Skip to main content

Thank you for visiting 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.

Protein interface redesign facilitates the transformation of nanocage building blocks to 1D and 2D nanomaterials


Although various artificial protein nanoarchitectures have been constructed, controlling the transformation between different protein assemblies has largely been unexplored. Here, we describe an approach to realize the self-assembly transformation of dimeric building blocks by adjusting their geometric arrangement. Thermotoga maritima ferritin (TmFtn) naturally occurs as a dimer; twelve of these dimers interact with each other in a head-to-side manner to generate 24-meric hollow protein nanocage in the presence of Ca2+ or PEG. By tuning two contiguous dimeric proteins to interact in a fully or partially side-by-side fashion through protein interface redesign, we can render the self-assembly transformation of such dimeric building blocks from the protein nanocage to filament, nanorod and nanoribbon in response to multiple external stimuli. We show similar dimeric protein building blocks can generate three kinds of protein materials in a manner that highly resembles natural pentamer building blocks from viral capsids that form different protein assemblies.


Shape transformation phenomena are ubiquitous in nature. Many living organisms by shape transformation perform shape-to-function activities in response to the external environment1. For instance, Amoeba proteus undergoes multidirectional shape transformation to form pseudopod for navigation and rapid path alteration. These phenomena have triggered tremendous interest in mimicking the structure–property relationship of living systems. At a molecular level, shape-shifting related to DNA2, RNA3, peptides4, and small molecules5 has been reported in recent years owing to their relatively simple and controllable structure. In viral capsids, a single protein fold can be evolved to form multiple oligomeric states with different symmetries6, but to construct smart protein architectures artificially whose structure and shape transformation could be modulated by external stimuli remains challenging.

Proteins, as Nature’s most versatile building blocks, are mainly responsible for the complexity of living organisms7. During evolution, proteins have acquired self-assembly properties to construct a variety of large, complex, and symmetric architectures such as one-dimensional (1D) actin filaments8, two-dimensional (2D) bacterial surface layers (S-layers)9, and three-dimensional (3D) light-harvesting protein complexes of phycobilisomes10, thereby endowing their hosts with plenty of functions. It is well known that protein–protein interactions (PPIs) at protein interfaces are the chief contributors to construct the diversified protein nanostructures11,12,13. Following Nature’s inspiration to assemble protein building blocks into exquisite nanostructures, various self-assembly strategies, such as symmetry-directed design14,15,16,17, metal coordination7,18,19,20, host–guest interactions21,22, and the use of bifunctional ligands23,24, have been applied to construct 1D, 2D, and 3D hierarchical protein nanostructures. Among these various protein nanostructures, natural protein nanocages represent a class of versatile nanomaterials that fulfill a wide range of functions, such as CO2 fixation by carboxysomes25, iron metabolism by ferritins26, DNA protection by Dps27, and nucleic acid storage and transport by viral capsids28. By taking advantage of their well-defined architectures, isolated interiors, and high biocompatibility, scientists have subverted the above natural functions of the protein nanocages and explored them as nanocontainers for encapsulation and delivery of bioactive cargo molecules29, as bio-templates for preparation of various nanomaterials30, and as reaction centers for multienzyme catalysis31. So far, different strategies such as de novo design32,33,34, fusion protein14,35,36, directed evolution37,38,39, and key interface redesign40,41 have been built to create a variety of artificial hollow protein nanocages that rival the size, property, and functionality of their natural analogs. Despite these advances, rendering PPIs controllable to facilitate the transformation of the building blocks from protein nanocages into 1D or high-order nanomaterials in the laboratory has yet to be explored.

Herein we introduce a protein interface redesign approach that could be used for the self-assembly transformation of dimeric building blocks from hollow protein nanocage to filament, nanorod, and nanoribbon. The basic building block of this approach is a naturally occurring dimeric protein—Thermotoga maritima ferritin (TmFtn), which tends to assemble into 24-meric hollow protein nanocage induced by calcium ions (Fig. 1a). The crystal structure analyses revealed that the assembly of two adjacent dimeric protein molecules in a head-to-side manner is responsible for the formation of such a shell-like structure (Fig. 1a). In contrast, upon tuning such head-to-side state to a fully side-by-side manner by protein interface redesign, similar dimeric protein molecules self-assemble into filaments or nanorods in the presence of calcium ions or polyethylene glycol (PEG), respectively (Fig. 1b). Differently, when we adjusted the two adjacent dimeric proteins to interact in a partially side-by-side manner by protein interface redesign, the self-assembly of these similar dimeric protein molecules are able to transform from the inherent hollow protein nanocage into nanoribbon in the presence of PEG (Fig. 1c). The dimensions of these filaments, nanorods, and nanoribbons collectively span between nanometer and micrometer scales (50 nm to 4.0 µm). In-depth characterization by X-ray crystallography, transmission electron microscopy (TEM), and atomic force microscopy (AFM) confirmed that this protein interface redesign approach can regulate the transformation between hollow protein nanocage and 1D and 2D nanomaterials. This approach opens up an avenue for constructing 1D or 2D nanoarchitectures with the building blocks of hollow protein nanocage as starting materials.

Fig. 1: Schematic representation of the protein interface redesign approach used to control the self-assembly transformation of dimeric building blocks between different types of nanomaterials.
figure 1

a The naturally occurring dimeric Thermotoga maritima ferritin (TmFtn) molecules interact with each other in a head-to-side manner to form 24-meric protein nanocages in the presence of calcium ions or PEG. b, c Upon Rosetta docking and designing new PPIs between adjacent dimeric building blocks in a fully or partially side-by-side manner, the assembly of similar dimeric building blocks can be transformed from the above formed hollow protein nanocages into nanofilaments or nanorods or nanoribbons in the presence of calcium ions or PEG.


Natural dimeric TmFtn assembly into hollow protein nanocages

The four helix bundle structure, which is widely distributed in Nature, has been utilized as building blocks to construct a number of proteins and enzymes to perform a considerably wide range of functions, such as iron storage by ferritin26, DNA protection by Dps protein27, copper storage by Csp142, electron transfer by cytochrome cb56243, ribonucleotide reduced into deoxynucleotide by R2 subunit of ribonucleotide reductase44, methane oxidized into methanol by methane monooxygenase45, and so on. Four helix bundles are also attractive for synthetic chemists because its interfaces are dominated by side chain and side chain interactions, which can be more tunable than β-strands. This study focuses on TmFtn, a naturally dimeric protein consisting of two antiparallel four helix bundles, as shown in Supplementary Fig. 1. In contrast, most known ferritins are usually composed of 24 identical or similar subunits that assemble into a shell-like structure. Interestingly, the dimeric TmFtn can convert into 24-meric protein nanocage in the presence of divalent metal ions such as Mg(II) and Ca(II)46,47. Consistent with these recent findings, our results show that, in solution, purified TmFtn molecules (Supplementary Fig. 2) exist as dimers and can self-assemble into 24-meric hollow protein nanocage in the presence of Ca2+, and addition of EDTA causes the formed protein nanocage disassembly back into its dimeric form (Supplementary Fig. 3a), indicative of a reversible process of protein assembly (Supplementary Fig. 3b).

