Phase transitions in biogenic amorphous calcium carbonate

Mapping CaCO₃ Phases in Spicules.

Sea urchin spicules were embedded in epoxy, polished to expose their cross-sections, and then coated as described in refs. 19 and 20. Once we identified a spicule with real-time PEEM imaging, we remained on the spicule and acquired stacks of images at varying photon energies, scanning across the calcium L-edge. Typical images had a 20-μm, or smaller, square field of view, and contained 10⁶ pixels. Each pixel in a stack of images, therefore, had a size of 20 nm and contained a complete Ca XANES spectrum. With unique data processing software (21) we performed component analysis: We extracted a spectrum from each pixel and measured the proportion of each of the three component spectra shown in Fig. 1 (also see Figs. S1 and S2). The proportions were then displayed as colors in red, green, and blue (RGB) maps as the ones in Figs. 2 and 3 (also see Tables S1 and S2).

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Fig. 1.

The three reference spectra used for component analysis. (A) XANES spectra across the calcium L-edge extracted from sea urchin spicules. To minimize experimental noise, 6–10 independently acquired single-pixel spectra, with pixel sizes of 20 nm, were averaged to give each reference spectrum. (B) Spectra resulting from peak-fitting the spectra in A, which completely eliminates experimental noise from these spectra, thus they can be used as reference components for all analyses in this work. The red spectrum is hydrated amorphous calcium carbonate (ACC·H₂O, see Fig. S1), the green spectrum is anhydrous ACC, and the blue spectrum is crystalline calcite, as identified by Politi et al. (16). A comparison of the three spectra highlights that the main peaks labeled 1 and 3 do not vary across the three mineral phases, whereas peaks 2 and 4 do vary. Specifically, in red ACC·H₂O both peaks are low, in green ACC peak 2 is high and peak 4 is low, whereas in calcite both are high. More details on how these spectra were obtained are provided in Fig. S2 and Table S1.

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Fig. 2.

Component mapping in 48-h spicules, at the prism developmental stage, analyzed within 24 h of extraction from the embryo. (A) XANES-PEEM image of three spicules embedded in epoxy, polished to expose a cross-section, and coated. The image is an average of all 121 images acquired across the Ca L-edge. The larger triradiate portion of a spicule at the center is polished in plane, whereas two other cylindrical spicules at the top have their long axes perpendicular to the plane of the image. (B) RGB map displaying the results of component mapping, in which each component is color-coded as in Fig. 1. The box indicates the region magnified in C. (C) Zoomed-in portion of the RGB map in B, where each 15-nm pixel shows a different color. Pure phases are R, G, or B, whereas mixed phases are cyan, magenta, or yellow, according to the rules of additive color mixing: G + B = C, R + B = M, R + G = Y (59). The white vertical line shows the positions of the 20 pixels from which the spectra in D were extracted. (D) Sequence of 20 XANES spectra extracted from 15-nm adjacent pixels along the white line in C. The color-coding is the same as used in B, C, and Fig. 1. Notice that the white line in C runs from the outer rim of the spicule (red), passing through orange, yellow, green, cyan, and finally blue, toward the crystalline center of the spicule. Correspondingly, moving from bottom to top across the spectra in D, one can see peak-2 growth leading, and peak-4 emergence and growth lagging.

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Fig. 3.

RGB maps resulting from component analysis done on spicules extracted 36 h, 48 h, and 72 h after fertilization, analyzed within 24 h of extraction from the embryos. Horizontally, the spicules are ordered from most amorphous to most crystalline. Notice the large density of R and B pixels in 36-h, and 72-h spicules, respectively. See Table S2 for a quantitative analysis of R, G, B pixels. In the 48-h spicules R and G pixels, indicating amorphous phases, are always at the outer rims, whereas blue crystalline calcite is always at the center of each cross-section. Also notice that magenta nanoparticles are quite frequent (see spicules on the right, for instance). Magenta nanoparticles are made of colocalized ACC·H₂O and calcite. Insets on the right show zoomed-in maps of the four regions in white boxes on the 48-h and 72-h spicules on the right. (Insets) Pixels are 20 nm, and the color balance has been adjusted to enhance the magenta nanoparticle, otherwise faint, because magenta nanoparticles contain a much greater proportion of calcite than ACC·H₂O. These nanoparticles are 60–120 nm in size, and are consistently surrounded by blue calcite. See Fig. S3 for further spectroscopic analysis of the magenta nanoparticles.

