Fossil biomolecules from an endogenous source were previously identified in Cretaceous to Pleistocene fossilized bones, the evidence coming from molecular analyses. These findings, however, were called into question and an alternative hypothesis of the invasion of the bone by bacterial biofilm was proposed. Herewith we report a new finding of morphologically preserved blood-vessel-like structures enclosing organic molecules preserved in iron-oxide-mineralized vessel walls from the cortical region of nothosaurid and tanystropheid (aquatic and terrestrial diapsid reptiles) bones. These findings are from the Early/Middle Triassic boundary (Upper Roetian/Lowermost Muschelkalk) strata of Upper Silesia, Poland. Multiple spectroscopic analyses (FTIR, ToF-SIMS, and XPS) of the extracted "blood vessels" showed the presence of organic compounds, including fragments of various amino acids such as hydroxyproline and hydroxylysine as well as amides, that may suggest the presence of collagen protein residues. Because these amino acids are absent from most proteins other than collagen, we infer that the proteinaceous molecules may originate from endogenous collagen. The preservation of molecular signals of proteins within the "blood vessels" was most likely made possible through the process of early diagenetic iron oxide mineralization. This discovery provides the oldest evidence of in situ preservation of complex organic molecules in vertebrate remains in a marine environment.
Citation: Surmik D, Boczarowski A, Balin K, Dulski M, Szade J, Kremer B, et al. (2016) Spectroscopic Studies on Organic Matter from Triassic Reptile Bones, Upper Silesia, Poland. PLoS ONE 11(3): e0151143. doi:10.1371/journal.pone.0151143
Editor: Steffen Kiel, Naturhistoriska riksmuseet, SWEDEN
Received: October 8, 2015; Accepted: February 24, 2016; Published: March 15, 2016
Copyright: © 2016 Surmik et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: All relevant data are within the paper and its Supporting Information files.
Funding: This research project is supported by National Science Center (www.ncn.gov.pl) grant no. 2011/01/N/ST10/06989.
Competing interests: The authors have declared that no competing interests exist.
The conventional wisdom states that no original organic components remains associated with Mesozoic vertebrate bones over geological time. It is based on models using unrealistically harsh chemical conditions as proxies for time . However, half a century ago, one of us (RP) was the first to demonstrate, by describing fossilized cells, collagen fibrils and vessels from Cretaceous dinosaur bones from the Gobi Desert , that this conventional wisdom may not hold for all fossils. Beginning in the 1970s, Pawlicki documented histochemical reactions of glycosaminoglycans , lipids , and nucleic acids  in dinosaur bones. Later, various amino acids were extracted from 150 Ma old sauropod bones by Gurley et al. . Muyzer et al.  identified remains of osteocalcin, non-collagenous bone matrix protein in dinosaurs, using radioimmunological assays. Recently, Schweitzer and her colleagues, following up on these early investigations, identified soft tissues in dinosaur bones consistent with collagenous matrices, bone cells (osteocytes), blood vessels, and intravascular contents high in iron. The morphological studies were supported by in situ immunological assays and MS/MS sequence data that identified proteins consistent with a vertebrate origin [8–15]. Reports of preserved organic compounds in dinosaurs have been criticized due to the possible presence of bacterial biofilms  and other forms of contamination as a potential source of organic matter (compare in ). However, the recovery of both sequences for, and antibody binding to, histone proteins eliminates a microbial source .
Molecular taphonomy, a branch of modern vertebrate paleobiology, addresses alterations of molecules in natural environments over geological time scales. This emergent discipline has been made possible by the advent of highly sensitive and accurate high-resolution analytical methods, including spectroscopy and mass spectrometry. These methods have been employed to support the hypothesis that complex organic molecules can survive, under certain conditions, over long periods of time. However, interpretation of data from a single method is not conclusive. For example, amide signals recovered by synchrotron radiation Fourier transform infrared spectroscopy (SR-FTIR) in fast-growing embryonic bones of Early Jurassic dinosaurs in China  may suggest the preservation of bone proteins. However, according to one of the authors, the spectra interpreted as amide may have been misconstrued [K. Stein, personal communication]. Protein remains were detected from the femur of a Cretaceous mosasaur from Belgium using various methods . Time of Flight Secondary Ion Mass Spectrometry (ToF-SIMS) was used successfully to identify amino acid residues [9, 10], [20–22], heme-derived compounds [22, 23] and melanin pigment [24, 25].
This paper summarizes the results of research on molecules which may indicate a proteinaceous source associated with goethite particles extracted from the bones of Early/Middle Triassic reptiles in southern Poland. The Triassic bones had not been studied previously for potential preservation of organic molecules. During such a long deposition the bones were subjected to various diagenetic processes, most of which negatively affected their preservation. However, diagenetic processes not always have to remove organic signals from bones completely. It has been observed that relatively early mineralization can protect delicate organic material from complete degradation [26, 27]. Minerals that nucleate directly on organic material block or limit the accessibility of enzymes involved in degradation. Thus, microcrystalline minerals deposited on an organic template may form a mineral “cast”, stabilizing the molecules and providing added resistance to long-term biological and physical degradation. Other factors, such as bone structure and the thickness and geochemical properties of sediment, play a crucial role in the preservation of organic matter. Therefore, even in the case of very old bones, original organic molecules can be preserved.
The bone samples are from fossiliferous beds at the boundary of the uppermost part of the Röt (Myophoria Beds)  and the lowermost part of the Lower Muschelkalk, known also as the Limestone with Entolium and Dadocrinus Unit (Lower Gogolin Formation, see also ). These bone-bearing limestones occur in Gogolin and Żyglin in Upper Silesia, southern Poland (S1 Fig). The age of the Gogolin Formation (formerly Gogolin Beds), as specified on the basis of lithostratigraphic , biostratigraphic  and more recent magnetostratigraphic [32, 33] data, has been dated as Early/Middle Triassic, 247.2 Ma (an absolute age, according to the IUGS International Chronostratigraphic Chart v. 2015/01, http://www.stratigraphy.org). Paleomagnetic studies date the Myophoria Beds and the first 5 m of the Limestone with Entolium and Dadocrinus Unit as Olenekian in age . The sediments were deposited on a carbonate platform situated in the southern part of a shallow epicontinental sea [34, 35].
Material and Methods
The samples of Nothosaurus sp. (Sauropterygia) bones (humerus, WNoZ/s/7/166; femur SUT-MG/F/Tvert/15) and the Protanystropheus sp. (Archosauromorpha) vertebral centrum (SUT-MG/F/Tvert/2) derive from the fossiliferous beds of the Limestone with Entolium and Dadocrinus Unit, the lowest part of the Gogolin Formation.
The vertebral centrum of Protanystropheus (SUT-MG/F/Tvert/2) and the nothosaur femur (SUT-MG/F/Tvert/15), are from the historical collection of the Catholic priest Eduard Kleemann, and are now deposited in the Museum of Geological Deposits, Faculty of Mining and Geology, Silesian University of Technology, Gliwice, Poland. Triassic vertebrate fossils were collected by Father Kleemann at the turn of the 19th and 20th centuries. The specimens SUT-MG/F/Tvert/2 and SUT-MG/F/Tvert/15 are labeled “Gogolin,” indicating the town of Gogolin, near Opole (Opole Voivodeship, Krapkowice County), as the fossils’ locality.
The humerus (WNoZ/s/7/166) is from the Entolium and Dadocrinus Unit in the Żyglin quarry in the town of Miasteczko Śląskie, near Tarnowskie Góry (Silesian Voivodeship). All permission required for collecting fossils in the Żyglin quarry was obtained through an agreement with the Regional Directorate for Environmental Protection in Katowice. The specimen is now deposited in the Museum of Earth Science, Faculty of Earth Science, University of Silesia, Sosnowiec, Poland.
A recent marine iguana femur (GIUS-12-3628), used in our study as a reference sample, is now kept at the Department of Paleontology and Stratigraphy, Faculty of Earth Sciences, University of Silesia. This femur belonged to an individual Galapagos marine iguana that died from natural causes, and was collected as an isolated element with the permission of the appropriate local authorities. All of these specimens are publicly deposited and accessible to others in permanent repositories.
Marine nothosaurs from the Early/Middle Triassic boundary of Southern Poland are usually preserved as isolated bones and represented mainly by medium-size species. Most likely they are represented by Nothosaurus cf. marchicus (according to personal observations by DS; see also ). Terrestrial tanystropheids, represented by Protanystropheus antiquus, lived and fed in intertidal zones (compare in ). The occurrence of these animals is relatively early in the European Basin (compare in [38–41]; personal observation by DS).
The bone samples of Triassic reptiles were analyzed in terms of preservation of organic matter residues because preliminary morphological studies (light microscopy and ESEM) revealed the occurrence of vessel-like structures in the cortical part of bone in several samples (Fig 1). The densest areas of cortical (compact) bone of the samples (Fig 2) were chosen for analysis in order to minimalize the risk of microbial contamination from the medullar cavity and from outside. The analyses of “blood vessels” were performed on a partially demineralized (phosphate phase removed) fragment of the Nothosaurus humerus and a thin section from a massive cortical part of the Protanystropheus cervical vertebra. After these morphological studies, the mineralogical composition of fossil bones was examined using X-ray diffraction (XRD) and subjected to detailed elemental study using an electron dispersive spectrometer (EDS) microanalyzer coupled with ESEM. In the next step, X-ray photoelectron spectroscopy (XPS), infrared spectroscopy (FTIR) and mass spectrometry (ToF-SIMS) techniques were applied to determine types of chemical bonds and to identify iron-mineralized organic matter within fossilized “bones vessels”.