The crystal structure of 24-meric Tmftn determined at a resolution of 2.2 Å (Supplementary Tables 1 and 2) shows that one calcium ion located nearby C3C4 interface is coordinated with two acidic residues (Glu51 and Glu132) and three water molecules (Supplementary Fig. 3c, d). Careful analyses of the crystal structure revealed that a group of acidic amino acid residues are lined along with the C3C4 interface, producing electrostatic repulsion along with this interface in the absence of calcium ions. This might be an important reason why TmFtn molecules naturally exist as protein dimers in solution in the absence of metal ions. In contrast, calcium ions near the C3C4 interface can essentially eliminate such electrostatic repulsion through their interaction with the acidic residues, strengthening the stability of C3C4 interface, finally producing the 24-meric protein nanocage. Besides, each protein nanocage is composed of 12 protein dimers, and any of the 2 adjacent protein dimers interact with each other in a head-to-side manner (Supplementary Fig. 3b, d). Based on these findings, it is reasonable to believe that calcium ions facilitate the interaction of these protein dimers in a head-to-side manner, resulting in the formation of hollow protein nanocage.

Engineering dimeric TmFtn for assembly into filaments and nanorods

The above head-to-side interaction manner is ubiquitous in nearly all known ferritins from animal, plant, to bacteria. Based on this interesting phenomenon, we envisioned that if this head-to-side interaction manner between two adjacent dimeric TmFtn was adjusted to a fully side-by-side manner by protein interface redesign, the 24-meric TmFtn nanocages would transform into 1D protein nanomaterials. Therefore, we describe a three-step computational assisted method for realizing this idea: (1) two adjacent dimers were manually placed in a fully side-by-side manner as shown in Supplementary Fig. 4a, (2) RosettaDock algorithm48 was carried out to optimize such fully side-by-side interactions into a more complementary protein–protein interface, and (3) building interactions at the designed interface to drive self-assembly. After completing the first two steps, predicted surface residues include sites 114 and 147 and sites 114’ and 147’ that lie across the designed interface from each other as appropriate locations for installing the interactions (Supplementary Fig. 4b, c). We made a mutant named FLAL where Asn147 was replaced by aromatic phenylalanine (Phe) residue to create ππ interactions, while Glu112, Glu113, and Lys114 were replaced by three hydrophobic residues Leu, Ala, and Leu to decrease the electrostatic repulsion and increase the hydrophobic interactions between two adjacent dimers at the same time (Supplementary Fig. 5). Subsequently, this mutant was purified to homogeneity as characterized by sodium dodecyl sulfate (SDS) and native polyacrylamide gel electrophoresis (PAGE; Supplementary Fig. 6). However, similar to wild-type (wt) TmFtn, the mutant FLAL also occurs as a dimer rather than liner arrangement in solution under different experimental conditions (pH value from 6.0 to 10.0; the concentration of NaCl from 0 to 500 mM; Supplementary Fig. 7). This might be because the designed interaction forces are not strong enough to drive protein dimers assembly in a side-by-side manner in solution. This situation is, at least partly, derived from the fact that a group of acidic amino acid residues from C-helix and D-helix occur between the designed subunits interface (Supplementary Fig. 8), reducing the designed attraction, thereby impeding adjacent FLAL molecule assembly in the designed side-by-side manner.

Inspired by the fact that Ca2+ has the ability to induce natural TmFtn dimer assembly into 24-meric protein nanocage through its interaction with acidic residues (such interaction not only eliminates electrostatic repulsion from acidic residues but also reinforces the attraction between dimeric building blocks; Supplementary Fig. 3c), we deemed that calcium ions might also have the ability to facilitate FLAL molecules to assemble side-by-side because many acidic amino acids are lined along with the designed interface. To confirm this idea, we examined the FLAL self-assembly behavior in solution concerning Ca2+ and FLAL concentrations. Upon screening the concentration of Ca2+ and FLAL (Supplementary Table 3), we found that the optimal condition for the formation of filaments is [FLAL] = 48.0 μM and [Ca2+] = 80.0 mM, which is close to the Ca2+ concentration (50 mM) used for the above nanocage assembly47. TEM under the above conditions showed that FLAL molecules self-assemble into two kinds of protein arrays: cuboid-like superlattices and filaments, as shown in Supplementary Fig. 9a. Since FLAL concentration used here is significantly lower than that needs during conventional crystallization procedures (at least 144.0 μM or 6.0 mg/mL), the formation of these two kinds of protein arrays corresponds to a protein self-assembly process in solution. Enlargement of the small cuboid-like assembly revealed that 12 dimeric FLAL molecules first assemble into 24-meric protein nanocages, which further assemble into well-organized 3D superlattices (Supplementary Fig. 9b–d) as we previously reported16,17. This result is not surprising for two reasons: (a) the above genetic modification for native dimeric TmFtn is only involved in amino acid residues nearby the C3 and C4 interfaces of the metal-mediated 24-meric protein nanocage rather than its C3C4 interfaces, thus hardly affecting its inherent assembly property; (b) substitution of Asn147 with Phe in native TmFtn can also have the possibility to make two adjacent protein nanocages join together along the fourfold channels through ππ interactions as reported recently16, resulting in the formation of such 3D protein superlattices. In contrast, enlargement of the linear-shaped species revealed the generation of filaments by FLAL mutant molecules (Supplementary Fig. 9e). Differently, wt TmFtn dimers can only assemble into discrete protein nanocages under identical experimental conditions (Supplementary Fig. 10). These findings demonstrate that protein interface redesign in conjunction with appropriate solution conditions can realize the self-assembly transformation of dimeric building blocks from protein nanocage into 1D nanomaterials.

To visualize the morphology of the formed filaments in detail, they were observed by TEM in different visual fields. With excess Ca2+ addition, filaments were formed rapidly within 30 min (Fig. 2a). As time goes on, the filaments become longer and more numerous (Fig. 2a–d), suggesting that the filament formation is thought to proceed through growth events. The length of these filaments grew up to tens of nanometers with the most extended filament up to 1.3 µm (Supplementary Fig. 11), and finally the formed filaments were tangled together (Fig. 2d). In addition, the filaments have a tendency to stack together, and thus individual filament is hardly observed. Usually, two or four filaments are stacked together, and these filament assemblies exhibit widths on the order of 7 or 17 nm, respectively, with the pitch of two filaments approximately 3 nm (Fig. 2e, f). The width of the individual filament is about 2 nm, which is in good agreement with the thickness of FLAL dimer (Supplementary Fig. 1).

