Hybrid human–chicken embryos illuminate key developmental milestone
A new technique reveals the earliest stages of human development without the need for human embryos.

Before a cluster of cells can develop into an embryo, it must first decide which end is up. But that process had never been observed in humans — until now.

For the first time, researchers have watched human ‘organizer’ cells direct the formation of an embryo’s top, bottom, front and back. They did so by developing a technique that sidesteps restrictions on research with human embryos by grafting human cells onto chicken embryos. The method, published on 23 May in Nature1, could supplant the use of human embryos in some laboratory experiments.

Organizer cells were discovered in 1924, during a series of experiments in Germany on salamanders2. A pair of developmental biologists transplanted cells from the back of one salamander embryo onto the front of another, where the cells grew into a second, conjoined salamander. This suggested that certain cells on an embryo’s back could organize their neighbours into the complex array of structures that make up an animal.

Since then, researchers have identified organizer cells in the embryos of many other species. But scientists had never observed such cells guiding early human development. Ethical guidelines and laws in many countries — including the United States — prohibit scientists from experimenting with human embryos more than 14 days old, which is about the time when organizer cells would be likely to appear.

“No one knew what happens after the ball of cells attaches itself to the uterus,” says Ali Brivanlou, a developmental biologist at the Rockefeller University in New York City and lead author of the latest study.


In 2016, Brivanlou’s group was the first to grow human embryos in a dish to the 14-day mark3. But the researchers halted the work before the point at which embryos begin a complex reorganization that leads to the growth of limbs and organs. They did not see organizer cells in the human embryos before the experiment ended.

In the latest study, the team bypassed the 14-day rule by growing embryo-like structures from human embryonic stem cells. By culturing the cells on small squares just 22 millimetres across, the scientists forced the cells to organize into structures instead of spreading horizontally. They also treated the cells with a series of growth factors that stimulated them to form the various cell layers seen in early embryos. Tests revealed that the embryo-like structures included a cluster of cells that expressed genes seen in other species’ organizer cells.

Brivanlou and his colleagues then transplanted their embryo-like clusters of human cells onto 12-hour-old chicken embryos (which are the rough equivalent of a 14-day-old human embryo). The researchers found that as the modified embryos grew, the human organizer cells directed the chicken cells to differentiate and form a second chicken nervous system. That result mimics the findings of the 1924 salamander experiment, Brivanlou says, although his hybrid embryos did not live long enough to hatch.

Charting growth

Martin Pera, a stem-cell researcher at the Jackson Laboratory in Bar Harbor, Maine, is impressed with the study. “There’s quite a lot there that this system will lead to,” he says — including a better understanding of defects in the early development of human embryos that can lead to miscarriages, and the ability to compare the embryo-like structures with human stem-cell cultures to better define stem cells’ abilities.

The technique might also avoid the ethical issues associated with studying human embryos in the lab. “It’s a real advance — it’s beautiful this can be shown without the need of using embryos,” says Martin Blum, a developmental biologist at the University of Hohenheim in Stuttgart, Germany. “At the moment I could not think of a case where an early human embryo would be needed to answer basic questions.”

Brivanlou disagrees. “There is no substitute for studying the real embryo,” he says. “Everything else we do when we try to model kind of oversimplifies it.”

The next step, he says, is to determine how exactly the human organizer cells influence their neighbours. This could inform efforts to manipulate human stem cells into specific tissues or structures, as part of therapies to regenerate organs and tissues. “Human embryonic stem cells and eggs have all the information,” Brivanlou says. “Everything else is pushing the first domino.”

doi: 10.1038/d41586-018-05202-0
Origin and Immunological Functions of Spleen Stromal Cells


Embryonic mesenchymal progenitors within the splenic primordium (the clustering of cells from which the spleen develops) are the precursors of virtually all spleen stromal cell subsets, including follicular dendritic cells (FDCs), marginal reticular cells (MRCs), and fibroblastic reticular cells (FRCs).

Spleen stromal cell subsets appear as central regulators of organ development and tissue regeneration, although the precise cellular and molecular determinants involved in these processes remain largely unknown.

Distinct stromal cell subsets provide support for lymphocyte migration and locomotion and have unique functions involved in regulating adaptive immune responses.

The mammalian spleen is a peripheral lymphoid organ that plays a central role in host defense. Consequently, the lack of spleen is often associated with immunodeficiency and increased risk of overwhelming infections. Growing evidence suggests that non-hematopoietic stromal cells are central players in spleen development, organization, and immune functions. In addition to its immunological role, the spleen also provides a site for extramedullary hematopoiesis (EMH) in response to injuries. A deeper understanding of the biology of stromal cells is therefore essential to fully comprehend how these cells modulate the immune system during normal and pathological conditions. Here, we review the specificities of the different mouse spleen stromal cell subsets and complement the murine studies with human data when available.

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Photosynthetic Energy Transfer at the Quantum/Classical Border


Quantum mechanics diverges from the classical description of our world when very small scales or very fast processes are involved. Unlike classical mechanics, quantum effects cannot be easily related to our everyday experience and are often counterintuitive to us. Nevertheless, the dimensions and time scales of the photosynthetic energy transfer processes puts them close to the quantum/classical border, bringing them into the range of measurable quantum effects. Here we review recent advances in the field and suggest that photosynthetic processes can take advantage of the sensitivity of quantum effects to the environmental ‘noise’ as means of tuning exciton energy transfer efficiency. If true, this design principle could be a base for ‘nontrivial’ coherent wave property nano-devices.

Quantum Theory Describes Our World

Quantum mechanics is the cornerstone of modern physics and chemistry. All experiments done so far show that, while many aspects of quantum mechanics are counterintuitive and seem paradoxical, the description of quantum behavior is correct. An example of this is the famous double-slit experiment, which demonstrated that a single electron could travel in two paths and create an interference pattern with itself. This experiment validated the wave/particle duality concept, a key concept in quantum mechanics that will also play an important role in this review.

While quantum effects direct the mechanics of atoms and electrons, it is important to remember that the number of particles in a given volume increases with the cube of its radius, so going from 0.5 nm (a small molecule) to 5 nm (a typical protein) brings into play a thousand times more atoms. These dimensions place an explicit quantum simulation of a biological process beyond the reach of calculating power of current computers.

Nevertheless, quantum effects in biology are evident in daily life. Two major concepts of quantum mechanics govern their operation. The first is the quantized behavior of physical properties like energy and momentum. A simple demonstration is related to quantized energy levels (see Glossary) confined in small chemical structures. For example, a pigments’ absorption spectrum (Box 1) or Förster resonance energy transfer (FRET) (Box 2) between pigments.

Identifying the Fingerprints of Quantum Effects in Photosynthesis

Probing ultrafast processes requires sophisticated spectroscopic tools, such as 2D electron spectroscopy (2DES) [12345]. The introduction of these techniques to the study of photosynthetic EET processes resulted in the suggestion that coherent transfer could be detected in a small soluble antenna protein of a green sulfur photosynthetic bacterium containing eight pigments (the FMO protein) [6]. This was a revolutionary hypothesis, since for many years these EET processes were described by the more basic FRET energy transfer equations. FMO transports excitons from one end to another via eight chlorophyll molecules embedded in the protein, like currants in a bun. The small number of pigments in this protein made it an ideal test case for a 2DES study (for insight into 2DES methodology and its importance in biological and chemical quantum studies, see the recent review by Scholes and coworkers [4]). In photosynthesis, the picture that has emerged from these studies provides a remarkably detailed map of the dynamics of the EET process [78].

According to the coherent interpretation of the data, the exciton does not usually reside on a single chlorophyll, but is spread over several chromophores, creating a wave packet [910111213]. In this scenario, the phase of the wave packetbecomes important (Box 3). Dealing with waves, EET will be controlled by constructive and destructive interference patterns. In other words, changing phase differences between packets will control EET rates. This manifests itself as ‘beats’ in the rate of exciton transfer as the different paths interfere.

Since this original discovery, evidence for quantum coherent effects were reported for a number of photosynthetic LH and RC pigment–protein complexes (examples include [14151617181920212223242526]). However, it is important to note that the interpretation of these 2DES results is still debated. The beats in the 2DES spectra could be either due to true electronic coherences, where the beats are created by the quantum properties of the wave packet while energy is transferred, indicating the involvement of coherent wave packets. Alternatively, they could be due to coupling of the excitation to mechanical vibrations of the protein. The energies involved in exciting an electron from a ground state to an excited state in a photosynthetic pigment are large, of the order of 2 electron-volts. Molecular vibration energies of proteins take place at energies 10–100 times smaller. This means that the electron excitation could transfer energy to the vibrations, and these could in turn modulate electron transfer, thereby giving rise to beats without the need to invoke quantum coherence [272829].