Stereoscopic and ESEM microscope images of blood vessels: a) partially demineralized bone sample from the near-cortical region shows parallel-oriented fossilized blood vessels (SUT-MG/F/Tvert/2 sample) in stereoscopic microscope image; b) fossilized “floating” blood vessels from sample SUT-MG/F/Tvert/2 during the demineralization (decalcification) process in EDTA solution in stereoscopic microscope image; c) ESEM image of bifurcated blood vessels mounted on a carbon conductive tab (WNoZ/s/7/166 sample); d-f) isolated branch-like-shaped blood vessels (WNoZ/s/7/166 sample) in stereoscopic microscope images; g) ESEM image of fossilized blood vessel mounted on carbon conductive tab; h) ESEM images of magnified fragment of a mineralized blood vessel with preserved tubular morphology from a demineralized part of bone from specimen WNoZ/s/7/166; i) ESEM image of heavily mineralized, damaged walls of a blood vessel (SUT-MG/F/Tvert/2) with nodular-form goethite crystals, mounted on a carbon conductive tab.
a) Silhouette of Protanystropheus vertebra (SUT-MG/F/Tvert/2 sample) with an indication of the sectioning area; b) silhouette of Nothosaurus humerus (WNoZ/s/7/166 sample) with an indication of sampling; c) an idealized schematic cross section of bone with a sampling area within dense, cortical bone tissue.
All of the studied specimens possess a documented storage history and have never been glued or treated with any contemporary organic-based materials. The outermost surface contaminants were removed prior to the analyses and the samples were rinsed several times according to the protocols presented herein. All studied fossil bones, as well as control samples, were purified by means of incubation in methanol solution (Methanol:Dichloromethane, CH4O:CH2Cl2, 1:1, Sigma-Aldrich, USA) to remove surface contaminants and rinsed several times with deionized water.
Three types of preparation were performed: (1) powdering, (2) thin sectioning, (3) demineralization.
Fragments of compact bone obtained from the cortical region in the middle shaft of the Nothosaurus humerus and Protanystropheus vertebral centrum were triturated to an analytical fraction (5‒10μm) in an agate mortar for X-ray powder diffraction and FTIR analysis. A recent control sample of a marine iguana femur was frozen in liquid nitrogen (LN, ‒195.8°C), and then triturated to XRD and FTIR analyses.
The analyses were performed on covered and uncovered (polished) thin sections about 30 μm thick. Bone fragments were embedded in Araldite 2020 epoxy resin (Huntsman Advanced Materials, USA). The thin sections were polished with silicon carbide (SiC) and aluminum oxide (Al2O3) papers. Then, the surface was cleaned using diamond paste. Additionally, prior to each analysis, the thin-section surface was cleaned with isopropyl alcohol, 99.9% pure (Sigma-Aldrich, USA), to remove the outermost contaminants.
A small bone fragment of sample WNoZ/s/7/166 (46.1 mg) was mounted on the top of a vacuum filtration kit (Sartorius AG, Germany) on a sterile Whatman Anodisc 0.02-μm aluminum oxide (Al2O3) membrane filter (Anopore Inorganic Membranes, GE Healthcare Life Science, USA). The samples were incubated in 0.5M EDTA agent (pH 8.0, filtered by a 0.45-μm Millipore sterile membrane, Merck Millipore, Germany) at room temperature, with two changes of EDTA dilution per day, and rinsed in ultra-pure deionized water with conductivity of 0.05 μS/cm (Elix Essential Water Purification System, Merck Millipore, Germany) several times to remove contaminants. The EDTA dilution and deionized water were removed by manual vacuum pump filtration (PHYWE Systeme GmbH und Co. KG, Germany). We excluded disodium ethylenediaminetetraacetic agent (EDTA) as a source of amino acids by comparing FTIR spectra of pure EDTA salts with sample spectra (S2 Fig).
A residuum containing vessel-like as well as bone-cell-like structures and amorphous reddish-brown mineral material were dried in a vacuum desiccator under sterile conditions at room temperature. Some of the isolated”blood vessels” were manually picked up and separated from the residuum, mounted on carbon conductive tabs to be analyzed in ESEM with and without coating. Another portion of the sample was powdered for XRD and FTIR analyses. The remaining portion of the sample was mounted on a molybdenum holder and placed in a high-vacuum chamber for chemical analysis using ToF-SIMS and XPS.
Optical measurements were carried out using an Olympus BX51 polarizing microscope equipped with an Olympus SC30 camera and a halogen light source, both installed at the Department of Geochemistry, Mineralogy and Petrography, University of Silesia. Optical micrographs were collected using Cell^A 5.1 software (Olympus Soft Imaging Solutions GmbH) using a UMPlanFI 10× objective and an aperture of 0.30.
Environmental Scanning Electron Microscopy (ESEM)
ESEM images were performed on a Philips XL30 ESEM/EDAX, installed at the Laboratory of Scanning Electron Microscopy, Faculty of Earth Science, University of Silesia, and equipped with an EDAX Sapphire energy-dispersive X-ray spectroscope to analyze the morphology and chemical composition of isolated fossilized “vessels”. The measurements were done on gold-coated bone residuum (high vacuum, accelerated voltage 15 kV) and uncoated thin sections (low vacuum, acc. voltage 15 kV).
X-ray Diffraction (XRD)
X-ray diffraction analyses (XRD) were undertaken to investigate bone mineral content. We used a PANalytical X'Pert PRO MPD PW 3040/60 diffractometer at the Laboratory of X-ray Diffraction, Faculty of Earth Science, University of Silesia. Quantitative phase content and crystallographic parameters were calculated using the Rietveld Module in HighScore Plus software with the ICDD PDF-4+ pattern database. X-ray diffraction analysis was performed for powdered bone samples as well as for powdered extracted fossilized “blood vessels”. The powder was placed in a reflection-free silicon base in the analyzed area and mounted in a sample changer. The measurements were carried out using the following parameters: source of radiation, Cu Kα1 (λ = 1.540598 Å); nickel filter, 0.02 mm; voltage, 45 kV; current, 30 mA; scan range, 2.5‒80° 2Θ; step size, 0.01° 2Θ; counting time, 600 s; detector, X'Celerator; analysis time, 6 h.
Infrared Spectroscopy (FTIR)
Infrared spectroscopy (FTIR) was performed using an Agilent Cary 660 FTIR spectrometer equipped with a standard source and a DTGS Peltier-cooled detector installed at the Department of Biophysics and Molecular Physics, Institute of Physics, University of Silesia. All spectra were accumulated with a spectral resolution of 4 cm-1 and recorded by accumulating 16 scans. The baseline correction and fitting analysis by Voigt function for each spectrum were performed using the GRAMS software package. The spectra were collected using a GladiATR diamond accessory (Pike Technologies) in the 4000–400 cm-1 range.
Time of Flight Secondary Ion Mass Spectrometry (ToF-SIMS)
ToF-SIMS experiments were performed using a ToF-SIMS 5 (IONTOF GmbH, Münster, Germany) reflectron-type spectrometer equipped with a bismuth liquid metal ion gun (Bi+ and Bi3++ primary beams) installed at the Department of Solid State Physics, Institute of Physics, University of Silesia. The measurements were performed at room temperature in ultrahigh vacuum conditions (~2‒5∙10−9 mbar). High-resolution mass spectra were obtained using a focused high-energy primary ion beam (pulsed 30 keV Bi+ or Bi3++ ions at an ion current of ~1pA and 0.1pA, respectively) aimed at the sample surface at an angle of 45° relative to the surface normal, causing emission of secondary ions. Because structurally different molecules may have almost identical masses, all measurements were performed at high mass resolution mode, given herein an accuracy of 0.01 Da. Positive and negative secondary ion spectra and distribution maps for selected ions were collected by rastering the bismuth ion beam across the regions of interest with an m/z range of 1‒800 Da. The size of the areas analyzed varied from 50×50 to 500×500 μm, depending on the region of interest. The mass spectra were internally calibrated using CH3+, C2H3+, C2H5+, C3H7+, and C4H9+ ions for measurements performed for positive polarity and C-, CH-, C2-, C2H-, C3-, and C3H- ions for negative polarity. Line broadening and thus reduction of mass resolution m/Δm appeared as a result of sample morphology and surface charging. The surfaces of the analyzed samples were neutralized with the use of an electron flood gun. Nevertheless, mass resolution varied depending on polarity or/and sample morphology at the level of 5,000‒9,000. To avoid the impact of contamination, the analyses were performed on surfaces cleaned in the vacuum chamber with the use of a cesium ion gun (Cs at 2 keV and 100 nA rastered over an area typically several times larger than the region of interest; the estimated depth of the removed surface was about 2 μm). Although etching the sample surface with the cesium gun may cause fragmentation of primary molecules present in the specimens, removal of surface contamination was deemed justified. Analysis of the ToF-SIMS spectra, for both negative and positive polarity, enabled the identification of several dozen organic secondary ion species. A number of peaks which, by definition, are organic in nature (showing a mass excess) may be assigned to the secondary ion species typically observed in amino acid mass spectra (see Results). The absence of all molecular peaks in the mass spectrum for a particular amino acid may result from Cs etching, the performance of the ToF-SIMS measurements above the static limit, or significant degradation of the organic molecules in the analyzed specimens. Nevertheless, the presence of amino-acid-related fragment ions was confirmed for both specimens in both polarities, and a number of characteristic peaks showing a mass excess were assignable to the secondary ion species of specific amino acids (see Results). Moreover, taking into account the sample preparation, specifically Cs etching, it was determined that the detected secondary ion originated from the surface of the specimens, not from surface contamination. The analysis of the high mass resolution secondary ion mass spectra, together with the distribution maps of selected secondary ions, enabled the unambiguous determination of ion location in the analyzed area.