We analyzed a total of 83 spicule cross-sections, from three samples, and distinct embryo cultures, extracted 36 h, 48 h, and 72 h after fertilization, respectively, and found consistent results. Fig. 3 shows a representative set of spicules with different orientations, sizes, and developmental stages.

Several observations stand out from the transforming, 48-h spicules in Figs. 2 and 3. First, red pixels, which contain pure ACC·H₂O, are usually localized at the periphery of the spicule, with few or none at the center. This finding is consistent with previous knowledge that new spicule mineral is deposited at the outer edges of the spicule (12, 13). One can conclude that the ACC·H₂O is short lived, and rapidly dehydrates after it is deposited on the spicule surface.

Dehydrated ACC green pixels are much more abundant than ACC·H₂O red pixels, and they too are preferentially localized all around the spicule outlines. Politi et al. (16) also used XANES-PEEM but were only able to analyze the surfaces of intact spicules, rather than cross-sections as presented here. They found that green ACC was the most abundant phase in forming spicules. Here we find 32% ACC in 48-h spicule cross-sections, whereas 72-h spicules do not show any residual green ACC in spicule cross-sections (Fig. 3, Table S2), which is consistent with previous Raman spectroscopy results (14).

Pure calcite blue pixels are concentrated at the center of the spicules. The sequence of spectra acquired going from the outside to the inside of the spicule cross-section (Fig. 2 C and D) shows the sequence of phase transformations, and their intermediates. This observation supplies direct evidence that the sequence of phase transformations leading to biogenic calcite is indeed ACC·H₂O → ACC → calcite. This sequence of transitions was hypothesized by Raz et al. (14) and Politi et al. (16) and then confirmed to be thermodynamically reasonable by Radha et al. (6). Our studies here directly observe these transitions in time and space in biogenic minerals.

We observe few yellow pixels (Y = R + G = ACC·H₂O + ACC), which is consistent with the paucity of red ACC·H₂O observed, and its short lifetime. There are, however, numerous cyan pixels (C = G + B = ACC + calcite) indicating that ACC in those pixels is transforming to crystalline calcite; but there are also abundant magenta pixels (M = R + B = ACC·H₂O + calcite, Fig. S3) even at the center of the spicules, where most of the mineral is already crystalline. This final observation was unexpected and led us to investigate how the short-lived ACC·H₂O persists in this way.

In Fig. S4 we present additional infrared data showing that spicules become progressively dehydrated as the embryo develops from 48 to 72 h (prism to pluteus stages), and the mineral crystallizes. Each infrared spectrum is strongly averaged over many spicules, and hence has significance for the chemical composition of spicules. The spatial distributions of Figs. 2 and 3 are in agreement with the infrared result, but provide much greater resolution. Notice in particular that in transforming spicules at 48 h the center of the spicules in cross-section is mostly crystalline, whereas amorphous phases tend to be localized at the outer rims.

The Persistence of ACC·H₂O.

Given the ACC·H₂O → ACC → calcite sequence of phase transitions established in Fig. 2, it is surprising that we find magenta nanoparticles of ACC·H₂O + calcite in the middle of the spicule cross-sections surrounded by blue calcite and not by green dehydrated ACC (Figs. 2 and 3). The magenta nanoparticles persist 2 mo after extraction from the embryo, as shown in Fig. S5. We hypothesize that there is an inhibiting agent that greatly delays or completely stops the transition from ACC·H₂O → ACC. This inhibitor is likely a protein or proteins because nucleic acids, lipids, and polysaccharides are not found in the spicule (22). We propose that when the inhibitory proteins are trapped in specific locations inside a crystallizing spicule, the ACC·H₂O in those locations cannot dehydrate.

Radha et al. (6) showed recently that both transitions ACC·H₂O → ACC and ACC → calcite have negative enthalpies of transformation. These transitions are energetically favorable and should happen spontaneously with time in the absence of inhibitory molecules. However, the persistence of ACC·H₂O in the magenta nanoparticles suggests that occasionally there is a high activation barrier for the ACC·H₂O → ACC transition perhaps because of proteins that inhibit this transition, thus stabilizing ACC·H₂O. Aizenberg et al. (23, 24) showed a similar function of polyanionic proteins in mollusk shells that stabilize ACC.