Fig. 2: Characterization of the filaments constructed by 48.0 µM FLAL and 80 mM Ca2+.
figure 2

ad TEM images of the filaments at different time points (0.5, 1, 12, and 24 h). e High-magnification transmission electron microscopic (HRTEM) images of the filaments. f Real map of the inverted FFT of e.

To obtain detailed structural information on the FLAL filament, we tried to crystallize this protein and eventually obtained qualified single crystals suitable for X-ray diffraction. The crystal structure was solved at a resolution of 2.1 Å (Supplementary Tables 1 and 2). The packing pattern of FLAL molecules in the crystal is pronouncedly different from wt TmFtn. The side view of the crystal structure revealed that FLAL molecules arrange in a repeating, side-by-side fashion to form filaments (Fig. 3a). In contrast, native TmFtn exhibits a different packing pattern in its crystal where 12 TmFtn dimers assemble into a 24-mer protein cage (Supplementary Fig. 3). Such a difference in protein assembly between TmFtn and mutant FLAL agrees with our design. The crystal structure shows that the width of the filament is about 5 nm from the side view and about 2 nm from the top view, these findings being in accordance with the above TEM observation showing that the width of filaments is about 2 nm (Fig. 2).

Fig. 3: Structural basis of the 1D filaments in atomic detail.
figure 3

a Side and top views of the FLAL filament in the crystal structure where the Ca2+ is shown as cyan sphere. be Close-up views of the interfacial interactions between two adjacent dimers in the 1D filament, including ππ stacking interaction (b), hydrophobic interactions (c, d), and metal coordination (e).

Further crystal analyses reveal that two adjacent FLAL molecules have opposite orientations, forming another interface along their C and D helixes. In the structure with resolutions that permit detailed analysis of side-chain configurations, Phe147 and Leu114 side chains at the designed interface adopt suitable conformations to generate ππ stacking interactions and hydrophobic interactions, respectively (Fig. 3b, c), again approving our design at an atomic level. Besides the designed noncovalent interactions, Leu112 and Val119 also produce hydrophobic interactions (Fig. 3d), which is unexpected. Additionally, one calcium ion occurs nearby the designed protein interface, which binds to Glu108, Asp127, Asn105, and one water molecule (Fig. 3e). We believe that the cooperation of these noncovalent interactions and metal coordination along the inter-building-block interfaces promotes the formation of the filaments. It should be noted that only the bounded calcium ion with obvious densities can be identified in the crystal structure, but other interactions with low occupancy were not counted. In the crystal structure, the formed filaments further arrange in the vertical direction to create 2D protein assemblies (Supplementary Fig. 12a). Besides, these filaments are parallel displaced from the side view (Supplementary Fig. 12b), and two adjacent filaments are connected by weak interactions in the crystal structure. For example, Lys10 and Glu164 from two contiguous filaments are in close proximity, leading to the generation of electrostatic attraction (Supplementary Fig. 12c). However, TEM analyses revealed that the M1 mutant where Lys10 and Glu164 were mutated into Gly exhibits a similar assembly behavior to the FLAL molecule (Supplementary Fig. 13), suggesting that other kinds of non-covalent interactions might be also responsible for the formation of the observed 1D filament. The detailed stacking mechanism between adjacent filaments needs further investigation.

One overarching goal of synthetic biomimetic nanomaterials is to construct hierarchical assemblies that are able to respond to various external stimuli so that the fabricated assemblies can be controlled. Therefore, besides calcium ions, we also investigated the effect of PEG on the assembly behavior of FLAL molecules because PEG is a hydrophilic nonionic polymer widely used in many biochemical and pharmaceutical applications due to its mild action on the biological activity of cell components49,50. After trying different molecular weights (PEG1000, PEG1500, and PEG3000) and concentrations (10, 20, and 30%) of PEG, we finally obtained nanorods formed in the presence of 30% PEG1500. As shown in detail in Fig. 4a, nanorods of several micrometers in length (up to 4 μm) can be visualized through TEM. Magnification of the assembled components showed that FLAL molecules are well organized and arranged in a linear manner as shown by the yellow dotted line (Fig. 4b). Fast Fourier transform (FFT) based on the TEM image presents a clear view of the assembled arrangement (Fig. 4c). The corresponding assembly pattern of the FLAL molecules observed under TEM is shown in Fig. 4d. Further analysis by AFM with an intelligent mode revealed that the height of the nanorod is 220 ± 5 nm (Supplementary Fig. 14). In contrast, wt TmFtn dimers only assemble into discrete protein nanocages under identical experimental conditions (Supplementary Fig. 15). These results again demonstrate that the designed driving force enables dimeric FLAL molecules to self-assemble into nanorods.

Fig. 4: TEM analyses of the nanorods constructed by 12.0 µM FLAL and 30% PEG1500.
figure 4

a Low-magnification TEM view of the formed nanorods. b High-magnification view of a. The yellow dotted line indicated the assembled direction of FLAL molecules. c Real map of the inverted FFT from b. Inset: Fast Fourier transform image. d Structural diagram based on the reconstruction of c.

To determine the structural basis of such nanorods, we set out to grow single crystals large enough for X-ray diffraction analyses in the presence of PEG1500. We solved the crystal structure at 2.6 Å resolution (Supplementary Tables 1 and 2). As expected, the designed interface is responsible for driving self-assembly, but no electron densities of the PEG were observed (Supplementary Fig. 16), most likely due to the high flexibility of PEG and its weak ability to bind to protein50. The crystal structure proved remarkably similar to the design model: protein molecules connect through designed π stacking and hydrophobic interactions in a side-by-side repeating pattern with adjacent FLAL molecules antiparallel with each other (Supplementary Fig. 16a, e). Thus, the crystal structure is in good agreement with the above results observed by TEM (Fig. 4b, c), confirming the side-by-side interaction manner of dimeric FLAL molecules.