A major challenge in this field is therefore to identify the contributions of incoherent and quantum coherent processes.

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Making Maps on a Micrometer Scale

Geographic information system software, created for mapping cities and continents, works equally well with the minuscule layers and inclusions that record a crystal’s history.

Researchers on the cutting edge of geochemistry are tracing Earth’s history through the clues recorded in tiny mineral crystals. Often, they must work with the microscopic (or nanoscopic) features in rare, hard-won specimens to pull apart the complete history of the mineral’s formation. Even in large pieces of rock, microscopic variability may be distributed throughout in patterns that contain valuable information. Researchers using microanalysis have read the information stored in layers of a single zircon crystal, the cements in a sandstone, tiny shells of sea creatures like ammonite hatchlings, and minerals in a meteorite.

A variety of imaging and chemical analysis techniques produce maps illustrating how chemical elements and crystal growth features are distributed across a specimen. Currently, these data are shared through static figures or images contained in a data repository, but this setup does not facilitate deeper inquiry and full use of spatial relationships. What if widely used geographic information system (GIS) software, which typically deals with data on the scale of many square kilometers, could be applied to data on a microscopic scale?

Here we showcase use of the free and open source software QGIS to integrate in situ chemical data with images to enrich interpretation.

Integrating the Information

Minimally destructive geochemical analysis at the nanometer to micrometer scale can peel apart the events that took place over the formation of a mineral crystal and still preserve the crystal for future analyses. This analysis is especially important for deciphering the geological history of a specimen that is small, rare, or zoned, like a 4.4-billion-year-old zircon.No one analytical technique, however, can provide all necessary information for many questions, and the range of instrument manufacturers and data types involved makes integrating data from various instruments difficult.

To understand, for instance, how cementation in a sandstone evolved or the chemical evolution of a magma, images from light microscopes or scanning electron microscopes (SEM) are used to examine petrographic relationships, and then electron probe microanalysis (EPMA) provides point analyses of elemental composition (Figure 1).

Zoned dolomite-ankerite grain from a polished rock surface mapped using QGIS software to composite several image layers
Fig. 1. To create this map of a zoned dolomite-ankerite grain from a polished rock surface, we used QGIS software to composite several SEM-backscattered electron image layers. We overlaid these with two SIMS transects and an EPMA data set. We added the final polygon layer (yellow dotted lines) to draw visual attention to different growth domains within the crystal. Data are from Denny et al. [2017]. Credit: A. C. Denny

In situ microanalytical techniques have become faster and more precise, and they are now routinely used in the geosciences [Valley and Kita, 2009; Sylvester and Jackson, 2016]. Microanalytical instruments like secondary ion mass spectrometers (SIMS), electron probe microanalyzers, and laser ablation–inductively coupled plasma–mass spectrometers produce large data sets from individual thin sections or chips (Figure 1). Other techniques like optical light microscopy, SEM, X-ray mapping, and nano-SIMS produce suites of images.

A Change of Scale

For years, scientists have managed field-scale data that span scales of meters to kilometers, incorporating images and point information using GIS software. However, in situ microanalytical data, like SEM images and SIMS or EPMA point analysis, also fundamentally contain spatial information that can be combined using GIS.

On a field scale, data in a map may have vector components (e.g., points, lines, or polygons) or raster components (e.g., images or similar pixel-based scans). In the case of microanalytical data, SIMS or EPMA data can be treated as vectors, and SEM scans or other images can be treated as rasters. Spatially overlapping sampling images and point analyses allow relation of these data sets to each other for visualization and further exploration.

Adapting an Open Source Tool

QGIS is a free, open source, user-friendly, cross-platform (Mac, Windows, Linux, Unix, and Android) software package for collecting and processing macroscopic geographic data. Under the banner of the Open Source Geospatial Foundation, a community of volunteers maintains and develops the software with financial support from corporate and nonprofit sponsors.

Although QGIS was not originally designed for microanalytical techniques, we have compiled in situ microanalytical data from multiple instruments to create integrated maps of individual samples.QGIS has many advantages, making it a good candidate for adoption by the wider microanalytical community for data visualization and management. First, the open-source nature removes the cost barrier to adopting the platform. Second, the software is supported by a growing international community of users and developers. Finally, custom plug-ins can be written in the Python, C++, and R computer languages, and these can provide ways of refining data input for different instruments. Plug-ins written in Python can be tailored to specific structured instrumental outputs to speed data compilation.

Map generation in QGIS for microanalytical data sets is straightforward (Figure 2). A tutorial structured to teach refined use of QGIS is available at the WiscSIMS Micro-QGIS website.

This workflow for data import into QGIS relies on X-Y coordinates from one instrument to calibrate the map units
Fig. 2. This workflow for data import into QGIS relies on x–y coordinates from one instrument to calibrate the map units. In our examples, we use SIMS files from a CAMECA IMS 1280 instrument for calibration, and the units are micrometers. We also use our SEM Image Placer plug-in to position tens of SEM images simultaneously. Results of this data integration are shown in Figure 3. Data are from Linzmeier et al. [2018]. Credit: B. J. Linzmeier and A. C. Denny

Creating Plug-ins

QGIS plug-ins can be created to solve specific problems relevant to a lab, analytical technique, or scientific question. We have used a plug-in called Plugin Builder to create several tools specific to the WiscSIMS laboratory at the University of Wisconsin–Madison. This platform provides a basic framework and files for building your own plug-in to interface with QGIS.

We have developed a plug-in that places images using the xy coordinates of a microscope stage to align SEM images with data maps from other instruments. The software parses a text file made by our SEM (Hitachi S3400-N) that contains image dimension, stage coordinates, and pixel size and loads the associated images into a QGIS map. We are distributing our SEM Image Placer plug-in on GitHub, so anyone can download, fork, modify, and make a pull request for the development under the GNU General Public License to extend this functionality to other types of SEMs and other microscopes with stage coordinates.

Integrating and Archiving a Diversity of Data

Using free, open source QGIS software for the integration of in situ microanalytical data sets improves our ability to integrate data from multiple instruments. It also decreases the time spent annotating and reformatting supplemental data sets for publication (Figures 1 and 3).

This map for AMNH 75647, currently the most analyzed ammonite in the world, was completely generated in the QGIS composer.
Fig. 3. This map for AMNH 75647, currently the most analyzed ammonite (extinct marine mollusk) in the world, was completely generated in the QGIS composer. After compiling the data, a user with intermediate-level skills could use this composer to create an initial figure in less than 20 minutes. The project file that was used to create this map integrates all the analytical data performed on this small SIMS mount. Data are from Linzmeier et al.[2018].

Data collected from multiple instruments can be compiled quickly using built-in tools and custom-designed components. Adapting GIS software to the microscale also enables us to perform more complex spatial analysis. Most important, these compiled microspatial data can be shared between collaborators and used to explore patterns that may not be obvious from static displays of images and data points.Our compilations use standard, widely used file formats, so they have the potential to interface easily with database infrastructure for archiving and depositing data collected with public funding [Chan et al., 2016]. This potential will ensure that extensive, expensive, and cutting-edge in situ geochemical data sets are easily shared and integrated into existing databases like Macrostrat using widely available formats and software.


We thank John Czaplewski, Shanan Peters, Ian Orland, and others for discussion and troubleshooting the QGIS workflow. The WiscSIMS laboratory is partially supported by the National Science Foundation (EAR03-19230, EAR13-55590) and the University of Wisconsin–Madison.


Cammack, J. N. (2015), SIMS microanalysis of the Strelley Pool Formation cherts and the implications for the secular-temporal oxygen-isotope trend of cherts, M.S. thesis, University of Wisconsin–Madison, Madison.

Cammack, J. N., et al. (2018), SIMS microanalysis of the Strelley Pool Formation cherts and the implications for the secular-temporal oxygen-isotope trend of cherts, Precambrian Res.304, 125–139, https://doi.org/10.1016/j.precamres.2017.11.005.

Chan, M. A., S. E. Peters, and B. Tikoff (2016), The future of field geology, open data sharing and cybertechnology in Earth science, Sediment. Rec., 14, 4–10, https://doi.org/10.2110/sedred.2016.1.

Denny, A. C., et al. (2017), Isotopically zoned carbonate cements in early Paleozoic sandstones of the Illinois Basin: δ18O and δ13C records of burial and fluid flow, Sediment. Geol.361, 93–110, https://doi.org/10.1016/j.sedgeo.2017.09.004.

Linzmeier, B. J., et al. (2018), Ion microprobe measured stable isotope evidence for the habitat and mode of life of ammonites in early ontogeny, Paleobiology, in press.

Sylvester, P. J., and S. E. Jackson (2016), A brief history of laser ablation inductively coupled plasma mass spectrometry (LA–ICP–MS), Elements12, 307–310, https://doi.org/10.2113/gselements.12.5.307.