High lateral resolution maps of ion distribution were obtained by applying the Fast Imaging Mode of the ToF-SIMS spectrometer. In this mode the mass resolution is significantly lowered (m/Δm ~100), which in practice means an inability to determine the presence of particular molecular ion species and/or to distinguish distributions of molecular ions with closely adjacent masses. However, since we performed measurements from the same areas in high mass resolution and high lateral resolution modes we may ascribe particular ions distribution maps to particular ion. We assumed that, since the peak indicating the presence of an ion assigned to a particular amino acid is characterized by the dominant intensity in high mass resolution mode, the related peak obtained from measurements in high lateral resolution mode would also be dominated by the presence of that ion. Hence the distribution maps for particular masses presented in Fig 3 are related to particular amino acid fragments.
ESEM images and ToF-SIMS fast imaging mode mapping of blood vessels sections displaying their tubular structure. a) ESEM image of thin section showing fossilized blood vessels; analyzed area marked by rectangle. b) the same thin section in optical microscopy; analyzed area marked. c) blood vessel in SEM image, enlarged part of Fig 3a shows location of ToF-SIMS mapping; d‒j) ToF-SIMS ion distribution maps generated for the selected masses corresponding to iron (55.86 Da) and amino acid ions: 30.03 Da–CH4N+ (glycine or proline), 44.05 Da–C2H6N+ (alanine), 70.07 Da–C4H8N+ (proline), 86.06 Da–C4H8NO+ (hydroxyproline), 84.08 Da–C5H10N+ (lysine) and total ion image (Fig 3j) in positive polarity. The distribution of iron (Fig 3d) within the vessel section overlaps with the distribution of ions.
X-Ray Photoelectron Spectroscopy (XPS)
X-ray Photoelectron Spectroscopy (XPS) was performed using an XPS PHI 5700 spectrometer from Physical Electronics, Inc., equipped with a monochromatized X-ray source, installed at the Department of the Solid State Physics, Institute of Physics, University of Silesia. The samples were cleaned in situ in an ultra-high vacuum by etching with an Ar-ion beam with an energy of 2 keV. This enabled the removal of surface contamination originating from sample preparation and storage. The region of interest focused on isolated “blood vessels” about 200×800 μm in size.
Results of Multiproxy Studies
”Vessels” Morphology and Microstructures
The “blood vessels” derived from the internal part of cortical bone from specimens WNoZ/s/7/166 and SUT-MG/F/Tvert/2 (Fig 1). The demineralized bone fragment revealed parallel-oriented “vessels” (fragments up to 2 mm long and about 50–100 μm wide) that bifurcate in some areas (Fig 1C–1G). They are preserved as reddish brown or yellow-orange, translucent, tube-like and branch-like floating structures (Fig 1A–1G). The vessels are mineralized with tiny crystals (1‒5μm, Fig 1I) of iron oxide, forming a coating that precisely mimics their external shape (Fig 1C–1H).
- ∎. The most intense ion signals from amino acid fragments of proline, hydroxyproline and leucine and others, Fig 3E–3I; were obtained from the vascular lumina of the blood vessels;
- ∎. The Fe+ ions and amino acids fragments overlap (compare distribution of ions on Fig 3D–3I);
- ∎. The most intense signals of iron derived from the outermost part of each of the studied “blood vessels”. Additionally, ion mapping indicated that iron ions seemed to be “scattered”, creating a form of an “agglutination” or “cloud” surrounding the vessel lumen (Fig 3D).
X-ray analyses revealed that powdered fossil bone samples (WNoZ/s/7/166, SUT-MG/F/Tvert/2) containing ferruginous layers are made mainly of fluoroapatite (95.3‒95.4%), and thus are typical diagenetically-altered fossil bones (Fig 4A). An admixture of goethite from 0.5 to 1.0 for both samples, as well as hematite (1%), was found in the SUT-MG/F/Tvert/2 sample. Isolated by EDTA incubation, powdered”blood vessels” from the WNoZ/s/7/166 sample (nothosaur humerus) showed the presence of only one crystalline phase: goethite (Fig 4B). XRD data from the recent control sample (marine iguana) indicated the presence of hydroxyapatite, a typical substance characterizing fresh, non-altered bones (S3 Fig).
a) Isolated blood vessels from sample WNoZ/s/7/166 and b) a fragment of cortical bone WNoZ/s/7/166. The bone consists mainly of fluoroapatite (95.4%), calcite (4.1%), and goethite (0.5%); however, in the case of isolated vessels, the crystalline phase of goethite occurred. FAp, fluoroapatite; C, calcite; Gt, goethite.
The infrared spectra of fossil bone fragments (WNoZ/s/7/166, SUT-MG/F/Tvert/2, SUT-MG/F/Tvert/15) and recent marine iguana bone (GIUS-12-3628) are dominated by typical phosphate and carbonate attributed to fluorapatite (Fig 5A–5D) [42, 43]. In greater detail:
- ∎. the bands in the 1200‒950 cm-1 range are linked to anti-symmetric (ν3) and symmetric (ν1) stretching vibrations of (PO4)3-, whereas at lower wavenumbers, from 650 to 530 cm-1, out-of-plane (ν2) and in-plane (ν4) bending vibrations of phosphate units can be found.
- ∎. anti-symmetric (ν3) and symmetric (ν1) stretching vibrations of the carbonate (CO3)2- ion are observed in the 1550‒1250 cm-1 range. Infrared bands in the 880‒750 cm-1 region originate from out-of-plane (ν2) and in-plane (ν4) bending vibrations of carbonate groups.
Peak fit analysis based on the FTIR measurements for recent (a) and fossil bones (b‒d); pure carbonate (e); and two samples of fossilized blood vessels of WNoZ/s/7/166 (f and g). Each cortical bone (a‒d) shows an apatite (PO4)3- as well as a carbonate (CO3)2- peak, while both samples of WNoZ/s/7/166 infrared spectrum reveal a goethite (OH)- and (FeO4)5- peak. a) The primary cortical bone of a marine iguana femur shows amide bands at 1700‒1500 cm-1; b) and c) fossil bones of WNoZ/s/7/166 and SUT-MG/F/Tvert/2 reveal an amide peak at 1650‒1550 cm-1; d) the lack of amide components as detected in the nothosaur femur (SUT-MG/F/Tvert/15) bone; e) a sediment control sample from the vicinity of bone WNoZ/s/7/166; f) and g) isolated fossilized blood vessels show amide peaks at 1670‒1600 cm-1 and at 1450‒1200 cm-1. The other peaks come from amino acid residues and lipid structures.
On the infrared spectra of “blood vessels” (WNoZ/s/7/166), bands in the region of 950‒750 cm-1 (OH modes) as well as below 650 cm-1 (vibration of ν(FeO)45-) have been ascribed to the goethite phase (Fig 5F and 5G) [44, 45].
The other bands in the range from 1800 to 1100 cm-1 (fossilized bone material), as well as between 1650‒950 and 650‒550 cm-1, are assigned to organic material remains , [46, 47]. A more detailed analysis of organic regions (especially using the deconvolution process) enabled location and separation of the signals from amide, lipids, other organic remains, and phosphate and carbonate units. In general, the amide signal is associated with bands in the ranges of 3400–3030 cm-1, 1670–1200 and 650–550 cm-1 , while the presence of amino acid side chains and lipids are well marked over a wide wavenumber range from 1750 to 750 cm-1 [48–52]. The very weak signal/noise ratio in the case of bands ranging from 3500‒2800 cm-1 is difficult to interpret (see S4 Fig) and at the same time unambiguously due to overlapping of the hydroxyl group, molecular water and amide ones vibration (see S4 Fig). Hence, the infrared data imply that bands from the 3310‒3270 cm-1 region might be evidence of the NH stretching vibration coupled with the hydrogen bond of a carbonyl group in amide A, whereas infrared features ranging from 3100‒3030 cm-1 are associated with the NH stretching vibration of amide B, especially in case of sample WNoZ/s/7/166 (S4F and S4G Fig). Moreover, according to the literature, below 3000 cm-1 very weak bands might be related to the asymmetrical stretching mode of CH3 and CH2 groups in the case of lipids as well as NH3+ units linked to low molecular weight peptides or other organic residues . Hence, our analysis was focused on data where signals from typical amide, amino acid and lipid regions are more clearly visible, i.e., below 1800 cm-1.