Further analyses of the crystal structure showed that the assembly process of FLAL molecules could be summarized as follows: first, FLAL molecules pack along the x-axis in such a way mentioned above to form 1D arrays (Supplementary Fig. 16a), and such assembly pattern was also observed by TEM shown in Fig. 4b; second, just like the stacking of filaments of FLAL molecules in the presence of Ca2+, these 1D arrays stack along the y-axis through electrostatic interaction to form 2D arrays (Supplementary Fig. 16b), which is likewise visualized by TEM (Fig. 4b, c); finally, the formed 2D arrays further arrange in the vertical direction to create 3D protein assemblies (Supplementary Fig. 16c, d), and the weak interaction involved in this step mainly comes from their E helix (Supplementary Fig. 16f). Taken together, all these findings demonstrate that our protein interface redesign approach yields assembly of dimeric FLAL protein building blocks into the filaments or nanorods induced by Ca2+ or PEG rather than the inherent Ca2+-mediated 24-meric protein shell-like assembly.

Engineering dimeric TmFtn for assembly into nanoribbons

The above results demonstrated that tuning the action mode of two adjacent protein dimers from the head-to-side manner to the fully side-by-side manner facilitates the self-assembly transformation of the dimeric building blocks from hollow protein nanocage into nanofilaments and nanorods. Bioinspired by the structure of α-keratin protofilaments formed from two staggered rows of head-to-tail coiled coils51, we wonder what if we rearrange two adjacent protein dimers in a staggered pattern, namely, a partially side-by-side pattern. To answer this question, we use the method mentioned above for protein docking but do not need to preset the dimers to search for their possible arrangement. To this end, we simulated the orientations of two TmFtn dimers through global docking using RosettaDock48. One thousand independent docking trajectories were carried out, and by combining energy simulation with a visual inspection, a model with dimers in a partially side-by-side manner was selected to assist interface redesign (Supplementary Fig. 17a). We found that several hydrophobic residues, including Leu107, Val119, Val126, and Val130, are distributed along with the designed interface (Supplementary Fig. 17b). To effectively utilize these hydrophobic residues, we plan to design hydrophobic interactions as the driving forces to construct such partially side-by-side protein assembly. Based on the fact that FLAL mutant contains three more hydrophobic amino acid residues located on its outer surface than wt TmFtn, therefore, to build stronger hydrophobic interactions at this designed interface (Supplementary Fig. 17c), we chose FLAL mutant instead of wt TmFtn as starting materials for further engineering.

To enable two dimers to interact with each other in a partially side-by-side fashion, we made another mutant named FLAL-L where Arg137 in FLAL was replaced with Leu (Supplementary Fig. 5) to increase the area of the hydrophobic patch as shown in Supplementary Fig. 17d. To gain insight into the assembly behavior of FLAL-L mutant, we purified it to homogeneity as suggested by SDS-PAGE and native-PAGE (Supplementary Fig. 18). We next investigated the assembly of FLAL-L molecules in the presence of PEG in solution. Upon screening the concentration and molecular weight of PEG, we found that FLAL-L molecules can likewise assemble into filaments in the presence of 15 or 20% PEG1500, as shown in Supplementary Table 4. The filaments with different sizes ranging from 100 nm to several micrometers can be visualized (Fig. 5a, b). Enlargement of the assembly revealed that the FLAL-L molecules are well organized in a linear fashion (Fig. 5b). To obtain more insights into the structural information, the formed filaments were further characterized by AFM with an intelligent mode. As shown in Fig. 5c, d, the height of the array is 6 ± 0.5 nm, which is comparable with the height of FLAL-L molecules (5 nm) in the crystal (Supplementary Fig. 1). To gain deep insight into the above process, we investigated the formation of the filaments as a function of time. Short filaments were rapidly formed at 5 min. With an increase in time, the length and number of the formed filaments increased gradually (Fig. 6a–e). After 15 days, except for the filament, nanoribbon-like nanomaterials appeared (Fig. 6f). A high-magnification TEM view (Fig. 6g) seized the periodic parallel arrangement of protein arrays, and the real map from invert FFT (Fig. 6h) gave an excellent view on the structure of the nanoribbon, which reveals that two kinds of lines interlaced to form such structure (Fig. 6i). Further examination of the nanoribbons using AFM revealed that the height of the nanoribbon is nearly 10 nm (Supplementary Fig. 19).

Fig. 5: Characterization of the 1D filaments constructed by 12.0 µM FLAL-L and 15% PEG1500.
figure 5

a Low-magnification TEM view of FLAL-L filaments. b Enlargement of FLAL-L filaments. c Atomic force microscopic (AFM) micrographs of the 1D filaments. d Height distributions measured along the black arrow in c.

Fig. 6: Kinetics of the formation of 2D nanoribbon.
figure 6

af TEM views of the formation of FLAL-L assemblies as a function of time (5 min, 30 min, 1 h, 12 h, 24 h, and 15 days, respectively) in the presence of 15% PEG1500. g High-magnification view of the 2D nanoribbon formed at 15 days. h Fast Fourier transform (FFT) of g. i Real map from invert FFT of h. The black and red dotted lines indicate the arrangement of the 2D FLAL-L assembly. ae Scale bars represent 500 nm, while scale bars represent 2 µm in f, and 100 nm in g, i, respectively.

To shed light on structural information on the above filaments and nanoribbons, FLAL-L was also crystallized by vapor diffusion, and eventually, qualified single crystals suitable for X-ray diffraction were obtained (Supplementary Fig. 20a). We solved the crystal structure at the resolution of 2.3 Å (Supplementary Tables 1 and 2). The crystal structure analyses revealed that FLAL-L molecules are perfectly aligned with each other in a partially side-by-side manner to form filaments (Fig. 7a), the top view of which is in good agreement with the filament observed under TEM (Fig. 5a, b). As expected, intermolecular associations between two adjacent FLAL-L molecules are mediated entirely through hydrophobic interactions, as the contact region of adjacent FLAL-L molecules is rich in hydrophobic amino acid residues (Fig. 7b). The engineered Leu114 and Leu137 side chains cooperated with the original V119, L107, V126, and V130 side chains provide the bulk of the hydrophobic core, whereas the engineered Leu112, Ala113, and Phe147 are not involved in such interactions. The crystal structure provides direct evidence to confirm the partially side-by-side manner of FLAL-L molecules. The above formed filaments coalesce in parallel along the y axes through hydrogen bonds (Supplementary Fig. 20b, c), leading to the generation of a protein layer (Fig. 7c), corresponding to the ribbons observed by TEM (Fig. 6). The arrangement of the protein layer in the crystal perfectly matches the pattern seen in the nanoribbons observed by TEM (Fig. 6f–i). Based on the observation that the thickness of each protein layer is about 2 nm as suggested by the crystal structure (Fig. 7c) and the height of the nanoribbons detected by AFM (Supplementary Fig. 19) is around ~10 nm, it is reasonable to believe that the observed nanoribbons are of five layers. In crystals, the formed protein layers further arrange along the z axes to form 3D protein frameworks (Fig. 7d) through ππ interactions and electrostatic interactions (Supplementary Fig. 20d–f). All these results demonstrate that the hydrophobic interactions between two contiguous dimeric protein-building blocks in a partially side-by-side fashion carried out by protein interface redesign facilitate the transformation of the dimeric building blocks from 24-meric nanocages into nanoribbons through filaments.