Valley, J. W., and N. T. Kita (2009), In situ oxygen isotope geochemistry by ion microprobe, in Secondary Ion Mass Spectrometry in the Earth Sciences, MAC Short Course, vol. 41, edited by M. Fayek, pp. 19–63, Mineral. Assoc. of Can., Quebec.

Author Information

B. J. Linzmeier (email: benl@earth.northwestern.edu), Department of Earth and Planetary Science, Northwestern University, Evanston, Ill.; K. Kitajima, WiscSIMS Facility, University of Wisconsin–Madison; A. C. Denny, Department of Geoscience, University of Wisconsin–Madison; and J. N. Cammack, Department of Geoscience, University of Wisconsin–Madison; also at Geology Department, Fort Lewis College, Durango, Colo.

Citation: Linzmeier, B. J., K. Kitajima, A. C. Denny, and J. N. Cammack (2018), Making maps on a micrometer scale, Eos, 99,https://doi.org/10.1029/2018EO099269. Published on 17 May 2018.
Source: eos.org
Atomic Structural Models of Fibrin Oligomers


The space-filling fibrin network is a major part of clots and thrombi formed in blood. Fibrin polymerization starts when fibrinogen, a plasma protein, is proteolytically converted to fibrin, which self-assembles to form double-stranded protofibrils. When reaching a critical length, these intermediate species aggregate laterally to transform into fibers arranged into branched fibrin network. We combined multiscale modeling in silico with atomic force microscopy (AFM) imaging to reconstruct complete atomic models of double-stranded fibrin protofibrils with γ-γ crosslinking, A:a and B:b knob-hole bonds, and αC regions—all important structural determinants not resolved crystallographically. Structures of fibrin oligomers and protofibrils containing up to 19 monomers were successfully validated by quantitative comparison with high-resolution AFM images. We characterized the protofibril twisting, bending, kinking, and reversibility of A:a knob-hole bonds, and calculated hydrodynamic parameters of fibrin oligomers. Atomic structures of protofibrils provide a basis to understand mechanisms of early stages of fibrin polymerization.


Fibrin is an end product of blood clotting that forms the scaffold of hemostatic clots and obstructive thrombi in blood vessels. Fibrin is also a major component of the extracellular matrix and is involved in a broad range of cellular processes, including cell adhesion, migration, proliferation and differentiation, wound healing, angiogenesis, and inflammation (Weisel and Litvinov, 2017Litvinov and Weisel, 2017). Fibrin is widely used as a versatile biomaterial in a variety of applications, such as hemostatic sealants, tissue engineering, as a delivery vehicle for cells, drugs, growth factors, and genes, and matrices for cell culturing (Janmey et al., 2009Radosevich et al., 1997). Because of the fundamental biological and medical importance, molecular mechanisms of fibrin formation as well as fibrin structure and properties continue to be major areas of research (Weisel and Litvinov, 2013Weisel and Litvinov, 2017Litvinov and Weisel, 2016).

Fibrin formation is initiated by the cleavage of fibrinopeptides A and B from the N termini of Aα and Bβ chains of fibrinogen, respectively, to produce fibrin monomer. The release of fibrinopeptides A exposes an N-terminal α-chain motif GPR, called knob “A”, which binds to constitutively exposed hole “a” in the γ nodule of another fibrin molecule (Everse et al., 1998Kostelansky et al., 2002), resulting in the formation of an A-a knob-hole non-covalent bond (Litvinov et al., 2005). Exposure of knobs “A” is necessary and sufficient to form fibrin through the interaction with holes “a.” The release of fibrinopeptides B exposes an N-terminal β-chain motif GHRP, called knob “B”, which is complementary to hole “b” located in the β nodule of another fibrin molecule.

Fibrin polymerization begins when two monomeric fibrin molecules interact in a half-staggered fashion through the A-a knob-hole interaction. The addition of a third molecule is accompanied by an end-to-end association where, in addition to the A-a knob-hole interactions, the globular D regions of two adjacent molecules form the D:D interface. The D:D interface provides a junction between the monomers in one of the two strands in a fibrin trimer. Furthermore, fibrin monomers add longitudinally via the inter-strand A-a knob-hole bond formation and intra-strand D-D interactions to form fibrin oligomers. This growth continues until the fibrin oligomers reach the critical length of protofibrils: oligomers made of ∼20–25 fibrin monomers. Fibrin protofibrils self-associate laterally to form twisted fibers of variable thickness. These branches form a three-dimensional fibrin network called a clot (Weisel and Litvinov, 2017).

The monomeric fibrin is essentially identical in structure and composition to fibrinogen except for small fibrinopeptides A and B, which are cleaved when fibrinogen is converted to fibrin, and αC domains, which are bound to the central nodule in fibrinogen but detached in fibrin (Medved et al., 2001). Therefore, fibrin oligomers and protofibrils can be reconstructed using resolved crystal structures of the human fibrinogen molecule and parts of fibrinogen and fibrin molecules, including the fibrinogen fragment D and the double-D fragment from crosslinked fibrin (see Table S1). Yet using the crystal structures of fibrinogen or fibrin [together denoted as fibrin(ogen)] is challenging. First, the crystallographic data available are incomplete. There are several flexible unstructured portions that are not resolved crystallographically yet are essential for fibrin formation, including residues 1–26 and 1–57 at the N-termini of the Aα and Bβ chains, respectively, and residues 201–610, 459–461, and 395–411 at the C-termini of the Aα, Bβ, and γ chains, respectively (Kollman et al., 2009). Second, a manifold of possible spatial arrangements of fibrin monomers when forming a protofibril makes in silico reconstruction of fibrin protofibril difficult. Third, the large system size requires using vast computational resources: a 0.5- to 0.6-μm-long protofibril made of 20 fibrin monomers contains ∼60,000 amino acids, which corresponds to ∼106 atoms.

Determination of atomic structures of fibrin oligomers cannot be accomplished by X-ray crystallography and/or electron microscopy, owing to the unstable nature of these heterogeneous intermediate supramolecular assemblies and their characteristic elongated shape. Yet atomic-level information about these structures is necessary to elucidate the mechanisms of formation and properties of fibrin polymers, which provide the three-dimensional scaffold necessary to maintain the integrity and viscoelasticity of blood clots and thrombi. Here we employed multiscale modeling to computationally reconstitute the atomic structures of double-stranded fibrin oligomers of varying length. The atomic structural models were successfully validated using high-resolution atomic force microscopy (AFM) imaging of fibrin oligomers.

We employed the molecular dynamics (MD) simulations of atomic structural models (Brooks et al., 2009Zhmurov et al., 2012) and Cα-based self-organized polymer (SOP) models of fibrin(ogen) and its fragments (Hyeon et al., 2006), accelerated on graphics processing units (GPUs) (Zhmurov et al., 2010aZhmurov et al., 2010bZhmurov et al., 2011Alekseenko et al., 2016), to perform a step-by-step reconstruction of a complete atomic structure of a 19-monomer-long fibrin protofibril using the recently published structure of a short fibrin oligomer (Zhmurov et al., 2016). The protofibril structure has interesting properties, such as twisting, bending, and kinking, and the presence of free knobs “B” necessary for formation of additional intra- and inter-protofibril bonds. The models obtained enabled us to explore the dynamic structural transitions in fibrin protofibrils and to predict experimentally unavailable dynamic characteristics of fibrin oligomers and protofibrils, including density, radius of gyration, diffusion coefficient, and intrinsic viscosity.


Stepwise Reconstruction of Fibrin Oligomers and Protofibril

As a building block, we used the structure of short double-stranded fibrin oligomer FO2/3 with two fibrin monomers in the first and three monomers in the second strands (Figure 1A). Using this structure, we performed stepwise elongation to create longer oligomers up to the length of a protofibril. The full-atomic model of FO2/3 was constructed computationally in our previous study (Zhmurov et al., 2016) using all 27 relevant crystal structures of fibrinogen and its fragments resolved to date (Table S1). The structure of FO2/3 showed good agreement with high-resolution AFM images (Zhmurov et al., 2016). In this work, we took the next step to elongate several-fold the known structure of FO2/3 in order to reconstruct longer fibrin oligomers FOm/n (m/n is the number of fibrin monomers in the first/second strand). This enabled us to recreate short fibrin oligomers from FO2/3 to FO5/6. A mere replication of the FO2/3 structure along the longitudinal axis has resulted in formation of elongated oligomers and protofibrils that do not show any twisting detected in experimental AFM and electron microscopy images (Weisel et al., 1987Medved et al., 1990Protopopova et al., 2015Huang et al., 2014). To overcome this problem, we designed an approach that uses two main crystal structures of the D:D junction. These structures correspond to the straight conformation (PDB: 1N86) of the D:D interface, used to recreate shorter fibrin oligomers, and the bent conformation (PDB: 1FZG) of the D:D interface, which we used to recreate longer oligomers (and a protofibril). To recreate twisted structures, we align two FO2/3constructs using the straight conformation of D-D junctions and then gradually switch to the bent conformation of the D:D junction (STAR Methods). This builds in the desired twist in the fibrin strands, in full agreement with AFM and electron microscopy experiments (Protopopova et al., 2015Weisel et al., 1987).