Our model simulation shows how the presence of dehydration-inhibiting protein(s) results in islands of ACC·H₂O after crystallization of the spicule (Fig. S6 and Movies S1 and S2). Crystallinity propagates through the fully formed, space-filling (25), three-dimensional anhydrous amorphous phase, following random-walk patterns in three dimensions. This mechanism was first described by Killian et al. (26) in the polycrystalline matrix of the sea urchin tooth, and we believe that it occurs identically in the sea urchin spicules studied here.

Persisting, long-lived nanoparticles of dehydrated ACC (green or cyan) are not found anywhere in spicule cross-sections. This result suggests that the dehydration and crystallization transitions have very different dynamics. These transitions happen in minutes in synthetic ACC, but much more slowly in spicules: Green and red pixels persist 24 h after extraction from the embryo (Figs. 2 and 3–48 h). Both transitions, therefore, must be inhibited in vivo.

In Fig. 3, compared to the newly formed 36-h, and the almost entirely crystalline 72-h, the transforming 48-h spicules are the most revealing to analyze and discuss in depth. Based on the spicules in Fig. 3, and the following considerations, we arrived at a schematic representation of the energy landscape of the ACC·H₂O → ACC → calcite transitions, and the hypothetical activation barriers between them, as presented in Fig. S7. First, the transitions from red to green (dehydration) and from green to blue (crystallization) are thermodynamically downhill (exothermic) (6). Second, the majority of ACC·H₂O is short-lived, as is evident from its paucity in 48-h spicules in Figs. 2 and 3–48 h, and its restriction to the zone of deposition at the outer rims of the spicules in transforming 48-h spicules. The dehydration transition, therefore, must be fast, and correspondingly the activation barrier for ACC·H₂O → ACC must be the smallest. Third, in 48-h spicules there are many more green pixels than there are red pixels (Figs. 2 and 3–48 h). In addition, in 48-h spicules analyzed 4 d after extraction, some green ACC is still detectable (see Fig. S5), therefore the activation barrier for ACC → calcite must be greater than that for ACC·H₂O → ACC. Fourth, in the presence of inhibiting protein(s), the activation barrier becomes much larger, because even 2 mo after extraction the ACC·H₂O in those magenta nanoparticles still had not dehydrated nor crystallized (see Fig. S5).

The Role of SM50 in Stabilizing ACC·H₂O.

We devised an assay to identify proteins that stabilize amorphous calcium carbonate mineral forms in vitro. A promising candidate is the sea urchin matrix protein SM50. SM50 is the most prevalent integral matrix protein from sea urchin embryonic spicules, as well as from adult spines, tests, and teeth (11, 27, 28). An incorrect amino acid sequence for SM50 was originally published in 1987 at the time of the report of the initial cloning of the SM50 gene and its cognate complementary DNA (29, 30). The corrected SM50 amino acid sequence was published in 1991 (31). The SM50 protein is neither glycosylated (32) nor phosphorylated (11, 32), and it has an alkaline pI (31, 32). In fact, SM50 is one of the most alkaline of the spicule matrix proteins (32). Previous studies have also shown that decreasing SM50 protein levels in sea urchin embryos causes spiculogenesis to stop (17, 33). The Lytechinus pictus sea urchin ortholog of SM50, designated LSM34, has also been shown to directly interact with mineralizing calcium carbonate (34).

Fig. 4 and Fig. S8 show the spectroscopic results of the in vitro assays for the proteins stabilizing amorphous mineral phases. In this assay, a water droplet dissolves the topmost layers of geologic calcite. If the droplet deposited is just water, then as the droplet dries and the water evaporates, the ion clusters recrystallize as calcite. If, instead, the inhibiting protein is present in the droplet solution, it prevents dehydration and crystallization, thereby making ACC·H₂O the spectroscopically detectable species in the dried droplet.

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Fig. 4.