Fig. 7: The crystal structure and arrangement of FLAL-L mutant.
figure 7

a Side and top views of the 1D FLAL-L filament in the crystal structure. b Close-up view of the hydrophobic interactions between two adjacent FLAL-L molecules. c The 1D filaments coalesce in parallel along the y axes to form 2D protein layer, corresponding to the 2D ribbons observed by TEM. The dashed lines in c correspond to the lines shown in Fig. 6i. d From the top view, FLAL-L molecules assemble into 3D protein frameworks.


Particle polymorphism is a popular phenomenon in virus capsids, which possess inherent switches that allow efficient disassembly and reassembly in response to solution conditions. For example, an icosahedral plant virus, cowpea chlorotic mottle virus, can convert into a tubular nanostructure, which needs double-stranded DNA to act as a template and take advantage of the nonspecific binding of capsid proteins and DNA52,53. Simian virus 40 (SV40) represents another interesting example of shape transformation between protein nanostructures with different dimensions. The SV40 capsid is mainly composed of 72 pentamers of VP1. Electron microscopic observations revealed that, at pH 5.0, long and tubular structures are formed, whereas at high salt concentrations, small (20 nm) particles predominate54. However, how to transform the assembly of the building blocks from natural protein cages into 1D or 2D architecture by a simple, effective method in the laboratory has yet to be explored. The challenge lies in the fact that protein nanocages occurs as discrete molecules in solution while filament/nanorod/ribbon created in this study closely resemble 1D and 2D polymers and that the intermolecular interface and assembly geometry for the construction of hollow protein nanocage and filament/nanorod/ribbon nanomaterials are entirely different. We demonstrate that spatially directed assembly of protein-building blocks might be a solution to solve such problems, which will reduce the computational workload and lower the barriers to protein assembly design. To confirm this idea, we have built here a protein interface redesign approach that is able to manipulate the directed assembly of protein-building blocks, resulting in the self-assembly transformation of dimeric building blocks from hollow protein nanocage to 1D and 2D protein arrays with nanoscale and microscale long-range order.

In pursuit of our goal to transform the dimeric building blocks from hollow protein nanocages into 1D and 2D nanostructure, external stimuli were introduced to exert control over PPIs for dimeric FLAL or FLAL-L assembly. Researchers have demonstrated that the self-assembly of a monomeric four helix bundle protein can be directed in all three dimensions through the inherent chemically tunable and modular nature of metal coordination7. In this study, the transformation of dimeric building blocks into different protein nanomaterials including hollow protein nanocage and filament/nanorod/nanoribbon mainly depends on the redesigned PPIs. These PPIs are largely mediated by the designed weak, noncovalent interactions, although external stimulation is required to trigger the assembly of the designed protein dimers.

It is noteworthy that there is only one amino acid difference in amino acid sequence between FLAL and FLAL-L molecules, but their assembly behavior is markedly different from each other. FLAL molecules self-assemble into nanorods, whereas FLAL-L has the ability to assemble into the nanoribbons. The significant difference in self-assembly behavior between these two dimeric protein molecules reflects the importance of amino acid residue Arg137 in FLAL, suggesting that Arg137 could act as a switch to control the conversion of nanorods to nanoribbons. In all cases, the crystal structures reveal that the backbones in the side-by-side interaction manner were designed with high accuracy compared to the computationally designed model (Supplementary Fig. 21). The occurrence of 1D and 2D protein arrays with the dimeric protein as building blocks recalls among natural proteins the case of actin filaments and S-layers in terms of their dimensions and structural uniformity. Thus, our reported construction of 1D and 2D protein arrays from the dimeric protein as building blocks provides a model to study the assembly mechanism of natural protein architectures.

Controlling self-assembly is critical to the advancement of nanotechnology. Nowadays, scientists are able to accurately control the protein self-assembly behaviors to construct various supramolecular structures through the rational design of PPIs. Though a variety of intricate protein nanostructures such as hollow protein cages, filaments/tubules, nanosheets, and 3D crystalline frameworks have been created18,19,20,21,22,23,24,36,37,38,39,40,41, rendering directed assembly of protein-building blocks into the custom-tailored nanoarchitectures remains challenging. Our reported protein engineering approach could tune the inherent head-to-side interaction manner of two adjacent dimeric protein-building blocks to the fully or partially side-by-side manner by redesigning protein interfaces, yielding directed assembly of the building blocks, thereby facilitating the self-assembly transformation of the dimeric building blocks from hollow protein nanocage into 1D or 2D nanomaterials. PPIs at the designed protein interfaces are mainly contributed from the cooperation of the hydrophobic interactions, aromatic ππ interactions, and external stimulation, which effectively stabilize the designed protein interface. The above protein engineering approach that focuses on adjustment for the geometric arrangement of protein-building blocks is conceptually and operationally simple. It is interesting that the head-to-side interaction between two contiguous dimeric protein-building blocks occurs not only in all known ferritins but also in other cage-like proteins such as Dps, where six dimeric protein-building blocks also assemble into a shell-like structure27. Therefore, our engineering approach should, in principle, be applicable to some other protein architectures. This would produce a variety of protein nanomaterials with different geometries. Furthermore, the filaments obtained in this study could provide a multiple enzyme port scaffold to convene variant enzymes align into a supramolecular enzyme system with unexplored property55.


Protein preparation

The gene encoding TmFtn was synthesized by Synbio Technologies, which has been inserted into the plasmid pET-3a. Mutagenesis of the TmFtn cDNA was performed with the fast site-directed mutagenesis kit (TIANGEN Biotech Co., Ltd.). Polymerase chain reaction amplification was carried out using the pET-3a plasmid with the TmFtn gene as a template, and primers for mutagenesis are listed in Supplementary Table 5. Plasmid sequences were verified by DNA sequencing. TmFtn, as well as mutants, were purified as follows. First, the plasmids corresponding to FLAL and FLAL-L were transformed into BL21 (DE3) Escherichia coli cells, respectively, and then cultured at 37 °C in 1 L of LB media containing 100 µg/mL ampicillin. After the cell density reached an absorbance of 0.6 at 600 nm, protein expression was likewise induced with 200 µM IPTG for 10 h at 37 °C. Cells were harvested by centrifugation (8609 × g) and the precipitate was re-suspended in 50 mM Tris–HCl (pH 8.0), followed by sonication. The supernatant was collected from lysed cell samples and subjected to heating at 90 °C for 10 min. Then thermal-treated supernatant was collected after centrifugation at 8609 × g for 30 min and passed through a membrane filter. Finally, the protein solution was applied to an ion-exchange column (DEAE Sepharose Fast Flow, GE Healthcare), followed by gradient elution with 0–1.0 M NaCl. The purified protein was then dialyzed against 50 mM Tris–HCl (pH 8.0) at 4 °C to exclude NaCl from the solution, and protein concentrations were determined according to the Lowry method with bovine serum albumin as standard. Protein purity was confirmed by SDS–PAGE. The molecular weight of TmFtn subunit was estimated to be approximately 20 kDa, which is consistent with our electrophoretic band as shown in Supplementary Fig. 2b, and the molecular weight of the dimer is approximately 40 kDa.