A step-by-step reconstruction of short fibrin oligomers (FOm/n) is illustrated in Figure 1B (elongation step with the straight conformation of D:D interface). Reconstruction of longer fibrin oligomers and protofibril (FP9/10) is illustrated in Figure 1C (a procedure to introduce a twist; bent conformation of D:D interface; see also STAR Methods for more details). In step A of the twisting procedure, coarse-graining of FO2/3 is performed (diamonds in Figure 1B) and Langevin simulations of the Cα-based representation of FO2/3 is carried out to switch from the straight to the bent configuration of the D:D interfaces. In step B of the twisting procedure, the obtained conformation of FO2/3 is back-mapped and energy-minimized using the all-atom solvent-accessible surface area model of implicit solvation. Next, we perform the elongation procedure. The atomic model of FO2/3 with knobs “A” and “B” is replicated to reconstruct fibrin oligomers (FOn/m) of the desired length. In the last structure-addition step, the αC regions are incorporated into each fibrin monomer, and the covalent γ-γ crosslinks between residues γ398 and γ406 of abutted fibrin monomers are introduced (Rosenfeld et al., 2015). The final structures of double-stranded fibrin polymers from the structure-addition step (Table 1) were energy-minimized to exclude possible steric clashes.

Table 1Molecular Parameters of Fibrin Monomer, Oligomers FOn/m, and Protofibril FP9/10Calculated Based on the Atomic Models Reconstructed In Silico with and without the αC Regions: Molar Mass (M), Radius of Gyration (Rg), Diffusion Coefficient (D), Density (ρ), and Intrinsic Viscosity (η)
Constructs M(G/mol) Rg(nm) D (cm2/s) ρ(g/cm3) η(cm3/g)
Fibrin(ogen) monomers
Truncated des-αC fibrin monomer 246,395 12.5 ± 2.0 (2.5 ± 0.3) × 10−7 1.361 24 ± 9
Full-length fibrin monomer 332,418 12.7 ± 1.3 (1.9 ± 0.2) × 10−7 1.328 38 ± 19
Double-stranded fibrin oligomers/protofibril without the αC regions
FO1/2 739,185 12.5 ± 2.0 (1.4 ± 0.1) × 10−7 1.350 42 ± 12
FO3/4 1,724,765 19.6 ± 2.1 (8.1 ± 0.4) × 10−8 1.352 114 ± 18
FO5/6 2,710,345 41.6 ± 2.2 (6.0 ± 0.3) × 10−8 1.346 209 ± 29
FO7/8 3,695,925 67.5 ± 2.1 (4.79 ± 0.08) × 10−8 1.344 344 ± 19
FP9/10 4,681,505 117.1 ± 2.0 (4.0 ± 0.1) × 10−8 1.342 483 ± 42
Double-stranded fibrin oligomers/protofibril with the αC regions
FO1/2 997,254 20.1 ± 1.9 (1.14 ± 0.04) × 10−7 1.326 50 ± 7
FO3/4 2,326,926 41.8 ± 2.4 (6.8 ± 0.2) × 10−8 1.325 113 ± 17
FO5/6 3,656,598 67.5 ± 2.0 (5.1 ± 0.1) × 10−8 1.325 204 ± 12
FO7/8 4,986,270 93.0 ± 1.7 (4.15 ± 0.07) × 10−8 1.324 309 ± 14
FP9/10 6,315,942 116.8 ± 1.9 (3.4 ± 0.2) × 10−8 1.324 450 ± 27

View Table in HTML

The values of RgDρ, and η are for 20°C.

Atomic Structures and AFM Images of Fibrin Oligomers and Protofibrils

To compare in silico structures with AFM images, we employed the computational Monte Carlo procedure, which overlaps the positions of the centers of mass of D and E regions in the atomic structural model and in AFM images (see STAR Methodsand Figure 2B). To quantify the agreement between AFM images and atomic models, we monitored the dynamics of total root-mean-square deviation (RMSD) in Monte Carlo runs. The trajectories in Figure 2C show a great reduction in RMSD values to 0.9–2 nm depending on the oligomer length.

We first recreated atomic models of short fibrin oligomers by applying the elongation procedure (Figure 1B) to the initial structure of FO2/3, to reconstruct the structures up to nine monomers long (FO4/5Figure 2A). We correlated these structures with their high-resolution AFM images for short oligomers containing up to nine fibrin monomers (FO4/5Table 1). In AFM imaging, short fibrin oligomers appear as elongated constructs with regularly spaced heart-shaped nodules and two adjacent nodules facing in opposite directions (Figure 2). Each of these nodules corresponds to a single D-E-D trinodular unit. The derived atomic structures and AFM images for short fibrin oligomers are compared in Figures 2B and 2D, which show good agreement between the structures obtained experimentally and computationally. Next, we turned to reconstruction of longer oligomers (FO5/6 and longer) up to a protofibril FP9/10. We elongated oligomer FO4/5 with FO2/3 using the elongation procedure described in the STAR Methods (Figure 1B). The structures obtained in silico did not compare well with their corresponding AFM images (Figures 2E and 3F ), which could be due to protofibril twisting not present in the modeled structures. Quantitatively, this is reflected in higher values of RMSD for longer structures (0.9–1.0 nm for short oligomer FO3/3 versus 1.8–2.0 nm for long oligomer FO6/7; see Figure 2C). Next, we elongated short oligomers up to the length of a fibrin protofibril FP9/10 (Figure 3A and Table 1). At this length scale, the structure of FP9/10 obtained with the straight conformation of D:D interface did not capture the helical twist observed in AFM images (Figures 2E, 2F, and 3D). Using the structure of FP9/10obtained computationally, we calculated the helical radius and helical pitch, which came to 650 nm and 3,300 nm, respectively. This is a straight structure on the protofibril length scale of ∼500 nm.

To build in a twist in fibrin oligomers and protofibrils, we first applied the twisting procedure (Figure 1C) and then the elongation procedure (Figure 1B). The equilibrium structure obtained shows that the transition from the straight to the bent double-D conformation with the twisting procedure results in an overall shape change of FP9/10 from the parallel double-stranded (Figure 3A) to the twisted (double-stranded) helical form (Figure 3B). Transient structures of FP9/10 populated in the course D:D interface remodeling are displayed in Figure S2 (see Video S1). As the protofibril FP9/10 twists, the helical radius and helical pitch decreases, respectively, from 650 nm to 5 nm and from 3,300 nm to 400 nm (see Figure S2 and Video S1), as a result of dynamic remodeling of all D:E:D interfaces reinforcing the protofibril’s structure. The comparison of atomic structures and AFM images of longer fibrin oligomers showed better agreement (Figure 3D). Note that the average values for RMSD are slightly lower for twisted structures (1.2 ± 0.3 nm; sample size = 30) compared with straight oligomers (1.4 ± 0.4 nm; sample size = 30).

Complete Structure of a Fibrin Protofibril with the αC Regions

The C-terminal part of fibrinogen’s Aα chain, called the αC region (residues Aα221–610), consists of the proline-rich unstructured αC connector (Aα221–390) and the relatively compact αC domain (Aα391–610) (Tsurupa et al., 2009). The αC region is missing in all the crystal structures of fibrinogen and its fragments resolved to date. The structure of bovine fibrinogen’s αC domain was partially resolved by nuclear magnetic resonance (Burton et al., 2007), yet the structure of human fibrinogen’s αC domain is not known (Tsurupa et al., 2009). We recreated this structure using sequence homology between the human and bovine fibrin(ogen) with the Modeller software suite (Webb and Šali, 2017). Structure snapshots of the αC domain randomly selected from independent MD runs showed a double β hairpin stabilized by the S-S bond. The αC-domains can be separated into the N-terminal and C-terminal subdomains as suggested earlier (Tsurupa et al., 2009Tsurupa et al., 2012). Since αC connectors are not resolved by the X-ray crystallography, they do not possess stable secondary or tertiary structure. Therefore, the incorporation of αC connectors in a random coil conformation does not lead to any structural artifacts. In a structure-addition procedure (Figure 1D), we incorporated the missing C-terminal portions of the α connector in a random conformation to arrive at the complete atomic structure of a fibrin protofibril FP9/10 (Figure 3C).