On the infrared spectrum of recent marine iguana samples (GIUS-12-3628), typical secondary amide structures were found at 1649 (amide I) and 1542 cm-1 (amide II) , , [53–56]. Amide I originates from the stretching vibration of C = O with minor contributions from CN, a CCN deformation and an NH bend , . The amide II mode is related to the combination of the NH bend and the stretching vibration of CN with contributions from CO, CC and NC ,  (Fig 5A). It is well known that all amide frequencies are conformation-sensitive, but amide I is the most widely used to determine protein conformations. Hence, we may attribute the α-helix secondary amide structure to the band at 1645 cm-1 . Additionally, according to the band-fitting procedure, the band located at 1451 cm-1 can be ascribed to the CN stretching mode in proline , ,  (compare Table 1). The bands corresponding to proteinaceous and lipid materials in Triassic fossil bones and blood vessels are summarized in Table 1. One important point worthy of consideration in conducting organic analysis based on infrared spectroscopy is the possible impact of bacterial and organic contamination which can be preserved in carbonate. For this reason, infrared analysis of bone material due to the strong vibration of νasymm(CO3)2- in the range of 1550‒1250 cm-1 is not completely unambiguous (Fig 5A–5C). To reduce the possibility of error during data analysis, SUT-MG/F/Tvert/15 without ferruginous coating (Fig 5D) was analyzed, as well as a sediment control sample (Fig 5E). In these cases, due to the high degree of degradation of the peptide, the amide signal was not observed. However, bands observed on the infrared spectrum of other Triassic bone samples (WNoZ/s/7/166, SUT-MG/F/Tvert/2; Fig 5B and 5C) at about 1594 and 1597 cm-1 originate from amino acid side chains , , . Additionally, according to the literature, this band may correspond to the CC stretching vibration in tyrosine , , [58, 59] or to the bending amine mode in glycine , [59, 60]. In turn, bands located at 1396, 1167 (SUT-MG/F/Tvert/2), and 1161 cm-1 (WNoZ/s/7/166) are associated with, respectively, the bending of N+(CH3)3 [49, 50] or stretching of (COO−) in asparagine , , [59, 60] and the anti-symmetric stretching of CO-O-C in asparagine , [51, 52]. Amide components were also detected in the blood vessel sample (Fig 5F and 5G) mineralized with goethite. The blood vessel FTIR spectra justified by peak fit analysis in the 1670‒1200 cm-1 region demonstrate features characteristic of structural proteins. Typical amide bands were found at approximately 1667, 1620 (amide I), 1584 (amide II) and 1366 cm-1 (amide III) . We infer that amide bands are associated with the stretching and bending vibrations of peptide (CO–NH) bonds. Moreover, due to protein conformations, the band at 1667 cm-1 may originate from turns secondary amide structure, while the band at 1620 cm-1 can be assigned to aggregated strands , . Importantly, the three additional bands at 1478, 1064 and 972 cm-1 resulted in the presence of amino acid residues and lipid absorptions , [51, 52]. According to the data in the literature, the amino acids and lipids preserved in the”blood vessel” are ascribed to vibrations of:
- CH2/CH3 with an anti-symmetric character ,  (1478 cm-1);
- NC/CC in trypsin  or C-O-P-O-C modes  (1064 cm-1);
- N+(CH3)3 with anti-symmetric stretching  (972 cm-1).
The organic signal observed on the infrared spectrum of WNoZ/s/7/166 (Fig 5F and 5G) is interpreted here as related to collagen or its degradation products. Amide I, in the form of aggregated strands, and amide III were assigned to bands located at 1609 and 1337 cm-1, respectively , . It is known that many amino acid side chains absorb in or near the amide I, amide II, and amide III regions of the infrared spectrum. Hence, the amino acid side chains on the infrared spectrum might be represented by the NH3+ vibration of lysine ,  or the CN vibration of proline or histidine  while the lipid absorptions are ascribed to the bending vibration of CH2 or stretching vibration of N+(CH3)3 . The impact of oxidative deamination which cleaves the N–C covalent bonds typical of proteins should be taken into account in the case of fossil material. Thus, many amino acid and lipid structures were assigned to 1549, 1478, 1423, 1099, 1043 and 972 cm-1 (see Table 1). Moreover, the very low-lying bands at 569 and 533 cm-1 were linked to the CH2 vibration of lipids.
High-Resolution Mass Spectrometry (ToF-SIMS)
Analyses of the ToF-SIMS spectra for both negative and positive polarity enabled the identification of a number of organic secondary ion species. The presence of various amino-acid-related nitrogen-containing species, for instance CH2N+ (m/z 28.02 Da), CH3N+ (m/z 29.03 Da), C3H2N+ (m/z 52.02 Da), NH3+ (m/z 17.02 Da), NH4+ (m/z 18.04 Da), CH5N+ (m/z 31.05 Da), C2H2N+ (m/z 40.02 Da), C2H3N+ (m/z 41.02 Da), C2H6N+ (m/z 44.05 Da), C3H4N+ (m/z 54.03 Da), C3H8N+ (m/z 58.06 Da), and C3H4NO+ (m/z 70.03 Da), observed in a mass spectrum is insufficient evidence to assign masses to specific amino acids. Similarly, in the case of research carried out for the detection of negative polarity arising from amino acids, specific ions, for instance NH- (m/z 15.01 Da), NH2- (m/z 16.02 Da), CN- (m/z 26.00 Da), CH2N- (m/z 28.02 Da), C2HN- (m/z 39.01 Da), C2H2N- (m/z 40.02 Da), CNO- (m/z 42.00 Da), C2H4N- (m/z 42.04 Da), CH2NO- (m/z 44.02 Da), CHS- (m/z 44.98 Da), CHO2- (m/z 44.99 Da), C3H3O2- (m/z 71.02 Da), C3HN2- (m/z 65.02 Da), C3H4NO- (m/z 70.03 Da), C6HN- (m/z 87.01 Da), and C6H3N- (m/z 89.03 Da), do not permit the clear identification of specific primary amino acids. Nevertheless, taking into account the presence of the several species CH4N+ C2H6N+ C4H6N+, C4H8N+, C5H10N+, C4H8NO+ and C5H10NO+, typically observed in amino acid mass spectra, we were enabled to conclude that organic compounds of glycine (CH4N+, m/z 30.03 Da), alanine (C2H6N+, m/z 44.05 Da), proline (C4H6N+, m/z 68.05 Da and C4H8N+, m/z 70.07 Da), leucine (C4H10N+, m/z 72.11 Da), and lysine (C5H10N+, m/z 84.08 Da), as well as hydroxyproline (C4H8NO+, m/z 86.06 Da) and hydroxylysine (C5H10NO+, m/z 100.08 Da) (Fig 6B and 6D) are present in the studied samples (compare in [9–11], [62–65]). Although CH4N+ (m/z 30.03 Da) is an ubiquitous amino-acid fragment, its presence next to fragments C4H6N+, C4H8N+ (attributed to proline), and C4H8NO+ (attributed to hydroxyproline) are very characteristic residues of type I collagen (compare ,  and the literature cited therein).
The spectra show expanded m/z regions associated with amino acids. The chemical structures of the ions (in red, framed) corresponding to a) lysine, b) hydroxylysine, c) proline, d) hydroxyproline, e) glycine, f) alanine, g) leucine, and h) iron are shown in the spectra in panels (a‒h). Other nitrogen-containing organic fragments corresponding to amino acids are also shown.
We did not detect the presence of possible organic-associated ions in the sediment control sample from close proximity to bone (not shown in the paper). The ToF-SIMS spectra of bone matrix provided additional information about inorganic ions, for example residues of the bone apatite matrix, such as Ca+ (m/z 39.96 Da), CaO+ (m/z 55.96), Ca2PO3+ (m/z 158.89 Da), Ca2PO4+ (m/z 174.88 Da), and many others, including P‒O species (compare in ). Most organic ions are absent, including hydroxyproline and hydroxylysine fragments (compare S5 Fig). The very weak signal from the CH4N+ ion, along with that from the C2H6N+ fragment, may have originated in the intercellular spaces of bone matrix (compare S5 Fig).
The XPS survey spectrum revealed oxygen, iron and carbon as the main components. Minor contributions to atomic concentration came from nitrogen, sodium, silicon, sulfur and phosphorus. In addition to their strong correlation with the results obtained from preliminary EDS investigations, the XPS measurements provided more complete information about the composition and chemical state of the analyzed surfaces. The atomic concentration of nitrogen with respect to iron is about 9%, while for sulfur it is 2%. The atomic O/Fe ratio is about 2.8. Analysis of the Fe 2p photoemission multiplet (Fig 7A) was performed in relation to the known experimental and theoretical data on Fe-O compounds . The structure of the spectrum indicates the presence of trivalent iron ions and probably more than one component. The main components can be attributed to goethite and hematite . The presence of a satellite peak with a binding energy of about 719 eV is characteristic for trivalent Fe compounds [67, 68], while the relatively strong component at 708.7 eV can be associated with divalent Fe ions, as in Fe3O4 [67, 68]. Taking into account the results obtained with other techniques, we can confirm that FeOOH is the main component containing iron, but other iron-containing compounds are present as well. This conclusion can be confirmed by the shape of the O 1s line, where more than two components characteristic for FeOOH were detected [69–71]. Analysis of the N 1s photoemission line shows the main component at 400.0 eV (Fig 7B). This binding energy is characteristic for amine or amide groups . The structure of the S 2p multiplet indicates two chemical states of sulfur (Fig 7C), one with binding energy of about 163 eV, which is associated with organic matter, and another with a maximum at about 168.8 eV, characteristic of the oxidized state of sulfur . In the control sample of recent marine iguana bone, the N 1s photoemission line and S 2p multiplet presented very similar values (not shown in the paper).
a) Fe 2p multiplet obtained for isolated fossilized blood vessels together with the results of fitting; b) N 1s line obtained for isolated fossilized blood vessels together with the results of fitting; c) S 2p multiplet obtained for isolated fossilized blood vessels from two different spots in the same sample of blood vessel: red line: internal part of fractured fossilized blood vessel (corresponding to lumina); purple line: external part of fractured fossilized blood vessel (corresponding to vessel wall).