Preparation of nanocages, filaments, nanorods, and nanoribbons

After purification, TmFtn molecules remain as a dimer in the absence of metal ions. For protein nanocages, 50 mM Tris–HCl (pH 8.0) was used as buffer and 50 mM CaCl2 was required to induce dimeric TmFtn self-assembly. Filaments were prepared by adding a certain amount of CaCl2 to FLAL solution (48 µM) at room temperature. After being stirred for several minutes, the resulting mixture was incubated at 4 °C overnight. To optimize the assembly conditions, different concentrations of CaCl2 were tested over a range of 0–100 mM. Similarly, nanorods were prepared by adding a certain amount of PEG1500 to FLAL solution (12 µM) at room temperature. After gently shaking for a few minutes, the resulting mixture was incubated at 4 °C overnight. Nanoribbons were prepared by mixing FLAL-L solution (12 µM) with 30% PEG1500, and then the reaction mixtures were incubated for 15 days. The concentrations and polymerization degree of PEG used were optimized.

Docking simulations

One thousand independent docking trajectories were carried out using RosettaDock48. The two TmFtn or FLAL subunits that form the designed interface were used as the starting structure for the docking simulations. One of the monomers was randomly spun along the axis connecting the centers of mass of both partners and the same monomer was also allowed to search a space of up to 3 Å normal to that axis, 8 Å in the plane perpendicular to the axis, and with up to an 8˚ tilt from the axis and an 8˚ additional spin around the axis.

Polyacrylamide gel electrophoresis

The purity and molecular weight of protein samples were estimated by PAGE. Gel electrophoresis under denaturing conditions was carried out using a 15% polyacrylamide–SDS gel as reported by Laemmli56, and samples need to be heated in a water bath for 5 min. For native PAGE, a 4–20% polyacrylamide gradient gel was used and run at 5 mA for 10 h at 4 °C. Gels were stained with Coomassie brilliant blue R250.

High-resolution gel filtration chromatography analyses

High-resolution gel filtration chromatography analyses were performed using an ÄKTA pure system coupled to a Superdex 200 Increase column (GE Healthcare) in buffer (50 mM Tris, 100 mM NaCl, pH = 8.0) with a flow rate of 0.5 mL/min.

TEM imaging

Protein samples (10 μL) were deposited on carbon-coated copper grids and excess solution was removed with filter paper after a 2-min incubation. Then protein samples were stained using 2% uranyl acetate for 5 min. Transmission electron micrographs were obtained at 80 kV through a Hitachi H-7650 transmission electron microscope.

AFM measurements

For AFM sample preparation, protein samples (10 μL) were pipetted on freshly cleaved mica (Beijing Zhongxingbairui Technology Co., Ltd.) and dried at room temperature. The AFM images were collected using a Nanoman VS (Bruker) with tapping mode at a resolution of 256 lines per image and a scan rate of 1 Hz. The AFM images were processed using NanoScope Analysis.

Crystallization, data collection, and structure determination

Purified proteins were concentrated to 6 mg/mL in a buffer consisting of 20 mM Tris–HCl at pH 8.0, and crystals were obtained using the hanging drop vapor diffusion method under different conditions, which are shown in Supplementary Table 1. X-ray diffraction data were collected at Shanghai Synchrotron Radiation Facility (SSRF; BL17U and BL19U) with merging and scaling by the HKL-3000 software57. Data processing statistics are shown in Supplementary Table 2. The structures were determined by molecular replacement using the Molrep program in CCP4 using the structure of TmFtn (PDB code 1VLG) as a search model. Structure refinement was conducted using the Refmac5 program and PHENIX software58. The structure was rebuilt using COOT59, which made the model manually adjusted. All figures of the resulting structures were produced using the PyMOL60 program and UCSF61 Chimera package.

Data availability

The atomic coordinates and structure factors in this study have been deposited in the Protein Data Bank under the accession PDB IDs: 7DYA, 7DY8, 7DY9, and 7DYB. Source data are provided with this paper.


  1. 1.

    Lay, C. L., Lee, M. R., Lee, H. K., Phang, I. Y. & Ling, X. Y. Transformative two-dimensional array configurations by geometrical shape-shifting protein microstructures. ACS Nano 10, 9708–9717 (2015).

    Article  CAS  Google Scholar 

  2. 2.

    Rothemund, Paul & Folding, W. K. DNA to create nanoscale shapes and patterns. Nature 440, 297–302 (2006).

    ADS  CAS  PubMed  Article  Google Scholar 

  3. 3.

    Delebecque, C. J., Lindner, A. B., Silver, P. A. & Aldaye, F. A. Organization of intracellular reactions with rationally designed RNA assemblies. Science 333, 470–474 (2011).

    ADS  CAS  PubMed  Article  Google Scholar 

  4. 4.

    Aggeli, A. et al. Responsive gels formed by the spontaneous self-assembly of peptides into polymeric β-sheet tapes. Nature 386, 259–262 (1997).

    ADS  CAS  PubMed  Article  Google Scholar 

  5. 5.

    Waller, P. J. et al. Chemical conversion of linkages in covalent organic frameworks. J. Am. Chem. Soc. 48, 15519–15522 (2016).

    Article  CAS  Google Scholar 

  6. 6.

    Zhao, X., Fox, J. M., Olson, N. H., Baker, T. S. & Young, M. J. In vitro assembly of cowpea chlorotic mottle virus from coat protein expressed in Escherichia coli and in vitro-transcribed viral cDNA. Virology 207, 486–494 (1995).

    CAS  PubMed  Article  Google Scholar 

  7. 7.

    Brodin, J. D. et al. Metal-directed, chemically tunable assembly of one-, two- and three-dimensional crystalline protein arrays. Nat. Chem. 4, 375–382 (2012).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  8. 8.

    Reisler, E. & Egelman, E. H. Actin structure and function: what we still do not understand. J. Biol. Chem. 282, 36133–36137 (2007).

