodynamic barriers to nucleation (Fig. 3A). In contrast, the small net positive charge of chitosan is associated with the lowest energy barrier to nucleation. The relationship in Fig. 3A suggests net charge of a PS influences nucleation through the surface free energy of the substrate–liquid–crystal system.
Kinetic measurements provide insights to controls on thermodynamic barriers to nucleation. (A) Barriers are inversely correlated with charge density such that near-neutral PSs present the lowest barrier to calcite formation. (B) Measurements of surface free energy in air, a proxy for γSL, provide evidence for a competition between solvent and crystal interactions with the PSs that correlate with hydrophilicity. (C) Relationship between energy barrier and charge density can also explain the very high energy barrier measured on carboxylated SAMs. Offsets between SAMs and alginates of different chain lengths and stereochemistry suggest functional group structure and conformation also tune barrier height. SEs of B are derived from the linear fits of Eq. 2 to data in Fig. 2.
We can relate the observed trend to the underlying crystal– and solution–substrate interactions by evaluating the factors that influence the value of γnet contained in B. The net surface free energy, γnet, is a composite of three contributions:where γij is the interfacial free energy of the liquid–crystal (LC), substrate–crystal (SC), and substrate–liquid (SL) interface, and h is a nucleus shape factor (for example, h = 1/2 for a hemisphere). For the conditions of these experiments, we assume that γLC is approximately constant. Thus, the higher values of B that we estimate for nucleation onto the most negatively charged PS are associated with large γSC, small γSL, or some combination of the two.
In principle, one can test the hypothesis that large negative charge is the basis for the large barrier to nucleation via smaller substrate–liquid energies by conducting independent measurements of γSL for each of the PS substrates. Unfortunately, this quantity is difficult to measure. Instead, we measured γS-air using established methods (32⇓–34) (Fig. S1, Table S2 and SI Text, section S3) to serve as a rough proxy for γSL. This value also provides insight on the hydrophilicity of the substrates. That is, surfaces with a large amount of charge prefer interaction with polar water molecules and therefore exhibit greater surface free energies while exposed to air and smaller surface free energies in water. Recall that smaller γSL, which corresponds to larger γS-air, contributes to a greater γnet (Eq. 4) and thus a higher thermodynamic barrier to nucleation. Indeed we find PS substrates with high measured values of γS-air correlate with greater thermodynamic barriers to nucleation (Fig. 3B).
The trends in Fig. 3 A and B thus suggest the possibility of a broader relationship that could explain calcite nucleation behavior onto substrates ranging from neutral to highly charged. Measurements of energetic barriers to calcite nucleation onto carboxylated self-assembled monolayers (SAMs) provide insights into the influence of highly charged functional groups that are found in proteins and PSs in mineralizing systems (28). Due to the greater hydrophilicity of these substrates, this method of measuring γS-air cannot be used because the contact angles lie outside of the accessible range. Instead, we estimate the surface charge density from pKa values of functional groups and packing density of the SAMs or PSs (SI Text, section S4). Fig. 3C shows that, indeed, charge density is correlated with the barrier height to calcite nucleation along a single trend that includes the SAM substrates.
The implication of Fig. 3C is that charge density through functional group chemistry has a primary control on the barrier to nucleation through differences in γSL. Small offsets in B between the two alginates and the carboxylated SAMs (Fig. 3C) suggest that differences in the structure of substrates with similar charge densities further regulate the barrier height. This conclusion is supported by recent simulations showing that variations in head group geometry that arise from SAM–monomer interactions cause subtle differences in substrate–crystal interfacial energies (35). Thus, nucleation barriers are largely controlled by substrate charge density through γSL and further regulated by small differences in γSC through subtle variations in structure.
Our results demonstrate the energy barrier to calcite nucleation is determined by a competition between the energetics of crystal nucleus attachment to a substrate and creating new interface (γSC) versus the energetics of eliminating a solvated substrate (γSL). By minimizing the change in free energy through these thermodynamic drivers, the systematic relationship between nucleation and the chemistry and structure of substrate environments can be understood. Hydrophilic substrates prefer to maintain the substrate–water interface, thus presenting a high barrier to making a new substrate–crystal interface. In contrast, neutral to less-hydrophilic surfaces present a lower thermodynamic barrier to displacing water to form a new substrate–crystal interface and thus to mineral nucleation. This interpretation of the experimental data expands upon the conclusions of earlier computational studies that explored the importance of surface ionization, as well as the competition between the energies of the substrate–crystal and liquid–crystal interfaces (36).