Excluding Fungal and Microorganism Sources of Proteinaceous Organics
In 2008, Thomas G. Kaye and his coauthors (16) proposed that dinosaurian “soft tissues” found in fossil bones are bacterial biofilms which mimic real blood vessels and osteocytes. They suggested that microbial-mediated decay produced iron sulfides, which were later oxidized due to changing redox conditions. Therefore, in our study, special emphasis was placed on distinguishing mineralization of the original protein material of the bone from possible microbial contamination sources. Present-day studies on similar materials identified in bones of numerous taxa from the Cretaceous to the Recent , , , , as well as experimental approaches , support the endogeneity of the molecular material.
After an animal’s death, its bones are an attractive medium for diverse groups of microorganisms. Internal bone spaces such as medullary cavities and vascular channels can serve as migration paths for pore waters and mineral intrusions as well as biotic factors, for example fungi, hyphae and bacteria, which may introduce their own biomolecules (compare in ). Our examination of isolated fossilized “blood vessels” showed no microbial structures of any type in most analyzed samples. The absence of microbial activity traces, such as iron sulfides, especially pyritic framboids , as a product of microbial metabolism, and their oxidized forms, the pseudomorphoses  visible in optical or scanning electron microscopy, negate a significant impact by microbial contamination sources. Hyphae, filaments, and other spherical structures, both mineral and organic, are absent. There is no evidence of microborings on the outer bone surface or from fissures inside the bone.
The detection of hydroxyproline and hydroxylysine together in the analyzed material may indicate collagen as their potential source (compare in  and the literature cited therein). Although these amino acids may be included in proteins of various organisms, for the most part they occur separately. For instance, hydroxyprolines are found in plant glycoproteins [77, 78], and 2, 3-cis-3, 4-trans-3, 4-dihydroxy-L-proline, an analog of hydroxyproline, occurs in the cell walls of some diatoms [79, 80]. Hydroxylysine is also present in non-animal proteins, is a constituent of cell-wall-bound proteins in several groups of fungi , and can be formed by several bacteria , although the vast majority of bacteria cannot metabolize hydroxyproline (compare in ). Only some fungi and algae are able to produce both hydroxyproline and hydroxylysine . However, our finding derives from dense, compact bone. Penetration of microbial and non-microbial (remnants of other organisms) contamination into the buried bone would have been severely limited, if not impossible. It is noteworthy that ToF-SIMS analyses of isolated fossilized "blood vessels" and vascular lumina on the thin section failed to detect fragments corresponding to biomarkers found in many microorganisms (compare in [85–87]).
Preservation of Organic Molecules
We interpret the data presented here as evidence for the presence of organic residues in these specimens that may derive from collagen or its degradation products. Experimental approaches on thin sections of bone indicate that most of the bone collagen is removed by chemical rather than microbial degradation during the initial phase of bone diagenesis [88, 89]. Although protein degradation by bacterial activity in decaying bone can occur rapidly after death, does not progress rapidly, encompassing only 5 to 15% of the collagen present in fresh bone . Moreover, bacterial removal of collagen takes place only from the outermost 20 to 30 μm of the bone , where organic matter is most exposed. The inner part of the compact bone is therefore protected from bacterial invasion to a much greater extent than its outer part.
X-ray diffraction and infrared spectroscopy showed typical chemical alterations of bone apatite during fossilization, expressed as a transition from hydroxyapatite to carbonate fluoroapatite (compare in ). However, this diagenetic alteration has not entirely degraded the primary organic matter originally forming the "blood vessels". The ToF-SIMS mass measurement and ion imaging, as well as XPS and FTIR data collected on the isolated and in situ (in thin section) “blood vessels”, indicate that organic residues are strictly limited to ferruginous coating of “blood vessels” and do not occur in bone apatite separately. Organic signals are present in the infrared spectra of powdered fossil bone fragments (compare Fig 5B and 5C); however, they are very weak, and overlapped by phosphate and carbonate peaks.
The significant amplification of organic signals in FTIR analyses appears after EDTA incubation, and thus after removing phosphate and carbonate phases from samples (compare Fig 5F and 5G), which confirms that they are strongly connected with ferruginous mineralization of “blood vessels”. The fixation of organic residues must take place during collagen gelatinization at a very early stage of diagenesis, since later physicochemical alteration of bone apatite seemed not to have much of an effect on organic preservation. It has been hypothesized that iron (hydro)oxides may enhance the preservation of organic molecules, thus preventing microbial or enzymatic degradation , . Such a process of fossilization has been described from osteocytes in archaeological and fossil bones , and a chemical explanation for molecular and tissue “fixation” involving iron-catalyzed free-radical reactions without a role being played by bacterial decay was proposed by Schweitzer and her coauthors .
The marine iguana carcass was exposed to air after death, in contrast to the rapidly-buried Triassic bones. The remnants of partially removed or semi-dissolved collagen from the marine iguana, namely amide I (α-helix) at 1649 cm-1 and amide II at 1542 cm-1, are different from the iron-collagen cross links in fossil samples of “blood vessels”: amide I (turns) at 1667 cm-1, amide I (aggregated strands) at 1620 and 1609 cm-1, amide II at 1584 cm-1, and amide III at 1366 cm-1 and 1337 cm-1, respectively. Moreover, FTIR as well as ToF-SIMS studies of fossilized “blood vessels” indicate various amino acids functional for bone metabolism or formation of bone proteins and cell fluids, such as proline (CN stretching mode at 1478 cm-1 and C4H8N+, m/z 70.07 Da), glycine (bending amine mode at 1597 cm-1 and CH4N+, m/z 30.03 Da) as well as tyrosine, histidine, and asparagine ( and literature cited therein, see also ). Lipids have been also detected.
The mechanism of post-mortem iron-protein cross-linking proposed by Schweitzer and her colleagues  was also demonstrated by laboratory approaches. Additionally, it was shown  that iron oxides such as goethite may play an important role in both preserving and masking proteins in fossil tissues. The intimate association between organic molecules and iron in the studied bone samples is confirmed by SEM and ToF-SIMS imaging (compare Fig 3). Finally, the X-ray photoemission spectroscopy analysis helped to link molecular fragments identified by ToF-SIMS to bonding environments by confirming the presence of amide/amine bindings of nitrogen (Fig 7B). The low binding energy state of sulfur can be ascribed to sulfur-containing amino acids or to disulfides . The analysis of the Fe 2p the photoemission line (compare Fig 7A) showed no iron state which could be ascribed to iron sulfide. Thus, the low binding energy state of sulfur (Fig 7C) can be ascribed to sulfur-containing amino acids.
The blurring of microstructural features in the analyzed demineralized samples (Fig 1) as well as intensive signals from potential collagen-associated amino acids in the vascular lumen in thin sections (Fig 3E–3I) may result from the progressive gelatinization and/or partial dissolution of collagen, processes that take place at an early stage of bone diagenesis . Hydrolytic cleavage leads to fragmentation of bone collagen and its gelatinization and finally to collagen dissolution. Prior to complete dissolution, amorphous gelatin was leached by iron, triggering cross-linking, which acted as a fixative to stabilize the vessels. The source of iron for vessel mineralization could be heme and non-heme proteins, such as ferritin, derived from living cells and tissues (compare in , see also [90, 91]), since there were no sources of iron at all in the matrix surrounding the vessels. The breakdown of iron-bearing protein bonds releases iron, making it available for mineralization, and secondarily, remnant Fe3+ nanoparticles precipitate on the vessel walls . This seems to be consistent with ToF-SIMS imaging, where the most intense iron signals form an “agglutination” or “cloud” around the vascular channels (compare Fig 3D), while “organic” signals occupied the vascular lumen. This phenomenon of rapid fossilization must have occurred during early diagenesis, most likely immediately after the death of the organism. Because the total body iron content of various animals varies over a range of 25–75 mg/kg , which may be insufficient for the precipitation of iron (hydro)oxides, external sources of iron cannot be excluded . These iron-rich mineral casts are able to effectively protect fossil molecules over the long term.
Our study provides clear evidence that fossil molecules could survive through rapid, early diagenetic iron radical cross-linking. These biomolecules could effectively be preserved in iron-rich minerals when the minerals precipitated directly onto soft tissues, such as vessels and cells, and tightly covered their original structure. It can be assumed that the persistence of protein remains of endogenous origin in Early Triassic bones was the result of early post- mortem mineralization processes on the walls of blood vessels. Our observations confirm the hypothesis, that iron oxides can act as protective envelopes enabling the preservation of endogenous biomolecules in dinosaur bones from the distant geological past . This finding demonstrates that the possibility of the preservation of original soft tissue in iron-oxide mineral coatings may be greater than commonly believed and that molecules preserved in this way are structurally relatively undamaged and identifiable via spectral methods.
S1 Fig. Geographical location.
Geographical location. of outcrops and generalized geological section of Röt, Muschelkalk and Keuper in the Upper Silesia area. a) Geological section [after (32), strongly modified]; b) Map of Poland with location of outcrops.
S2 Fig. Infrared spectrum of pure disodium ethylenediaminetetraacetate (EDTA).
In the course of the analysis of the “blood vessel” samples, due to the demineralization process by EDTA, the EDTA spectrum was subtracted from the infrared spectra of vessels to completely eliminate the influence of this agent from the spectra and reveal the real component, i.e. part of the analyzed sample.
S3 Fig. Powder X-ray diffraction of a recent marine iguana (GIUS-12-3628).
The sample indicates poorly crystalline apatite corresponding to pattern #01-089-7834 (hydroxylapatite) with crystallites about 12 nm in size.
S4 Fig. Infrared spectra of analyzed samples and control samples in the hydroxylated region.