We compared the full-atomic structure of FP9/10 containing αC regions with the AFM images (Figure 3). The protofibril’s shape and positions of the αC regions in the atomic model and AFM images of FP9/10 agreed well. The αC regions were predominantly perpendicular to the protofibril axis. Although the αC regions were occasionally interconnected, they were mostly single. Not all αC regions were seen in AFM images (assuming two αC regions per monomer), and we identified on average 1.6 αC regions per monomer. Some of the αC regions might have been proteolytically truncated in the fibrinogen purified from plasma or have been adsorbed at positions not clearly visible on the surface (e.g., under the protofibril backbone).

Conformational Dynamics of the Fibrin Protofibril Chain

From experimental AFM images, the average contour length of fibrin protofibrils is 213 ± 101 nm and the average end-to-end distance is 197 ± 86 nm (n = 30). This gives an average end-to-end to contour length ratio of 0.94 ± 0.09 (n = 30), which shows that protofibrils are bent. Since our in silico structures were recreated based on the X-ray data, they lack this conformational flexibility. To explore dynamic transitions in the protofibril structure, we performed MD simulations using the obtained structure of FP9/10 (see STAR Methods and Video S2), which revealed significant structural alterations including bending (Figure 4A) and kinking (Figure 4B). This agrees well with the previously published experimental data (Protopopova et al., 2015Protopopova et al., 2017Huang et al., 2014Chernysh et al., 2011Medved et al., 1990Hunziker et al., 1988Fowler et al., 1981) and with our AFM images (Figure 4).

The distribution of end-to-end distances (i.e., the distances between centers of the end D:E:D complexes) in FP9/10 from MD simulations is displayed in Figure 4F. The average end-to-end distance in FP9/10 is R = 330 ± 15 nm. With the contour length L0 = 403 nm (9 monomers, 44.8-nm length of monomer), the average persistence length of protofibril FP9/10 is Lp = 320 ± 80 nm (see STAR Methods). There is a variation in experimental estimates of Lp for fibrin protofibrils, with values ranging from ∼100 nm to 500 nm (Piechocka et al., 2016Storm et al., 2005). Based on our AFM images, Lp = 420–480 nm, which is in good agreement with our simulations. The higher value of Lp observed in AFM images can be attributed to the non-covalent interactions (adsorption forces) between the protofibrils’ backbone and the surface. Reversible formation of kinks in the protofibril structure observed in our simulations was due to simultaneous bending of the coiled coils in adjacent strands around the positions identified in the previous simulation studies (Köhler et al., 2015Figure 3). This is in agreement with AFM images, in which kinks were indeed detected (Figure 4E). Deviations of the atomic structures from the AFM images at the protofibril’s tails are due to limited sampling of the conformational space in the MD simulations. The probability distribution of kinking angles from MD simulations for FP9/10 is shown in Figure 4G.

To quantitatively compare the AFM images and the atomic structural models, we computed the distributions of distances between adjacent D regions (Figure 4H), distribution of distances between D and E regions in DED constructs (Figure 4I), and distribution of distances between DED complexes (Figure 4J). To probe the bending rigidity of protofibrils, we computed the distributions of angles formed by three DED complexes (Figure 4K). To extract these characteristics from AFM images, we only selected protofibrils in which these fragments are visible and located their geometric centers; in the simulations, we computed the centers of mass of these fragments. The average values of all four quantities from AFM images and equilibrium MD simulations agree well (see Table S2), although SDs are larger in AFM images.

Structural Transitions in Fibrin Protofibril

Dissociation of A:a Knob-Hole Bonds

The long 10-ms MD simulations of FP9/10 showed that the A:a knob-hole bonds dissociate. This significantly weakens the D:E:D interface, leading to disruption of the D:D junction (Figure 4C), which does not occur when the A:a knob-hole bonds are intact. The D:D junction is the weakest link in the single-stranded fibrin oligomers (Zhmurov et al., 2011Zhmurov et al., 2012). In accord with these findings, AFM images also show irregularly shaped D:E:D fragments, which suggests the D:D interface disruption (see Figures 2E, 2F, 3E, 4D, and 4E). These results point to the importance of γ-γ covalent crosslinking, which reinforces the D:D interface when fibrin protofibrils form.

αC Regions

To sample conformations of the αC regions with flexible βN regions, we performed 10-ms equilibrium MD simulations of the protofibril FP9/10 with a constrained protofibril backbone and free knobs “B” (STAR Methods; see Video S3). We constructed the probability distribution of the distances between the protofibril longitudinal axis and the centers of mass of αC domains and compared it with the experimental histogram of the same quantity. Figure 5B shows that the agreement is very good, albeit the SDs are smaller in the simulations. This might be due to overstabilization of the αC domains in the simulations. The structure of the αC domain is not resolved experimentally, which suggests that it is not stable. Longer αC connectors are typically bent, which explains why the average distance between the αC regions and the protofibril backbone is only 17 nm (Figure 5B).

B:b Knob-Hole Interactions

We explored the conformational transitions in the βN regions with knobs “B.” The GHR active sequence does not drift far away from the central nodule, making the intra-protofibril B:b highly unlikely to form (Figure 5E). This suggests that additional structural changes in the protofibril are required for the B:b knob-hole bonds to form within the protofibril, in full agreement with earlier reports (Medved et al., 2001). These transitions (B:b knob-hole bond formation) cannot be sampled in MD simulations due to the limited time span (10 ms), and there might be additional putative inter-atomic contacts that guide the βN regions toward the holes “b.” There is experimental evidence suggesting that the B:b knob-hole bonds can form both between the fibrin strands inside the protofibril and between the protofibrils (Litvinov et al., 2007Blombäck et al., 1978Weisel, 1986). For this reason, we recreated two protofibril constructs: one with knobs “B” bound to holes “b,” and the other with free knobs “B”; see the PDB files in Data S1 for knobs-in structure and Data S2 for knobs-out structure.

Hydrodynamic Parameters of Fibrin Oligomers and Protofibril

We calculated the (hydro)dynamic molecular characteristics for double-stranded fibrin oligomers and protofibrils (STAR Methods) and profiled them as a function of their size (Figure 6 and Table 1). First, we compared our theoretical predictions with available experimental values for some of these quantities. Very good agreement was found for the (translational) diffusion coefficient D, i.e., (1.5–2.2) × 10−7 cm2/s (experiment for full-length fibrinogen; Raynal et al., 2013) versus (2.5 ± 0.3) × 10−7cm2/s (our simulations for truncated fibrin monomer without αC regions). Slightly lower values of D obtained for the full-length fibrin monomer can be attributed to the presence of bulky αC appendages, which are absent in truncated fibrin variants. Using confocal microscopy, Chernysh et al. (2011) estimated the diffusion coefficient (D) for 500-nm-long protofibril to be D = 3.7 × 10−8 cm2/s. This is in very good agreement with our values for FP9/10, i.e., D = (3.4 ± 0.2) × 10−8 cm2/s for the full-length molecules and D = (4.0 ± 0.1) × 10−8 cm2/s for those with truncated αC region (Table 1). Given these values of the diffusion coefficient the time needed for the protofibrils to travel toward one another will be fractions of a second, which is significantly shorter than overall polymerization timescale of minutes under similar conditions (Protopopova et al., 2017). Thus, the lateral aggregation of protofibrils is not limited by their diffusion.

The density of fibrin oligomers (1.34–1.36 g/cm3) was also found to be in good agreement with experiments (ρ = 1.38 g/cm3Adamczyk et al., 2012). The density of fibrin with flexible αC regions (1.32–1.33 g/cm3) was lower than the density of fibrin without αC regions (1.34–1.36 g/cm3). Theoretical values of the intrinsic viscosity ηfor the truncated fibrin (24 ± 9 cm3/g) and full-length fibrin monomer (38 ± 19 cm3/g) are also within the experimental range (21–48 cm3/g; Adamczyk et al., 2012). Larger variability in the theoretical values of η for the full-length fibrinogen is due to higher extensibility of αC appendages (Table 1). This supports our findings, namely that fibrinogen in solution exists in two conformational populations: one population with a lower value of η corresponding to conformations of fibrin’s αC domains attached to the central nodule; and the other population with a higher value of η that corresponds to conformations with free αC regions (Zuev et al., 2017). The agreement between experimental and theoretical values of Dρ, and η we have obtained for fibrin monomers and the structures we have recreated enabled us to predict the values of Dρ, and η and radius of gyration Rg for fibrin oligomers and protofibrils not available experimentally (Table 1). We also derived analytical expressions that allow for the extrapolation of these quantities to fibrin protofibrils of arbitrary length (Figure 6).