At first glance, the higher energy barriers we estimate for nucleation onto charged surfaces are counterintuitive given the long-standing perception that negatively charged functional groups promote nucleation by strong interactions with Ca2+ ions (14, 15, 37, 38). Moreover, a number of studies observe that calcite crystallites are preferentially formed on carboxyl-patterned regions, in sharp contrast to the surrounding hydrophobic methyl-functionalized areas (39⇓–41).
To understand why these seemingly disparate observations are consistent, recall that energy barriers are constant for a given substrate–liquid–crystal system and nucleation rates are dependent upon σ−2. Thus, for any two substrates, there must be a value of σ above which, paradoxically, the one with the higher value of B gives faster nucleation rates (Fig. 2E). Because the studies described above were conducted at very high levels of supersaturation, the charge-dense macromolecules produced the most crystallites over short time intervals. Fig. 2E shows that as supersaturation is lowered these trends eventually flip and neutral substrates with lower energy barriers promote the fastest rates of nucleation (Eq. 2). This physical picture reiterates the point that whereas energy barriers to nucleation at a given supersaturation are constant and substrate-specific, the local supersaturation environment has the overarching control on relative rates of nucleation onto charged versus neutral substrates.
The findings suggest a simple mechanism-based framework for understanding nucleation as a continuum of substrate–liquid–crystal interactions that are governed by acidic and neutral chemical domains, irrespective of macromolecular class. The possibility of regulating the onset of nucleation by this construct suggests the need to revisit the long-standing assumptions regarding the roles of neutral and acidic macromolecules at sites of calcification. If near-neutral macromolecules present a lower energy barrier to nucleation by promoting the formation of new substrate–crystal interfaces, an important part of the mineralization picture may be currently missing.
Implications
There are a number of implications for interpreting the origins of biominerals that form in organisms and for better controls on materials synthesis. By establishing a physical basis for how macromolecule chemistry favors or inhibits biomineral nucleation, it may be possible to interpret patterns of skeletal biomineralization through geologic time using an inverse approach. That is, differential expression of PSs and proteins with varying charge density, in concert with local supersaturation, regulate the placement, timing, and extent of mineral nucleation. For example, modern mollusks induce mineralization at epithelial membranes within neutral chitin matrices using acidic proteins, hydrophobic silk proteins, and glycosaminoglycans in the growth front of the shell (19, 41⇓–43). Recall that the chitin and glycosaminoglycans found in organisms are, in fact, glycoproteins (17, 18, 44).
These results also cast light on the processes of crystal templating and epitaxy. Heterogeneous nucleation theory has long recognized the contributions of interfacial energies as the primary drivers to minimizing the overall energy of the system (45). However, conventional wisdom focused on epitaxy mechanisms and assumed that substrate–crystal interactions were predominant in nucleating environments (30, 46). Our findings show this assumption must now be reconsidered within a broader mechanistic framework whereby the drivers to nucleation are a continuum of substrate–liquid–crystal interactions. This explains why the basic tenets of classical nucleation theory have always allowed for the possibility that poor substrate–crystal interfaces can promote nucleation. We show this can occur by eliminating a less favorable substrate–liquid interface. By considering nucleation as a continuum of interactions, a new paradigm for understanding diverse nucleation phenomena may emerge.
Materials and Methods
Preparation of PS Films.
PS substrates were deposited onto gold-coated Si wafers (Platypus Technologies) using established electrodepostion protocols (47⇓⇓–50). The electrodeposition apparatus consisted of two ∼1.5-cm2 wafers that were held 15 mm apart by a Teflon spacer and connected to an electrophoresis power supply using stainless steel alligator clips. For each type of film, the electrodes were submerged in 0.05% solutions of LG sodium alginate (<50% guluronic acid; Novamatrix), HG sodium alginate (>75% guluronic acid; Novamatrix), sodium hyaluronate (Novamatrix), chitosan chloride (75–90% deacetylated; Novamatrix), and de-N-sulfated heparin (20% N-acetylated; Sigma Aldrich), prepared at room temperature by gently mixing into 18.2 MΩ·cm ultrapure water for 1 h. The film was deposited by applying 20 V for 15–25 min. The integrity of PS film was confirmed before and after crystallization by SEM imaging or Alcian Blue (Sigma Aldrich) staining of carboxylated PSs.
Measurement of Nucleation Rates.