Peak fit analysis is based on the FTIR measurements for recent (a) and fossil (b‒d) bones; pure carbonate (e); and two samples of fossilized blood vessels of WNoZ/s/7/166 (f and g). In most cases (a‒c, f, g) distinguishing between an -OH group and amides A and B is difficult. In the control sample of nothosaurid femur (d), free of fossilized “blood vessels,” the typical amide signal from the region below 1800 cm-1 was not observed (compare Manuscript Fig 5D). Therefore the wide hump cannot be associated with any other amide in the region presented here. The signal/noise in the hydroxylated region for pure carbonate sample (host rock) is on very low level indicating lack of molecular water (e).
S5 Fig. ToF-SIMS positive polarity spectra of bone matrix (SUT-MG/F/Tvert/2 sample).
a) the spectrum from the range 20‒120 m/z corresponding to the range of occurrence of typical collagen-associated amino acid fragments, along with the juxtaposition of seven expanded m/z regions associated with amino acids as presented in Manuscript Fig 6; b) and c) weak signals from regions about m/z 30 (corresponding to CH4N+, m/z 30.03 Da) and about m/z 44 (corresponding to C2H6N+, m/z 44.05 Da) may have originated from intercellular spaces of bone matrix; d‒h) other regions corresponding to fragments as presented in Manuscript Fig 6, in detail: d) m/z 70.07 Da (C4H8N+), e) m/z 72.11 Da (C4H10N+), f) m/z 84.08 Da (C5H10N+), g) m/z 86.06 Da (C4H8NO+), h) m/z 100.08 Da (C5H10NO+), which may correspond to proline, leucine, lysine, hydroxyproline, and hydroxylysine, respectively. Note the lack of signals from other amino acids; i) comparison of ToF-SIMS spectra from the range m/z 55.92‒55.98 Da of bone matrix (black) and vessel wall (red) indicates the contribution of two different ions.
We thank Dr. Mary H. Schweitzer (North Carolina State University, Raleigh, NC, USA) for her insightful review of an early version of the manuscript, critical comments and scientific consultation, and Dr. Tomasz Krzykawski (University of Silesia, Sosnowiec, Poland) for performing X-ray diffraction analyses and for his kind help with the interpretation of the results. We would like to thank three anonymous reviewers whose opinions and comments have contributed to improving our manuscript. We also thank Dr. Timothy Bromage (New York University College of Dentistry, NY, USA) for providing the bones of a Galapagos marine iguana, and Editing Perfection (Gaj/Mogilany, Poland) for linguistic corrections and proofreading of our manuscript. This research project is supported by National Science Center, Poland (www.ncn.gov.pl) grant no. 2011/01/N/ST10/06989.
Conceived and designed the experiments: DS. Performed the experiments: DS AB RP KB MD JS. Analyzed the data: DS AB RP KB MD JS BK. Contributed reagents/materials/analysis tools: DS AB KB MD BK RP JS. Wrote the paper: DS AB KB MD BK JS. Designed the software used in analysis: DS AB KB MD JS. Experimental part made by: MD (FTIR) KB (ToF-SIMS) JS (XPS) DS AB RP (LM, ESEM).
- 1. Lindahl T. Instability and decay of the primary structure of DNA. Nature. 1993; 362, 709–715. doi: 10.1038/362709a0. pmid:8469282
- 2. Pawlicki R, Korbel A, Kubiak H. Cells, collagen fibrils and vessels in dinosaur bone. Nature. 1966; 211, 655–657. doi: 10.1038/211655a0. pmid:5968744
- 3. Pawlicki R. Histochemical reactions for mucopolysaccharide in the dinosaur bone. Acta Histochemica. 1977; 58, 75–78. http://www.ncbi.nlm.nih.gov/pubmed/140578. pmid:140578
- 4. Pawlicki R. Topochemical localization of lipids in dinosaur bone by means of Sudan B black. Acta Histochemica. 1977; 59, 40–46. doi: 10.1016/S0065-1281(77)80077-9. pmid:72479
- 5. Pawlicki R. Histochemical demonstration of DNA in osteocytes from dinosaur bones. Folia Histochemica et Cytobiologica. 1995; 33, 183–186. http://www.ncbi.nlm.nih.gov/pubmed/8612871. pmid:8612871
- 6. Gurley LR, Valdez JG, Spall WD, Smith BF, Gillette DD. Proteins in the fossil bone of the dinosaur, Seismosaurus. J Protein Chem. 1991; 10, 75–90. Proteins in the fossil bone of the dinosaur, Seismosaurus. pmid:2054066 doi: 10.1007/bf01024658
- 7. Muyzer G, Sandberg P, Knapen MHJ, Vermeer C, Collins M, Westbroek P. Preservation of bone protein osteocalcin in dinosaurs. Geology. 1992; 20. 871–874. doi: 10.1130/0091-7613(1992)020<0871:potbpo>2.3.co;2
- 8. Asara JM, Schweitzer MH, Freimark LM, Phillips M, Cantley LC. Protein sequences from mastodon and Tyrannosaurus rex revealed by mass spectrometry. Science. 2007; 316, 280–285. http://dx.doi.org/10.1126/science.1137614. pmid:17431180
- 9. Schweitzer MH, Suo Z, Avci R, Asara JM, Allen MA, Arce FT, Horner JR. Analyses of Soft Tissue from Tyrannosaurus rex Suggest the Presence of Protein. Science. 2007; 316, 277–280. http://dx.doi.org/10.1126/science.1138709. pmid:17431179
- 10. Schweitzer MH, Avci R, Collier T, Goodwin MB. Microscopic, chemical and molecular methods for examining fossil preservation. C. R. Palevol. 2008; 7, 159–184. doi: 10.1016/j.crpv.2008.02.005
- 11. Schweitzer MH, Zheng W, Organ CL, Avci R, Suo Z, Freimark LM, et al. Biomolecular characterization and protein sequences of the Campanian hadrosaur B. canadensis. Science. 2009; 324, 626–631. doi: http://dx.doi.org/10.1126/science.1165069. pmid:19407199
- 12. Schweitzer MH, Zheng W, Cleland TP, Bern M. Molecular analyses of dinosaur osteocytes support the presence of endogenous molecules. Bone. 2013; 52, 414–423. doi: 10.1016/j.bone.2012.10.010. pmid:23085295
- 13. Cleland TP, Schroeter ER, Schweitzer MH. Biologically and diagenetically derived peptide modifications in moa collagens. Proc. R. Soc. B. 2015; 282: 20150015. doi: http://dx.doi.org/10.1098/rspb.2015.0015. pmid:25972464
- 14. Buckley M, Walker A, Ho SY, Yang Y, Smith C, Ashton P, et al. Comment on “Protein Sequences from Mastodon and Tyrannosaurus rex Revealed by Mass Spectrometry”. Science 2008; 4 (319): 33c. doi: 10.1126/science.1147046.
- 15. Cleland TP, Schroeter ER, Zamdborg L, Zheng W, Lee JE, Tran JC, et al. Mass Spectrometry and Antibody-Based Characterization of Blood Vessels from Brachylophosaurus canadensis. J. Proteome Res., 2015, 14; 12, 5252–5262. doi: 10.1021/acs.jproteome.5b00675. pmid:26595531
- 16. Kaye TG, Gaugler G, Sawłowicz Z. Dinosaurian soft tissues interpreted as bacterial biofilms. PLoS ONE. 2008; 3(7): e2808. doi: 10.1371/journal.pone.0002808. pmid:18665236
- 17. Chinsamy-Turan A. The microstructure of dinosaur bone. Baltimore: Johns Hopkins University Press; 2005.
- 18. Reisz RR, Huang TD, Roberts EM, Peng SR, Sullivan C, Stein K, et al. Embryology of Early Jurassic dinosaur from China with evidence of preserved organic remains. Nature Letter. 2013; 496, 210–214. doi: http://dx.doi.org/10.1038/nature11978.
- 19. Lindgren J, Uvdal P, Engdahl A, Lee AH, Alwmark C, Bergquist K-E et al. Microspectroscopic Evidence of Cretaceous Bone Proteins. PLoS ONE. 2011; 6(4), e19445, doi: 10.1371/journal.pone.0019445. pmid:21559386
- 20. Schweitzer MH, Watt JA, Avci R, Forster CA, Krause DW, Knapp L, et al. Keratin immunoreactivity in the Late Cretaceous bird Rahonavis ostromi. Journal of Vertebrate Paleontology. 1999; 19, 712–722. doi: 10.1080/02724634.1999.10011183.
- 21. Schweitzer MH, Watt JA, Avci R, Knapp L, Chiappe L, Norell M, et al. Beta-Keratin Specific Immunological Reactivity in feather-like structures of the Cretaceous Alvarezsaurid, Shuvuuia desertii. Journal of Experimental Zoology. 1999; 285, 146–157. doi: http://www.ncbi.nlm.nih.gov/pubmed/10440726. pmid:10440726
- 22. Bertazzo S, Maidment SCR, Kallepitis C, Fearn S, Stevens MM, Xie H-n. Fibres and cellular structures preserved in 75-million-year-old dinosaur specimens. Nat Commun. 2015; 6, 7352, doi: 10.1038/ncomms8352 (2015). pmid:26056764
- 23. Greenwalt DE, Goreva YS, Siljeström SM, Rose T, Harbach RE. Hemoglobin-derived porphyrins preserved in a Middle Eocene blood-engorged mosquito. PNAS. 2013; doi: 10.1073/pnas.1310885110.