Fibrin oligomers and protofibrils are important intermediate products formed early during fibrin polymerization. Resolution of atomic structures of fibrin oligomers and protofibrils is needed to illuminate the mechanisms of the early stages of fibrin formation, including lateral aggregation of protofibrils, and to characterize the remarkable extensibility and viscoelasticity of fibrin fibers (Liu et al., 2010Litvinov and Weisel, 2017). Yet experimental determination of the structure and characterization of the properties of double-stranded fibrin polymers is difficult due to their elongated shape and highly unstable nature. We employed a powerful combination of the state-of-the-art experimental AFM imaging technique and theoretical approaches to multiscale modeling accelerated on a GPU to gather the atomic-level information about the structure and properties of fibrin oligomers and protofibrils. Using the full-atomic structure of a short fibrin oligomer FO2/3 (Figure 1Zhmurov et al., 2016), here we have reconstructed the atomic structures of longer fibrin oligomers FO3/4–FO7/8 up to a 19-mer protofibril FP9/10 (Figures 2 and 3Table 1). These constructs involve γ-γ crosslinking, A:a and B:b knob-hole bonds, and αC regions—all important functional elements of fibrin—and carbohydrates. The double-stranded fibrin structures were successfully validated through the direct comparison with high-resolution AFM images of oligomers and protofibrils (Figures 2 and 3Data S1 and S2).

Early products of fibrin polymerization are two-stranded oligomers (Fowler et al., 1981Chernysh et al., 2011Huang et al., 2014). A common feature of fibrin oligomers visualized with transmission electron microscopy is their twisted helical shape, although reported parameters of the oligomers’ helicity are highly variable. Medved et al. (1990) showed that some protofibrils form twisted structures with a helical pitch of ∼100 nm, whereas other protofibrils are nearly straight. In agreement with this study, we found that the helical pitch decreases from 3,300 nm to 400 nm (Figure 3) following the transition from the straight conformation (PDB: 1N86) to the bent conformation (PDB: 1FZG) of the D:D interface (Figures 3A, 3B, and S2), and the helical radius decreases from 650 nm to 5 nm. This points to the important role played by the D:D interfacial flexibility in early stages of fibrin polymerization. We did not observe a helical pitch <400 nm, which might be due to the experimental conditions used in previous studies (Medved et al., 1990) or to crystal packing forces in the atomic structures used. In most experiments, fibrin protofibrils are straight and thin, which agrees with our results. After reaching a certain length, fibrin protofibrils aggregate laterally to form thick twisted fibers. Fibrin fibers have a 20- to 60-nm helical radius and ∼2,000-nm helical pitch (Weisel et al., 1987), and continue to twist as they grow.

The reconstructed double-stranded fibrin oligomers and protofibrils correspond to the known ultrastructures, but surpass the available experimental data in spatial resolution. We are aware of other models of fibrin protofibrils (Yang et al., 2000Pechik et al., 2006Huang et al., 2014). The model proposed by Yang et al. (2000)captures the main structural features of fibrin oligomers, including the half-staggered molecular overlay formed by two fibrin strands. However, this model is ad hoc rather than systematic, and lacks a detailed analysis of the crystal forms. This model provides a static view of fibrin structure with missing γ-γ crosslinking, A:a and B:b knob-hole bonds, and αC regions. Another model (Huang et al., 2014) captures the half-staggered molecular arrangement of fibrin strands, and has a helical pitch of 90 nm. Yet a closer look reveals major steric clashes in the DED regions, which make the A-a bond formation unlikely. Also, this model is lacking γ-γ crosslinking, knob-hole bonds, and αC regions, and is based on the chicken fibrinogen structure (PDB: 1M1J).

We employed equilibrium MD simulations of fibrin protofibril FP9/10 to explore the dynamic structural transitions that occur in double-stranded fibrin polymers. Fibrin protofibrils behave like other double-stranded biopolymers, such as double-stranded DNA, but with a longer 320-nm persistence length, and show a high degree of bending. A theoretical probability density curve shows that due to bending, the end-to-end distance in FP9/10 decreases from ∼400 nm (contour length) to ∼330 nm (Figure 4F). This might be important for the fiber formation and fiber branching (Figure 4). Experimental AFM images reveal more bending flexibility than the in silico structures, and the protofibril’s bending becomes more pronounced with increasing length. We also observe reversible kinking of the protofibril backbone with the 80° to 140° kinking angle range and an average kinking angle of 115° (Figure 4G). Protofibril bending and kinking could be one of the mechanisms of initiation of branch points in growing fibrin fibers.

In the simulations, we observed the dissociation of A:a knob-hole non-covalent bonds, which was followed by the disruption of the D:E:D interface. This suggests a secondary role played by the D:D interface in fibrin polymerization, and also potentially supports the so-called Y-ladder model of fibrin fiber growth (Rocco et al., 2014). According to this model, the D:E:D interface becomes stable only after both knobs “A” are bound to their corresponding holes “a” (Rocco et al., 2014). Since upon the disruption of D:E:D interface and D-region rotation one A:a knob-hole bond is completely dissociated, a knob “A” and a hole “a” might become available for inter-protofibril cross-coupling. Another fibrin monomer from another protofibril could then bind, thus initiating a branch point. Formation of branch points is visible in some of the protofibril images (Figure 4E). We did not observe formation of new A:a knob-hole bonds in the millisecond timescale of simulations, hence this transition occurs in a longer timescale.

The length of αC connectors is very important for mechanical properties of fibrin fibers (Falvo et al., 2008). Since the αC domains are capable of interacting with each other (Tsurupa et al., 2011Tsurupa et al., 2012Litvinov et al., 2007) and with the globular parts of fibrin molecules (Tsurupa et al., 2009), it is important that they have an optimal length. When the αC connectors are long (as in human fibrinogen) their αC domains tend to form non-covalent bonds with other αC domains within the same protofibril and between the protofibrils. When the αC connectors are short (as in chicken fibrinogen), the αC domains hardly form binding contacts between protofibrils but only within the protofibril. We see in the simulations and in AFM images that the span of the αC regions is long enough so that the αC domains can form the αC-αC contacts within the protofibril and between protofibrils (Figure 5). The experimental histogram of the lengths of αC region shows the 10- to 35-nm range and an average length of 17.3 nm; the theoretical probability density curve reveals a smaller 10- to 20-nm range and a similar average length of 14.7 nm. This large variability also explains why in AFM images were on average 1.6 αC regions per fibrin monomer (<2). Our results imply that the conformational dynamics of αC regions plays a role in defining the thickness of fibrin fibers (number of protofibrils in a fiber).

The physiological role of B:b knob-hole bonds is not yet fully understood (Weisel and Litvinov, 2017). Although knobs “B” are long enough to reach and bind to the corresponding holes “b” in the same protofibril, our simulations of FP9/10 with free knobs “B” show that they have a limited span due to thermal fluctuations (Figure 5E). Hence, formation of intra-protofibril B:b contacts is possible only when Nβ regions are close to the globular parts of fibrin, interacting with γ and β nodules of adjacent molecules (Moskowitz and Budzynski, 1994). These interactions can guide the knob “B” to the hole “b” or/and to the thrombin active-site cleft (Pechik et al., 2006). Upon formation of B:b knob-hole bonds, the β nodule dissociates from the α-helical coiled coil, which results in the exposure of the tissue plasminogen activator and plasminogen binding cites in the coiled coil (Medved et al., 2001). This transition might help to bring holes “b” of adjacent protofibril closer to knobs “B,” thus facilitating the inter-protofibril contacts’ formation. Our simulations for protofibril FP9/10 suggest that the intra-protofibril B:b contacts are less probable than the inter-protofibril B:b contacts, which also explains why the formation of fibrin fibers occurs even in the absence of knobs “B” (Moskowitz and Budzynski, 1994Weisel, 1986).

We calculated the molecular hydrodynamic parameters for double-stranded fibrin oligomers and protofibrils, which are not available experimentally (Table 1), and extracted the scaling laws for RgDη, and ρ as functions of their size N (number of fibrin monomers; Figure 6). The protein density ρ was found to depend on Nexponentially (Figure 6C) in full agreement with the predictions made by Fischer et al. (2004). The profile of Rg shows a linear increase with N starting from 5 to 7 monomers (Figure 6A), because at larger N fibrin oligomers are pseudo-one-dimensional with size growing with N. This also explains why the intrinsic viscosity ηincreases quadratically with N. According to the Flory theory, η = ΦRg3/M, where Φis a universal constant and M is the molar mass (Doi and Edwards, 1986). Indeed, for a linear polymer Rg ∼ N and M ∼ N, and so η ∼ N2 (Figure 6D).

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Scientists make strong, super-tough carbon sheets at low temperature

An international research team led by scientists at Beihang University in China and The University of Texas at Dallas has developed high-strength, super-tough sheets of carbon that can be inexpensively fabricated at low temperatures.

The team made the sheets by chemically stitching together platelets of graphitic , which is similar to the graphite found in the soft lead of an ordinary pencil. The fabrication process resulted in a material whose mechanical properties exceed those of carbon fiber composites that are currently used in diverse commercial products.