Rates of heterogeneous calcite nucleation were measured using a flow-through method that maintained controlled supersaturation conditions for the duration of each experiment. Experiments began by placing a freshly prepared substrate inside an acrylic glass flow chamber (25-mm diameter and 1.5-mm depth) and sealed with a glass coverslip. Solutions of 3–7 mM CaCl2⋅2H2O (≥99%; Sigma Aldrich) and Na2CO3 (99.997%; Alfa Aesar) were prepared and placed in two polypropylene syringes that were connected to the flow chamber with Tygon tubing and a T junction. The syringes were loaded onto a high-precision syringe pump (PHD 2000 Infusion; Harvard Apparatus) and dispensed at a constant flow rate of 30 mL/h. Before each crystallization experiment, the substrate, flow chamber system, and tubing were flushed with distilled deionized water. The experiments were conducted at a suite of solution supersaturations, σ, ranging from 4.83 to 5.63, but were held at constant pH of 10.8 ± 0.1, constant [Ca2+]/[CO32−] = 1, and constant temperature of 25.0 ± 0.5 °C. The short residence time of solution in the flow chamber allowed us to assume that solution pH and σ remained constant for the entire experiment.
Each experiment proceeded by collecting time-lapse images of crystallites that formed onto the substrates as a series of time-lapse images under an optical microscope at 10× magnification. Rates of nucleation were determined using only data within steady-state nucleation conditions. We assumed all nuclei that achieve a critical size grow into an observable crystallite. The maximum duration of an individual experiment was 1 h, at which time the substrate was removed and rinsed with ethanol.
Measurements of Surface Free Energy.
The γS-air measurements were conducted using a well-established method (32⇓–34). Static contact angle, θ, was measured with a goniometer on electrodeposited PS substrates using three test liquids: 18.2 MΩ·cm ultrapure water, glycerol (99.5%; Fisher), and ethylene glycol (99.7%; Aldrich) with known polar and dispersive components to surface free energy (γLp and γLd). Six angle measurements (three left and three right) were made on three replicate droplets of each test liquid (SI Text, section S3 gives details).
Acknowledgments
We thank J. D. Rimstidt and M. Roman for thoughtful insights and discussions. This research was supported by US Department of Energy (USDOE) Grant DOE BES-FG02-00ER15112 (to P.M.D.) and National Science Foundation Grant NSF OCE-1061763. This work was also supported by the Office of Science, Office of Basic Energy Sciences, Division of Chemical Sciences, Geosciences, and Biosciences of the USDOE under Contract DE-AC02-05CH11231.
Footnotes
- ↵1To whom correspondence should be addressed. E-mail: dove{at}vt.edu.
Author contributions: A.J.G., L.M.H., N.H., J.J.D.Y., and P.M.D. designed research; A.J.G. performed research; A.J.G., L.M.H., N.H., J.J.D.Y., and P.M.D. analyzed data; and A.J.G., J.J.D.Y., and P.M.D. wrote the paper.
The authors declare no conflict of interest.
This article is a PNAS Direct Submission.
This article contains supporting information online at www.pnas.org/lookup/suppl/doi:10.1073/pnas.1222162110/-/DCSupplemental.
Freely available online through the PNAS open access option.
References
- ↵
- ↵
- Usov AI,
- Bilan MI,
- Klochkova NG
- Takano R,
- Hayashi J,
- Hayashi K,
- Hara S,
- Hirase S
- Leadbeater BSC,
- Riding R
- de Vrind-de Jong EW,
- et al.
- Marsh ME,
- Chang D-K,
- King GC
- Weiner S,
- Erez J
- ↵
- ↵
- Weiner S,
- Hood L
- ↵
- Watabe N,
- Wilbur KM
- Crenshaw MA,
- Ristedt H
- ↵
- Wada K
- ↵
- Rudall KM
- ↵
- ↵
- ↵
- ↵
- ↵
- ↵
- ↵
- Borman AH,
- et al.
- ↵
- Arias JI,
- et al.
- ↵
- ↵
- ↵
- ↵
- Nielsen AE
- ↵
- Chernov AA
- ↵
- ↵
- ↵
- Rabel W
- ↵
- ↵
- ↵
- ↵
- Addadi L,
- Moradian J,
- Shay E,
- Maroudas NG,
- Weiner S
- ↵
- Suzuki M,
- et al.
- ↵
- ↵
- ↵
- ↵
- Addadi L,
- Joester D,
- Nudelman F,
- Weiner S
- ↵
- Marxen JC,
- Hammer M,
- Gehrke T,
- Becker W
- ↵
- ↵
- Volmer M,
- Weber A
- ↵
- ↵
- ↵
- ↵
- ↵
- Lide DR
Citation Manager Formats
Article Classifications
- Physical Sciences
- Earth, Atmospheric, and Planetary Sciences