- 24. Lindgren J, Uvdal P, Sjövall P, Nilsson DE, Engdahl A, Schultz BP, et al. Molecular preservation of the pigment melanin in fossil melanosomes. Nat Commun. 2012; 3, 824, doi: 10.1038/ncomms1819. pmid:22569368
- 25. Lindgren J, Moyer A, Schweitzer MH, Sjövall P, Uvdal P, Nilsson DE et al. Interpreting melanin-based coloration through deep time: a critical review. Proc. R. Soc. B. 2015; 282: 20150614, doi: http://dx.doi.org/10.1098/rspb.2015.0614. pmid:26290071
- 26. Schweitzer MH, Zheng W, Cleland TP, Goodwin MB, Boatman E, Theil E et al. A role for iron and oxygen chemistry in preserving soft tissues, cells and molecules from deep time. Proc. R. Soc. B. 2014; 281 20132741 doi: http://dx.doi.org/10.1098/rspb.2013.2741. pmid:24285202
- 27. Kremer B, Bauer M, Stark RW, Gast N, Altermann W, Gursky H-J et al. Laser-Raman and atomic force microscopy assessment of the chlorococcalean affinity of problematic microfossils. J. Raman Spectrosc. 2012; 43, 32–39. doi: http://dx.doi.org/10.1002/jrs.2985.
- 28. Hagdorn H, Szulc J. STOP I. 1. Gogolin–inactive quarry. In: Szulc J. & Becker A., editors. Pan-European Correlation of the Epicontinental Triassic. 4th Meeting, International Workshop on the Triassic of Southern Poland. September 3–8, 2007. Fieldtrip Guide; 2007. pp. 46.
- 29. Kowal-Linka M. Formalizacja litostratygrafii formacji gogolińskiej (trias środkowy) na Śląsku Opolskim., Geologos. 2008; 14, 125–161 (in Polish).
- 30. Assmann P. Die Stratigraphie der oberschlesischen Trias. Teil II. Der Muschelkalk. Berlin: Reichsamts Bodenforsch. 1944.
- 31. Zawidzka K. Conodont stratigraphy and sedimentary environment of the Muschelkalk in Upper Silesia. Acta Geologica Polonica. 1975; 25, 217–257.
- 32. Szulc J. Middle Triassic Evolution of the Northern Peri-Tethys area as influenced by early opening of the Tethys Ocean. Ann. Soc. Geol. Polon. 2000; 70, 1–48.
- 33. Nawrocki J, Szulc J. Magnetic polarity scale for the Roetian and Muschelkalk deposits from Silesia and northern part of the Holy Cross Mts (Poland) (in Polish with English summary). Przegląd Geologiczny. 2000; 3, 236–238.
- 34. Kowal-Linka M, Jochum KP, Surmik D. LA-ICP-MS analysis of rare earth elements in marine reptile bones from the Middle Triassic bonebed (Upper Silesia, S Poland): Impact of long-lasting diagenesis, and factors controlling the uptake. Chem. Geol. 2014; 363, 213–228, doi: http://dx.doi.org/10.1016/j.chemgeo.2013.10.038.
- 35. Surmik D. Preliminary taphonomical analysis of Lower Muschelkalk bone accumulation in Silesia (Poland). In: Nowakowski D. editor. Morphology and Systematic of Fossil Vertebrates. Wrocław: DN Publisher; 2010. pp. 110–117.
- 36. Rieppel O. Sauropterygia I–Placodontia, Pachypleurosauria, Nothosauroidea, Pistosauroidea. In: Handbuch der Palaherpetologie. Verlag Dr. Friedrich Pfeil; 2000.
- 37. Diedrich CG. Palaeogeographic evolution of the marine Middle Triassic marine Germanic Basin changements–With emphasis on the carbonate tidal flat and shallow marine habitats of reptiles in Central Pangaea. Global and Planetary Change. 2009; 65, 27–55. doi: 10.1016/j.gloplacha.2008.11.002.
- 38. Rieppel O, Hagdorn H. Paleobiogeography of Middle Triassic Sauropterygia in Central and Western Europe. In: Callaway J. M. & Nicholls E. L., editors. Ancient Marine Reptiles. San Diego: Academic Press, 1997. pp. 121–144.
- 39. Rieppel O. Fragmenta Sauropterygiana. Neues Jahrbuch für Geologie und Palaeontologie. 1995; 197, 383–397.
- 40. Rieppel O. Phylogeny and paleobiogeography of Triassic Sauropterygia–problems solved and unresolved. Palaeogeography, Palaeoclimatology, Palaeoecology. 1999; 153, 1–15. doi: 10.1016/S0031-0182(99)00067-X.
- 41. Kowal-Linka M, Bodzioch A. Bonebeds with Dactylosaurus (Reptilia, Sauropterygia) from the Röt (Lower Triassic, Olenekian) in the Opole Silesia region (S Poland). Przegląd Geologiczny. 2012; 60 646–649.
- 42. Piga G, Santos-Cubedo A, Brunetti A, Piccinini M, Malgosa A, Napolitano E, et al. A multi-technique approach by XRD, XRF, FT-IR to characterize the diagenesis of dinosaur bones from Spain. Palaeogeography, Palaeoclimatology, Palaeoecology. 2011; 310, 92–107. doi: 10.1016/j.palaeo.2011.05.018.
- 43. Povarennykh AS. The use of infrared spectra for the determination of mineral. American Mineralogist. 1978; 63, 956–959.
- 44. Fysh SA, Frederick PM. Fourier transform infrared studies of aluminous goethites and hematites. Clays and Clay Minerals. 1983; 31, 377–382. doi: 10.1346/ccmn.1983.0310507
- 45. Cambier P. Infrared study of goethite of varying crystallinity and particle size: I. Interpretation of OH and lattice vibration frequencies. Clay Minerals. 1986; 21, 191–200. doi: 10.1180/claymin.1986.021.2.08
- 46. Tadic D, Epple M. A thorough physicochemical characterization of 14 Ca phosphate-based bone substitution materials in comparison to natural bone. Biomaterials. 2004; 25, 987–994. doi: 10.1016/S0142-9612(03)00621-5. pmid:14615163
- 47. Stathopoulou ET, Psycharis V, Chryssikos GD. Bone diagenesis: new data from Infrared spectroscopy and X-Ray Diffraction. Palaeogeography, Palaeoclimatology, Palaeoecology. 2008; 266, 168–174. doi: 10.1016/j.palaeo.2008.03.022.
- 48. Barth A. Infrared spectroscopy of proteins. Biochim. Biophys. Acta. 2007; 1767, 1073–1101. doi: 10.1016/j.bbabio.2007.06.004. pmid:17692815
- 49. Lagant P, Vergoten G, Peticolas WL. On the use of ultraviolet resonance Raman intensities to elaborate molecular force fields: application to nucleic acid bases and aromatic amino acid residues models. Biospectroscopy. 1998; 4, 379–393. doi: http://www.ncbi.nlm.nih.gov/pubmed/9851719. pmid:9851719
- 50. Venyaminov SY, Kalnin NN. Quantitative IR spectrophotometry of peptide compounds in water (H2O) solutions. I. Spectral parameters of amino acid residue absorption bands. Biopolymers. 1990; 30, 1243–1257. doi: http://www.ncbi.nlm.nih.gov/pubmed/2085660. pmid:2085660
- 51. Stuart B. Biological Applications of Infrared Spectroscopy. John Wiley and Sons; 1997.
- 52. Stuart B. Infrared Spectroscopy: Fundamentals and Applications. John Wiley and Sons; 2004.
- 53. de Vidal BC, Mello ML. Collagen type I amide I band infrared spectroscopy. Micron. 2011; 42, 283–289. doi: 10.1016/j.micron.2010.09.010. pmid:21134761
- 54. Krimm S, Bandekar J. Vibrational spectroscopy and conformation of peptides, polypeptides, and proteins. Adv. Prot. Chem. 1986; 38, 181–367. doi: 10.1016/S0065-3233(08)60528-8.
- 55. Oberg KA, Ruysschaert JM, Goormaghtig E. The optimization of protein secondary structure determination with infrared and circular dichroism spectra. Eur. J. Biochem. 2004; 271, 2937–2948. doi: http://www.ncbi.nlm.nih.gov/pubmed/15233789. pmid:15233789
- 56. Camacho NP, West P, Torzilli PA, Mendelsohn R. FTIR microscopic imaging of collagen and proteoglycan in bovine cartilage. Biopolymers. 2001; 62, 1–8. doi: http://www.ncbi.nlm.nih.gov/pubmed/11135186. pmid:11135186
- 57. Rothschild KJ, He YW, Gray D, Roepe PD, Pelletier SL, Brown RS, et al. Fourier transform infrared evidence for proline structural changes during the bacteriorhodopsin photocycle. Proc. Natl. Acad. Sci. 1989; 86, 9832–9835. http://www.ncbi.nlm.nih.gov/pmc/articles/PMC298596/ pmid:2602377
- 58. Hienerwadel R, Boussac A, Breton K, Diner B, Berthomieu C. Fourier transform infrared difference spectroscopy of photosystem II tyrosine D using site-directed mutagenesis and specific isotope labeling. Biochemistry. 1997; 36, 14712–14723. doi: 10.1021/bi971521a. pmid:9398191
- 59. Rothschild KJ, Roepe P, Ahl PL, Earnest TN, Bogomolni RA, Das Gupta SK, et al. Evidence for a tyrosine protonation change during the primary phototransition of bacteriorhodopsin at low temperature. Proc. Natl. Acad. Sci. 1986; 83, 347–351. http://www.ncbi.nlm.nih.gov/pubmed/3001733. pmid:3001733
- 60. Rahmelow K, Hübner W, Eckermann T. Infrared absorbances of protein side chains. Anal. Biochem. 1998; 257, 1–11. http://www.ncbi.nlm.nih.gov/pubmed/9512765. pmid:9512765
- 61. Tamm LK, Tatulian SA. Infrared spectroscopy of proteins and peptides in lipid bilayers. Quarterly Reviews of Biophysics. 1997; 30, 365–429. http://www.ncbi.nlm.nih.gov/pubmed/9634652. pmid:9634652
- 62. Sanni OD, Wagner MS, Briggs D, Castner DG, Vickerman JC. Classification of adsorbed protein static ToF-SIMS spectra by principal component analysis and neural networks. Surf. Interface Anal. 2002, 33, 715–728. doi: 10.1002/sia.1438.