“These sheets might eventually replace the expensive carbon fiber composites that are used for everything from aircraft and automobile bodies to windmill blades and sports equipment,” said Dr. Ray Baughman, the Robert A. Welch Distinguished Chair in Chemistry at UT Dallas and director of the Alan G. MacDiarmid NanoTech Institute. Baughman is a corresponding author of an article describing the material published online this week in the Proceedings of the National Academy of Sciences.

Today’s carbon fiber composites are expensive in part because the carbon fibers are produced at extremely high temperatures, which can exceed 2,500 degrees Celsius (about 4,500 degrees Fahrenheit).

“In contrast, our process can use graphite that is cheaply dug from the ground and processed at temperatures below 45 degrees Celsius (113 degrees Fahrenheit),” said Dr. Qunfeng Cheng, professor of chemistry at Beihang University and a corresponding author. “The strengths of these sheets in all in-plane directions match that of plied carbon fiber composites, and they can absorb much higher mechanical energy before failing than carbon fiber composites.”

Graphite consists of platelets made up of stacked layers of . Graphene is simply a single layer of carbon atoms, arranged in a pattern that looks like a chicken wire mesh fence, where each hexagon in the mesh is formed by six carbon atoms.

“While scientists can continuously make large sheets of graphene by high-temperature processing, and have shown these sheets to have remarkable strength, it is impractical to make thick plates of graphite by merely stacking large-area graphene sheets,” Cheng said. “One would need to stack about 150,000 graphene sheets to make a graphite sheet having about the thickness of a human hair.”

The researchers found inspiration in natural nacre, also known as mother-of-pearl, which gives some seashells their strength and toughness. Nacre is composed of parallel platelets that are bound together by thin layers of organic material, similar to the way bricks in a wall are held together by mortar.

“Instead of mechanically stacking large-area graphene sheets, we oxidize micron-size graphite platelets so that they can be dispersed in water, and then filter this dispersion to inexpensively make sheets of oriented graphene oxide,” Baughman said. “This process is akin to hand-making sheets of paper by filtering a slurry of fibers.

“At this stage, the sheets are neither strong nor tough, meaning they cannot absorb much energy before rupturing,” he said. “The trick we use is to stitch together the platelets in these sheets using sequentially infiltrated bridging agents that interconnect overlapping neighboring platelets, and convert the oxidized graphene oxide to graphene. The key to this advance is that our bridging agents separately act via formation of covalent chemical bonds and van der Waals bonds.”

Sheets that incorporated the bridging agents were 4.5 times stronger and 7.9 times tougher than agent-free sheets, said Beihang University PhD student Sijie Wan, who is a lead author of the journal article. “Unlike carbon fiber composites, no polymer matrix is needed,” he said.

“While sheets of expensive  can provide a similar strength in all sheet-plane directions, the energy that they can absorb before fracture is about one-third that of our sequentially bridged graphene sheets,” Wan said. “Because our sheets are fabricated at , they are low cost. In addition to exhibiting high  strength, toughness and fatigue resistance, they have high electrical conductivity and are able to shield against electromagnetic radiation. These properties make these sequentially bridged graphene sheets quite attractive for possible future applications.”

Explore further: For graphite pellets, just add elbow grease

More information: Sijie Wan el al., “Sequentially bridged graphene sheets with high strength, toughness, and electrical conductivity,” PNAS (2018). www.pnas.org/cgi/doi/10.1073/pnas.1719111115

Read more at: Phys.org

107 Studies Published in a Cancer Journal Have Just Been Retracted

In a massive cleanup, 107 articles have just been retracted from the open-access cancer research journal Tumor Biology.

“After a thorough investigation we have strong reason to believe that the peer review process was compromised,” writes editor-in-chief Torgny Stigbrand in the retraction notice.

Peer review is one of the golden standards that help sort the wheat from pseudoscientific babbling, making the process an integral part of academic publishing.

But there is massive publishing pressure in the scientific community, and with about 2.5 million papers published each year, some of those inevitably end up cutting corners. In this case, the transgression was what’s known as ‘fake peer review’.

Scientists are often asked to provide recommendations for potential reviewers of their work. While that sounds like an obvious invitation to cheat, it actually makes sense when the work is really specific and few others do similar research.

But it’s easy to game the system by providing a fake reviewer email address, impersonating an actual researcher and sending the journal a super-positive review in their name.

“The articles were submitted with reviewer suggestions, which had real researcher names but fabricated email addresses,” Springer representative Peter Butler told Yan Jie at Sixth Tone.

It’s a pretty massive lot of retractions all at once, but a few of the big academic publishers have been sweeping their portfolios for potential breaches, including fake peer review, plagiarism, data fabrication and more.

This time, the 107 papers were published between 2012 and 2016, and most were authored by Chinese researchers, although that doesn’t automatically reflect poorly on their scientific work.

Chinese scientists are known to rely on third-party agencies that provide language editing services, which give the papers a polish, increasing the chance of getting accepted. But it’s possible those companies have also done the authors a massive disservice.

“There is some evidence that so-called third-party language-editing services play a role in manipulating the reviewing process,” an unnamed Springer spokesperson told Cathleen O’Grady at Ars Technica.

While we don’t have details on whether any of the authors had a hand in contributing fake reviews, experts are willing to chalk at least some of the breaches up to those third-party companies, some of which are known to operate unethically.

“If the authors didn’t realise that this is what the editing company was doing, then I feel the authors should have a fair chance,” Elizabeth Wager, editor of the journal Research Integrity & Peer Reviewtold Ars Technica.

“There’s probably nothing wrong with the research; it just hasn’t been peer reviewed.”

China is one of the biggest scientific contributors in the world, producing more than 300,000 papers every year. With strides in nuclear fusion and revolutionary CRISPR experiments, Chinese researchers are major players in the international research scene.

But any large industry gets its share of scandals. For example, just last year news broke that 80 percent of data in Chinese clinical trials had been fabricated.

As for Tumor Biology, the journal actually moved from Springer to SAGE late last year, and the new publisher was made aware of the investigation into potential peer review fraud. The journal is run by the International Society of Oncology and BioMarkers.

“The society were open about the past instances of peer review fraud, and as part of the relaunch they wanted to address the underlying reasons,” a SAGE spokesperson told Alison McCook at Retraction Watch.

“As part of their transition to a new publisher, the Tumor Biology editorial team have already introduced new robust peer review practices expected from all SAGE journals.”

Source: journalgazett.com


A molecular dance of phospholipid synthesis

The most abundant molecule in cell membranes is the lipid phosphatidylcholine (PC, commonly known as lecithin); accordingly, the enzymes responsible for synthesizing it are essential. Research published in the May 4 issue of the Journal of Biological Chemistry used computer simulations to gain insights into how one of these enzymes activates and shuts off PC production. These results could help researchers understand why small changes in this enzyme can lead to conditions like blindness and dwarfism.

Rosemary Cornell, a professor of molecular biology and biochemistry at Simon Fraser University in Canada, studies the  CTP:phosphocholine cytidylyltransferase, or CCT. CCT sets the rate of PC production in cells by binding to cell membranes with low PC content. When bound to membranes, the CCT enzyme changes shape in a way that allows it to carry out the key rate-limiting step in PC synthesis. When the amount of PC making up the  increases, the CCT falls off the membrane, and PC production ceases.

“The membrane is this big macromolecular array with lots of different molecules in it,” Cornell said. “How does this enzyme recognize that ‘Oh, I should slow down because the PC content of the membrane is getting too high?'”

Cornell and her project team – a collaboration with Peter Tieleman and graduate student, Mohsen Ramezanpour at the University of Calgary and Jaeyong Lee and Svetla Taneva, research associates at SFU – thought that the answer must have to do with the dynamic changes in shape that the enzyme undergoes when it binds to a membrane. But these changes are difficult to capture with traditional structural biology methods like x-ray crystallography, which take a static snapshot of molecules. Instead, the team used computational simulations of , which use information about the forces between every individual atom in a molecule to calculate the trajectories of the enzyme’s moving parts.

“What it looks like (when you visualize the output) is your big molecule dancing in front of your eyes,” Cornell said. “We set up the molecular dynamics simulation not once, not twice, but 40 different (times). It took months and months just to do the computational parts and even more months trying to analyze the data afterward. We actually spent a lot of time once we got the data just looking on the screen at these dancing .”

The simulated dance of the CCT molecule showed that when the M-domain, the section of the enzyme that typically binds to the membrane, detaches from a membrane, it snags the active site of the enzyme, preventing it from carrying out its reaction. When the snagging segment was removed from the simulation, the team saw a dramatic bending motion in the docking site for the snagging element, and speculated that this bending would create a better enzyme active site for catalyzing the reaction when attached to a membrane. The team confirmed these mechanisms using biochemical laboratory experiments.