    CAS  PubMed  Article  Google Scholar 

  9. 9.

    Chung, S., Shin, S. H., Bertozzi, C. R. & De Yoreo, J. J. Self-catalyzed growth of S layers via an amorphous-to-crystalline transition limited by folding kinetics. Proc. Natl Acad. Sci. USA 107, 16536–16541 (2010).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  10. 10.

    Ma, J. et al. Structural basis of energy transfer in Porphyridium purpureum phycobilisome. Nature 579, 146–151 (2020).

    ADS  CAS  PubMed  Article  Google Scholar 

  11. 11.

    Kortemme, T. & Baker, D. Computational design of protein-protein interactions. Curr. Opin. Chem. Biol. 8, 91–97 (2004).

    CAS  PubMed  Article  Google Scholar 

  12. 12.

    Schreiber, G. & Fleishman, S. J. Computational design of protein–protein interactions. Curr. Opin. Chem. Biol. 23, 903–910 (2013).

    CAS  Google Scholar 

  13. 13.

    Jones, S. & Thornton, J. M. Principles of protein-protein interactions. Proc. Natl Acad. Sci. USA 93, 13–20 (1996).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  14. 14.

    Padilla, J. E., Colovos, C. & Yeates, T. O. Nanohedra: using symmetry to design self assembling protein cages, layers, crystals, and filaments. Proc. Natl Acad. Sci. USA 98, 2217–2221 (2001).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  15. 15.

    Sinclair, J. C., Davies, K. M., Venien-Bryan, C. & Noble, M. E. Generation of protein lattices by fusing proteins with matching rotational symmetry. Nat. Nanotechnol. 6, 558–562 (2011).

    ADS  CAS  PubMed  Article  Google Scholar 

  16. 16.

    Zhou, K. et al. On-axis alignment of protein nanocage assemblies from 2D to 3D through the aromatic stacking interactions of amino acid residues. ACS Nano 12, 11323–11332 (2018).

    CAS  PubMed  Article  Google Scholar 

  17. 17.

    Zheng, B., Zhou, K., Zhang, T., Lv, C. & Zhao, G. Designed two- and three-dimensional protein nanocage networks driven by hydrophobic interactions contributed by amyloidogenic motifs. Nano Lett. 19, 4023–4028 (2019).

    ADS  CAS  PubMed  Article  Google Scholar 

  18. 18.

    Bailey, J. B., Zhang, L., Chiong, J. A., Ahn, S. & Tezcan, F. A. Synthetic modularity of protein-metal-organic frameworks. J. Am. Chem. Soc. 139, 8160–8166 (2017).

    CAS  PubMed  Article  Google Scholar 

  19. 19.

    Gu, C. et al. Structural insight into binary protein metal-organic frameworks with ferritin nanocages as linkers and nickel clusters as nodes. Chem. Eur. J. 26, 3016–3021 (2020).

    CAS  PubMed  Article  Google Scholar 

  20. 20.

    Yang, M. & Song, W. J. Diverse protein assembly driven by metal and chelating amino acids with selectivity and tunability. Nat. Commun. 10, 5545 (2019).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  21. 21.

    Kitagishi, H. et al. Supramolecular hemoprotein linear assembly by successive interprotein heme-heme pocket interactions. J. Am. Chem. Soc. 129, 10326–10327 (2007).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  22. 22.

    Carlson, J. C. T. et al. Chemically controlled self-assembly of protein nanorings. J. Am. Chem. Soc. 128, 7630–7638 (2006).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  23. 23.

    Yang, R. et al. 2D square arrays of protein nanocages through channel-directed electrostatic interactions with poly(α, L-lysine). Chem. Commun. 50, 2879–2882 (2014).

    CAS  Article  Google Scholar 

  24. 24.

    Yang, G. et al. Highly ordered self-assembly of native proteins into 1D, 2D, and 3D structures modulated by the tether length of assembly-inducing ligands. Angew. Chem. Int. Ed. 56, 10691–10695 (2017).

    CAS  Article  Google Scholar 

  25. 25.

    Tanaka, S. et al. Atomic-level models of the bacterial carboxysome shell. Science 319, 1083–1086 (2008).

    ADS  CAS  PubMed  Article  PubMed Central  Google Scholar 

  26. 26.

    Arosio, P., Ingrassia, R. & Cavadini, P. Ferritins: a family of molecules for iron storage, antioxidation and more. Biochim. Biophys. Acta 1790, 589–599 (2009).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  27. 27.

    Grant, R., Filman, D., Finkel, S., Kolter, R. & Hogle, J. The crystal structure of Dps, a ferritin homolog that binds and protects DNA. Nat. Struct. Biol. 5, 294–303 (1998).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  28. 28.

    Douglas, T. & Young, M. Viruses: making friends with old foes. Science 312, 873–875 (2006).

    ADS  CAS  PubMed  Article  PubMed Central  Google Scholar 

  29. 29.

    Liang, M. et al. H-ferritin-nanocaged doxorubicin nanoparticles specifically target and kill tumors with a single-dose injection. Proc. Natl Acad. Sci. USA 111, 14900–14905 (2014).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  30. 30.

    Wen, A. M. & Steinmetz, N. F. Design of virus-based nanomaterials for medicine, biotechnology, and energy. Chem. Soc. Rev. 45, 4074–4126 (2016).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  31. 31.

    Jordan, P. C. et al. Self-assembling biomolecular catalysts for hydrogen production. Nat. Chem. 8, 179–185 (2016).

    CAS  PubMed  Article  Google Scholar 

  32. 32.

    King, N. P. et al. Computational design of self-assembling protein nanomaterials with atomic level accuracy. Science 336, 1171–1174 (2012).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  33. 33.

    King, N. P. et al. Accurate design of co-assembling multi-component protein nanomaterials. Nature 510, 103–108 (2014).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  34. 34.

    Hsia, Y. et al. Design of a hyperstable 60-subunit protein icosahedron. Nature 535, 136–139 (2016).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  35. 35.

    Lai, Y. T. et al. Structure of a designed protein nanocage that self-assembles into a highly porous cube. Nat. Chem. 6, 1065–1071 (2014).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  36. 36.

    Cannon, K. A., Nguyen, V. N., Morgan, C. & Yeates, T. O. Design and characterization of an icosahedral protein nanocage formed by a double-fusion protein containing three distinct symmetry elements. ACS Synth. Biol. 9, 517–524 (2020).

    CAS  PubMed  Article  Google Scholar 

  37. 37.

    Woersdoerfer, B., Woycechowsky, K. J. & Hilvert, D. Directed evolution of a protein container. Science 331, 589–592 (2011).

    ADS  CAS  Article  Google Scholar 

  38. 38.