- 63. Wagner MS, Castner DG. Analysis of adsorbed proteins by static time-of-flight secondary ion mass spectrometry. Applied Surface Science. 2004; 231–232, 366–376. doi: 10.1016/j.apsusc.2004.03.100.
- 64. Muramoto S, Graham DJ, Wagner MS, Lee TG, Moon DW, Castner DG. ToF-SIMS Analysis of Adsorbed Proteins: Principal Component Analysis of the Primary Ion Species Effect on the Protein Fragmentation Patterns. J Phys Chem C Nanomater Interfaces. 2011; 115, 24247–24255. doi: 10.1021/jp208035x. pmid:22308191
- 65. Graham DJ, Wagner MS, Castner DG. Information from Complexity: Challenges of TOF-SIMS Data Interpretation. Applied Surface Science. 2006; 252, 6860–6868. doi: 10.1016/j.apsusc.2006.02.149.
- 66. Henss A, Rohnke M, El Khassawna T, Govindarajan P, Schlewitz G, Heiss C, et al. Applicability of ToF-SIMS for monitoring compositional changes in bone in a long-term animal model. J R Soc Interface. 2013; 10, 20130332. http://dx.doi.org/10.1098/rsif.2013.0332. pmid:23864501
- 67. Grosvenor AP, Kobe BA, Biesinger MC, McIntyre NS. Investigation of multiplet splitting of Fe XPS spectra and bonding in iron compounds. Surf. Interface Anal. 2004; 36, 1564–1574. doi: 10.1002/sia.1984.
- 68. Graat P, Somers MAJ. Quantitative Analysis of Overlapping XPS Peaks by Spectrum Reconstruction: Determination of the Thickness and Composition of Thin Iron Oxide Films. Surf. Interface Anal. 1998; 26, 773–782. doi: 10.1002/(SICI)1096-9918(199810)26:11<783::AID-SIA420>3.0.CO;2-O.
- 69. Mansour AN, Brizzolara RA. Characterization of the Surface of -FeOOH Powder by XPS. Surface Science Spectra. 1996; 4, 357; doi: 10.1116/1.1247825.
- 70. Baltrusaitis J, Cwiertny DM, Grassian VH. Adsorption of sulfur dioxide on hematite and goethite particle surfaces. Phys. Chem. Chem. Phys. 2007; 9, 5542–5554. http://www.ncbi.nlm.nih.gov/pubmed/17957310. pmid:17957310
- 71. Welsh ID, Sherwood PMA. Photoemission and electronic structure of FeOOH: Distinguishing between oxide and oxyhydroxide. Physical Review B. 1989; 40, 6386–6392. http://www.ncbi.nlm.nih.gov/pubmed/9992712.
- 72. Jansen RJJ, van Bekkum H. XPS Of Nitrogen-Containing Functional Groups On Activated Carbon, Carbon 1995; 33, 1021–1027. doi: 10.1016/0008-6223(95)00030-H.
- 73. Atzei D, Fantauzzi M, Rossi A, Fermo P, Piazzalunga A, Valli G, et al. Surface chemical characterization of PM10 samples by XPS. Applied Surface Science, 2014 307, 120–128. doi: 10.1016/j.apsusc.2014.03.178.
- 74. Bell LS, Kayser M, Jones C. The Mineralized Osteocyte: A Living Fossil. Am. J. Phys. Anthropol. 2008; 137, 449–456. http://www.ncbi.nlm.nih.gov/pubmed/18615594. doi: 10.1002/ajpa.20886. pmid:18615594
- 75. Turner-Walker G. Pyrite and Bone Diagenesis in Terrestrial Sediments–Evidence from the West Runton Freshwater Bed. Bull. Geol. Soc. Norfolk. 1999; 48, 3–26.
- 76. Sawłowicz Z, Kaye TG. Replacement of iron sulphides by oxides in the dinosaur bone from the Lance Fm. (Wyoming, USA)–preliminary study. Mineralogia Polonica Spec. Pap. 2006; 29, 184–187.
- 77. Sommer-Knudsen J, Bacic A, Clarke AE. Hydroxyproline-rich plant glycoproteins. Phytochemistry. 1998; 47, 4, 483–497. doi: 10.1016/S0031-9422(97)00724-3.
- 78. Wu H, de Graaf B, Mariani C, Cheung AY. Hydroxyproline-rich glycoproteins in plant reproductive tissues: structure, functions and regulation. Cell Mol Life Sci. 2001; 58, 10, 1418–29. doi: 10.1007/PL00000785. pmid:11693523
- 79. Nakajima T, Volcani BE. 3,4-Dihydroxyproline: A New Amino Acid in Diatom Cell Walls. Science 1969; 164, 1400–1401. http://www.ncbi.nlm.nih.gov/pubmed/5783709. pmid:5783709
- 80. Nakajima T, Volcani BE. N-Trimethyl-α-hydroxylysinephosphate and its nonphosphorylated compound in diatom cell walls. Biochem. Biophys. Res. Comm. 1970; 39, 28–33. pmid:5438297 doi: 10.1016/0006-291x(70)90752-7
- 81. Ruiz-Herrera J. Fungal Cell Wall: Structure, Synthesis, and Assembly. CRC Press; Second Edition. 2012. ISBN 9781439848371.
- 82. de Lorenzo V, Bindereif A, Paw BH, Neilands JB. Aerobactin biosynthesis and transport genes of plasmid ColV-K30 in Escherichia coli K-12. Journal of Bacteriology 1986; 165, 2, 570–578. http://www.ncbi.nlm.nih.gov/pubmed/2935523. pmid:2935523
- 83. Watanabe S, Morimoto D, Fukumori F, Shinomiya H, Nishiwaki H, Kawano-Kawada M, et al. Identification and characterization of D-hydroxyproline dehydrogenase and Delta1-pyrroline-4-hydroxy-2-carboxylate deaminase involved in novel L-hydroxyproline metabolism of bacteria: metabolic convergent evolution. J. Biol. Chem. 2012; 287, 32674–32688. http://www.ncbi.nlm.nih.gov/pubmed/22833679. pmid:22833679
- 84. Adams E. Invertebrate collagens. Marked differences from vertebrate collagens appear in only a few invertebrate groups. Science. 1978; 202, 591–598. pmid:212833 doi: 10.1126/science.212833
- 85. Leefmann T, Heim C, Siljeström S, Blumenberg M, Sjövall P, Thiel V. Spectral characterization of ten cyclic lipids using time-of-flight secondary ion mass spectrometry. Rapid Commun Mass Spectrom. 2013; 27, 565–81. doi: 10.1002/rcm.6483. pmid:23413216
- 86. Ivarsson M, Broman C, Sturkell E, Ormö J, Siljeström S, van Zuilen M, et al. Fungal colonization of an Ordovician impact-induced hydrothermal system. Scientific Reports. 2013l 3, 3487, doi: 10.1038/srep03487. pmid:24336641
- 87. Thiel V, Blumenberg M, Kiel S, Leefmann T, Liebenau K, Lindgren J, et al. Occurrence and fate of fatty acyl biomarkers in an ancient whale bone (Oligocene, El Cien Formation, Mexico). Organic Geochemistry. 2014; 68, 71–81. doi: 10.1016/j.orggeochem.2013.12.006.
- 88. Collins MJ, Nielsen-Marsh CM, Hiller J, Smith CI, Roberts JP, Prigodich RV, et al. The survival of organic matter in bone: A review. Archaeometry. 2002; 44, 3, 383–394. http://dx.doi.org/10.1111/1475-4754.t01-1-00071.
- 89. Peretzschner H- U. Collagen gelatinization: the key to understand early bone-diagenesis. Palaeontographica Abteilung A Band. 2006; 278, 135–148.
- 90. Eisenstein RS. Iron regulatory proteins and the molecular control of mammalian iron metabolism. Ann. Rev. Nutr. 2000; 20, 627–662. http://www.ncbi.nlm.nih.gov/pubmed/10940348.
- 91. Theil EC, Goss DJ. Living with iron (and oxygen): questions and answers about iron homeostasis. Chem. Rev. 2009; 109, 4568–4579. http://www.ncbi.nlm.nih.gov/pmc/articles/PMC2919049/. doi: 10.1021/cr900052g. pmid:19824701
- 92. National Academy of Science. Iron. Report of the Subcommittee on Iron, National Academy of Science Committee on Medical and Biological Effects of Environmental Pollutants. Baltimore: University Park Press; 1979.
- 93. Pawlicki R. Metabolic pathways of the fossil dinosaur bones. Part I. Vascular communication system. Folia Histochem. Cytobiol. 1983; 21, 253–262.