Ca L-edge spectra acquired with XANES-PEEM on the surface of single-crystal calcite wafers, after depositing a droplet of water or protein in water, and letting it air dry. All data were acquired at the edge of each dried droplet, thus the two spectra in each plot were acquired simultaneously (magenta and blue curves). (A) The water droplet suspends a few ions or ion clusters, which then reprecipitate as calcite. The lower intensity crystal field peaks (vertical lines) in the H₂O-dried droplet spectrum indicate a polycrystalline calcite precipitate. (B) Cdk1 is a yeast cell cycle kinase expressed and extracted with the same methods used for SM50. This control spectrum also shows calcite reprecipitation. (C) PPL A2 is another protein present in sea urchin spicules (11). (D) The BSA dried droplet was very thick, hence the Ca signal is weak and noisy, but clearly calcite. (E) In the presence of the spicule matrix protein SM50 the reprecipitate is not calcite but hydrated ACC. (F) The SM50 spectrum from E, overlapped with the fitted ACC·H₂O from Fig. 1B (red curve). The two spectra are very similar. Hence we deduce that SM50 stabilizes ACC·H₂O, even in a dried droplet, in ultra-high vacuum, and in direct contact with a crystalline calcite wafer.

We tested SM50 because it is a very prevalent spicule matrix protein. Phospholipase A2 (PPL A2) and cyclin-dependent kinase 1 (cdk1) proteins were tested as controls. PPL A2 from honeybees was used because there is a PPL A2 present in the sea urchin spicule matrix (11). Cdk1 was tested as a control isolated from yeast using the same procedure as the SM50 protein, and because there is no cdk1 in the spicule matrix. This control ensures that the spectroscopic results were not an artifact of the protein preparation. BSA was used as another, non-sea-urchin, non-yeast-prepared control protein.

In Fig. S9 we present Ca and C spectra from all the proteins assayed, confirming that XANES spectroscopy is not simply detecting Ca, but Ca in a cluster of CaCO₃ extending at least to the nearest neighboring O atoms in all samples. Only areas of droplet that exhibited both carbonate crystal field peaks in Ca spectra and carbonate π^∗ peak at 290.3 eV in C spectra were accepted. The latter is a sharp, intense peak distinct from all other peaks in any organic or mineral C-containing species (35). It is impossible that the spectra we interpret as ACC·H₂O are instead single Ca²⁺ ions, each associated with one protein, because these would not show crystal field peaks in Ca spectra, nor a carbonate peak in C spectra, whereas all data presented show both.

The spectra in Fig. 4 show clearly that SM50 stabilizes ACC·H₂O in vitro whereas the other control proteins do not. These findings suggest that SM50 may stabilize ACC·H₂O in sea urchin-mineralized tissues. Because as many as 218 different proteins have been identified in the spicule (11), it is likely that other proteins along with SM50 stabilize ACC·H₂O. SM50 has been found to localize at the outer rim of the spicule (36, 37), where ACC·H₂O stabilization is most important, placing SM50 at the appropriate location in the spicule for it to function as an ACC·H₂O-stabilizing factor. Seto et al. (36), Urry et al. (37), and Killian and Wilt (32) have also detected SM50 occluded at lower density inside the spicule, which is where we observe the magenta nanoparticles. All these observations support the possibility that SM50 stabilizes ACC·H₂O in vivo. SM50 was first cloned 25 years ago (29). However, only in the context of our recent understanding of the dynamics of the mineral phase transformations in sea urchin spicules, and with the advent of powerful spectroscopic and molecular tools, are we now able to decipher SM50’s possible function.

Understanding the specific mechanism by which SM50 may stabilize ACC·H₂O is the next challenge. Acidic proteins have long been suspected to play a major role in carbonate biomineralization, and there is much evidence that such proteins stabilize ACC·H₂O (14, 23, 24, 38). SM50, however, is not an acidic protein (31, 32).

The function of only a few biomineral proteins has been identified thus far. Suzuki et al. (39) isolated a protein called Pif that is essential for mollusk shell nacre formation. Starmaker is a protein expressed in zebrafish, which Nicolson and coworkers (40) have shown to be necessary for aragonite polymorph selection, and morphology in the zebrafish otolith. Notwithstanding this paucity of functional analyses, amorphous mineral phases are widespread in biominerals. Therefore the role of proteins acting as inhibitors of phase transition is probably not restricted to sea urchin spicules. Amorphous mineral phases have been identified in forming biominerals from different phyla: echinoderms (7, 16, 26, 41), mollusks (42⇓–44), crustaceans (38, 45⇓⇓⇓⇓⇓–51), annelids (52⇓–54), porifera (55), urochordates (24, 56), and chordates (57, 58). Therefore, the phase transitions and their regulation by organic molecules observed here may be shared by numerous CaCO₃-mineralizing organisms. Biomineralization is a major mechanism of carbon sequestration and therefore a better understanding of this process is of major biogeochemical, environmental, and economic importance.