    Worsdorfer, B., Pianowski, Z. & Hilvert, D. Efficient in vitro encapsulation of protein cargo by an engineered protein container. J. Am. Chem. Soc. 134, 909–911 (2012).

    CAS  PubMed  Article  Google Scholar 

  39. 39.

    Butterfield, G. L. et al. Evolution of a designed protein assembly encapsulating its own RNA genome. Nature 552, 415–420 (2017).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  40. 40.

    Zhang, S. et al. “Silent” amino acid residues at key subunit interfaces regulate the geometry of protein nanocages. ACS Nano 10, 10382–10388 (2016).

    CAS  PubMed  Article  Google Scholar 

  41. 41.

    Zhang, S. et al. Conversion of the native 24-mer ferritin nanocage into its non-native 16-mer analogue by insertion of extra amino acid residues. Angew. Chem. Int. Ed. 55, 16064–16070 (2016).

    CAS  Article  Google Scholar 

  42. 42.

    Vita, N. et al. A four-helix bundle stores copper for methane oxidation. Nature 525, 140–143 (2015).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  43. 43.

    Wittung-Stafshede, P., Lee, J. C., Winkler, J. R. & Gray, H. B. Cytochrome b562 folding triggered by electron transfer: approaching the speed limit for formation of a four-helix-bundle protein. Proc. Natl Acad. Sci. USA 96, 6587–6590 (1999).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  44. 44.

    Kolberg, M., Strand, K. R., Graff, P. & Andersson, K. K. Structure, function, and mechanism of ribonucleotide reductases. Biochim. Biophys. Acta 1699, 1–34 (2004).

    CAS  PubMed  Article  Google Scholar 

  45. 45.

    Lee, S. J., Mccormick, M. S., Lippard, S. J. & Cho, U. Control of substrate access to the active site in methane monooxygenase. Nature 494, 380–384 (2013).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  46. 46.

    Ceci, P., Forte, E., Di Cecca, G., Fornara, M. & Chiancone, E. The characterization of Thermotoga maritima ferritin reveals an unusual subunit dissociation behavior and efficient DNA protection from iron-mediated oxidative stress. Extremophiles 15, 431–439 (2011).

    CAS  PubMed  Article  Google Scholar 

  47. 47.

    Chakraborti, S. et al. Three-dimensional protein cage array capable of active enzyme capture and artificial chaperone activity. Nano Lett. 19, 3918–3924 (2019).

    ADS  CAS  PubMed  Article  Google Scholar 

  48. 48.

    Gray, J. J. et al. Protein-protein docking with simultaneous optimization of rigid-body displacement and side-chain conformations. J. Mol. Biol. 331, 281–299 (2003).

    CAS  PubMed  Article  Google Scholar 

  49. 49.

    Wang, Y. & Annunziata, O. Comparison between protein-polyethylene glycol (PEG) interactions and the effect of peg on protein-protein interactions using the liquid-liquid phase transition. J. Phys. Chem. B. 111, 1222–1230 (2007).

    CAS  PubMed  Article  Google Scholar 

  50. 50.

    Cattani, G., Vogeley, L. & Crowley, P. B. Structure of a pegylated protein reveals a highly porous double-helical assembly. Nat. Chem. 7, 823–828 (2015).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  51. 51.

    Mckittrick, J. et al. The structure, functions, and mechanical properties of keratin. JOM 64, 449–468 (2012).

    Article  Google Scholar 

  52. 52.

    Mukherjee, S., Pfeifer, C. M., Johnson, J. M., Liu, J. & Zlotnick, A. Redirecting the coat protein of a spherical virus to assemble into tubular nanostructures. J. Am. Chem. Soc. 128, 2538–2539 (2006).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  53. 53.

    Xu, Y. et al. DNA-templated CMV viral capsid proteins assembly into nanotubes. Chem. Commun. 49–51 (2008).

  54. 54.

    Kanesashi, S. et al. Simian virus 40 vp1 capsid protein forms polymorphic assemblies in vitro. J. Gen. Virol. 84, 1899–1905 (2003).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  55. 55.

    Hudalla, G. A. et al. Gradated assembly of multiple proteins into supramolecular nanomaterials. Nat. Mater. 13, 829–836 (2014).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  56. 56.

    Laemmli, V. K. Determination of protein molecular weight in polyacrylamide gels. Nature 227, 680–685 (1970).

    ADS  CAS  Article  Google Scholar 

  57. 57.

    Otwinowski, Z. & Minor, W. Processing of X-ray diffraction data collected in oscillation mode. Methods Enzymol. 276, 307 (1997).

    CAS  PubMed  Article  Google Scholar 

  58. 58.

    Adams, P. D. et al. PHENIX: a comprehensive Python-based system for macromolecular structure solution. Acta Crystallogr. D Biol. Crystallogr. 66, 213–221 (2010).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  59. 59.

    Emsley, P., Lohkamp, B., Scott, W. G. & Cowtan, K. Features and development of Coot. Acta Crystallogr. D Biol. Crystallogr. 66, 486–501 (2010).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  60. 60.

    DeLano, W. L. The PyMOL Molecular Graphics System (DeLano Scientific, 2002).

  61. 61.

    Pettersen, E. F. et al. A visualization system for exploratory research and analysis. J. Comput. Chem. 25, 1605–1612 (2004).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

Download references


This work was supported by the National Natural Science Foundation of China (Nos. 31972018 and 31730069). The Shanghai Synchrotron Radiation Facility (SSRF) is especially acknowledged for beam time. We thank the staff from BL17U1/BL18U1/19U1 beamline of the National Center for Protein Sciences Shanghai (NCPSS) at Shanghai Synchrotron Radiation Facility for assistance during data collection.

Author information




G.Z. and T.Z. conceived and directed the project and wrote the paper. X.Z. designed and performed experiments, analyzed data, and co-wrote the paper. B.Z. performed experiments. Y.L. and H.W performed the crystal data collection. J.Z. and C.L. performed the experiments and co-wrote the paper.

Corresponding authors

Correspondence to Tuo Zhang or Guanghua Zhao.

Ethics declarations

Competing interests

The authors declare no competing interests.

Additional information

Peer review information Nature Communications thanks the 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.

Supplementary information

Source data

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Zhang, X., Liu, Y., Zheng, B. et al. Protein interface redesign facilitates the transformation of nanocage building blocks to 1D and 2D nanomaterials. Nat Commun 12, 4849 (2021).

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI:


By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.


Quick links

Nature Briefing

Sign up for the Nature Briefing newsletter — what matters in science, free to your inbox daily.

Get the most important science stories of the day, free in your inbox. Sign up for Nature Briefing