Interestingly, previous genetic studies had shown that mutations in the gene encoding CCT are responsible for rare conditions like spondylometaphyseal dysplasia with cone-rod dystrophy, which causes severe impairments in bone growth and vision, but it was unknown how these changes in the enzyme could lead to such dramatic consequences. Cornell hopes that understanding how the enzyme works could help researchers find out.

“If you have just one small change in CCT, then how is that going to make this whole process of synthesizing PC defective?” Cornell asks. “That’s what we’re studying right now.”

 Explore further: Flipping lipids for cell transport-tubules

More information: Mohsen Ramezanpour et al, An auto-inhibitory helix in CTP:phosphocholine cytidylyltransferase hijacks the catalytic residue and constrains a pliable, domain-bridging helix pair, Journal of Biological Chemistry (2018). DOI: 10.1074/jbc.RA118.002053

Read more at: Phys.org

Chemical Engineers Reveal How to Control Knots That Form in DNA Molecules

Just like any long polymer chain, DNA tends to form knots. Using technology that allows them to stretch DNA molecules and image the behavior of these knots, MIT researchers have discovered, for the first time, the factors that determine whether a knot moves along the strand or “jams” in place.

“People who study polymer physics have suggested that knots might be able to jam, but there haven’t been good model systems to test it,” says Patrick Doyle, the Robert T. Haslam Professor of Chemical Engineering and the senior author of the study. “We showed the same knot could go from being jammed to being mobile along the same molecule. You change conditions and it suddenly stops, and then change them again and it suddenly moves.”

The findings could help researchers develop ways to untie DNA knots, which would help improve the accuracy of some genome sequencing technologies, or to promote knot formation. Inducing knot formation could enhance some types of sequencing by slowing down the DNA molecules’ passage through the system, the researchers say.

MIT postdoc Alexander Klotz is the first author of the paper, which appears in the May 3 issue of Physical Review Letters.

Engineers Control Knots That Form in DNA Molecules

A knot near the end of a stretched DNA molecule is driven toward the end and unties, leaving an unknotted molecule. (Image: Alex Klotz)

Knots in motion

Doyle and his students have been studying the physics of polymer knots such as DNA for many years. DNA is well-suited for such studies because it is a relatively large molecule, making it simple to image with a microscope, and it can be easily induced to form knots.

“We have a mechanism that causes DNA molecules to collapse into a tiny ball, which when we stretch out contains very big knots,” Klotz says. “It’s like sticking your headphones in your pocket and pulling them out full of knots.”

Once the knots form, the researchers can study them using a special microfluidic system that they designed. The channel is shaped like a T, with an electric field that diverges at the top of the T. A DNA molecule located at the top of the T will be pulled equally toward each arm, forcing it to stay in place.

The MIT team found that they could manipulate knots in these pinned DNA molecules by varying the strength of the electric field. When the field is weak, knots tend to move along the molecule toward the closer end. When they reach the end, they unravel.

“When the tension isn’t too strong, they look like they’re moving around randomly. But if you watch them for long enough, they tend to move in one direction, toward the closer end of the molecule,” Klotz says.

When the field is stronger, forcing the DNA to fully stretch out, the knots become jammed in place. This phenomenon is similar to what happens to a knot in a bead necklace as the necklace is pulled more tightly, the researchers say. When the necklace is slack, a knot can move along it, but when it is pulled taut, the beads of the necklace come closer together and the knot gets stuck.

“When you tighten the knot by stretching the DNA molecule more, it brings the strands closer to each other, and this ramps up the friction,” Klotz says. “That can overwhelm the driving force caused by the electric field.”

Dmitrii Makarov, a professor of chemistry at the University of Texas at Austin, who was not involved in the study, describes it as “an elegant experimental demonstration that knots in DNA can ‘jam’ under tension, just like macroscopic knots do in our everyday experience. This work also provides important fundamental insights into friction on molecular scale, a phenomenon that is still poorly understood.”

Knot removal

DNA knots also occur in living cells, but cells have specialized enzymes called topoisomerases that can untangle such knots. The MIT team’s findings suggest a possible way to remove knots from DNA outside of cells relatively easily by applying an electric field until the knots travel all the way to the end of the molecule.

This could be useful for a type of DNA sequencing known as nanochannel mapping, which involves stretching DNA along a narrow tube and measuring the distance between two genetic sequences. This technique is used to reveal large-scale genome changes such as gene duplication or genes moving from one chromosome to another, but knots in the DNA can make it harder to get accurate data.

For another type of DNA sequencing known as nanopore sequencing, it could be beneficial to induce knots in DNA because the knots make the molecules slow down as they travel through the sequencer. This could help researchers get more accurate sequence information.

Using this approach to remove knots from other types of polymers such as those used to make plastics could also be useful, because knots can weaken materials.

The researchers are now studying other phenomena related to knots, including the process of untying more complex knots than those they studied in this paper, as well as the interactions between two knots in a molecule.

The research was funded by the National Science Foundation and the National Research Foundation Singapore through the Singapore MIT Alliance for Research and Technology.

Publication: Alexander R. Klotz, et al., “Motion of Knots in DNA Stretched by Elongational Fields,” Phys. Rev. Lett. 120, 188003, 2018; doi:10.1103/PhysRevLett.120.188003

Source: scitechdaily.com

Archaeologists Have Found a Mysterious Bloody Massacre From 5th Century Sweden

Around 1,500 years ago, perhaps around 450 CE, unknown raiders stormed the small, prosperous village of Sandby borg on the shore of Öland island, and slaughtered the inhabitants, leaving the bodies where they fell.

Now, archaeologists in Sweden have stumbled upon this grisly mystery. With less than 7 percent of the site excavated, the research team, led by archaeologists Clara Alfsdotter, Ludvig Papmehl-Dufay and Helena Victor, has already found the remains of at least 26 bodies.

It doesn’t look like much now – just a grassy green mound ringed by an oval of rock, but it was once a thriving settlement.

The village was inside a ringfort not far from the shoreline, containing 50 or so homes circled by walls that stood 4 to 5 metres (13 to 16 feet) high. Around 200 to 250 people would have lived there.

At the time, the European Migration Period was underway, and it was an unstable, tumultuous time; but who killed the villagers and why remains a mystery nonetheless.

sandby borg layoutThe layout of Sandby borg. (Alfsdotter et al./Antiquity)

The dig team has only excavated three of the homes – but what they have found is deeply moving. The bodies exhibit signs of blunt force trauma, or supine positions that indicate they died suddenly, or were unconscious prior to death.

The remains of a five-year-old child and an infant just a few months old were also found, and two skeletons were partially charred – in a manner that indicates that the soft tissue was still present. Possibly they fell into fires, or a fire was started – either accidentally or on purpose.

One skeleton (pictured at the top of this article), of an adolescent no older than 15, had its feet resting on the abdomen of another skeleton, as though the young person had tripped, or fallen backwards over another body, never to get up again.

Bodies were also found in the streets, along with the remains of dogs and livestock, which could have starved to death, or also been killed in the attack. One house contained nine sets of human remains.

Historically, the people of the area cremated their dead. It all points to absolute carnage.

“You don’t find people lying around in houses,” Victor told the BBC. “[People] don’t do it today, and didn’t do it then.”

sandby borg broochesFive gilt brooches recovered from Sandby borg. (Alfsdotter et al./Antiquity)

Even more curious: the site is abundant with treasure. Gold coins, glass beads, gilded brooches, rings and silver pendants of high quality were found scattered. Everything except weapons.

Whoever sacked the Sandby borg village didn’t loot the site – except, perhaps, for potential weapons, which may have been taken as a trophy or tribute to the gods. It’s unknown whether the residents defended themselves – but it seems like they didn’t, the researchers said.

“Damage resembling common battle injuries, such as parry fractures or facial trauma, both typically produced when facing an opponent, has so far not been identified,” they wrote in their paper.

“This pattern leads us to conclude that the perpetrators comprised a large number of people, striking simultaneously in several houses, and that several of the victims were not in a position to defend themselves.”

Although the island at the time was populated by around 15 other ringfort villages, no one ever visited the site to loot the homes or inter the bodies. They remained where they fell, the village abandoned, until the roofs collapsed and the macabre scene was buried by time.

sandby borg siteSnadby borg prior to the excavations. (Kalmar County Museum)

Even to this day, whispers remain, although there’s no record, either written or oral, of the massacre. Local people, the researchers said, warned them to stay away from the site, vaguely inferring it was dangerous.

“I do find it most likely that the event was remembered and that it triggered strong taboos connected to the site, possibly brought on through oral history for centuries,” Papmehl-Dufay said.

The local Kalmar County Museum is featuring an exhibition of the excavation, and work on the site continues.

A paper detailing the team’s work so far can be read in the journal Antiquity.