Category 1 comprises dubiofossils, structures resembling fossils that were previously associated with life but possess an ambiguous origin (Hofmann, 1972), Supplementary Material 2 presents all articles compiled about dubiofossils in relation to the data and applied techniques, which were quantified in Supplementary Material 3. These dubiofossils are categorized into three classes (Figure 2A). The microfossil-like dubiofossils class (1a) has substantial biogenicity criteria, postulated and revised by Buick (1990); Cady et al. (2003); Benzerara and Menguy (2009); Schopf et al. (2010); Brasier and Wacey (2012); McMahon et al. (2021), and Rouillard et al. (2021). These criteria encompass internal morphology (I) – approximately 83% of the total 1a articles; external structure (S), inorganic composition (C) data and mapping (M) – both with roughly 66% of the total of 1a (Figure 2B). For ichnofossil-like dubiofossils (1b), the biogenicity criteria are outlined by Awramik and Grey (2005); Porada et al. (2008); Noffke (2009, 2010, 2021); Wacey (2010); Noffke and Awramik (2013); Davies et al. (2016), Davies et al. (2020) and Lucas and Lerner (2017), Sanchez et al. (2023), which reveal that it is important to characterize data on inorganic composition (C) – almost 92% of the total 1b articles; and texture (T) – approximately 84% of the 1b articles, supported by internal morphological characteristics (I) – roughly 69% of the 1b (Figure 2B). The biomineral-like dubiofossils (1c) lacks well established biogenicity criteria discussed by García-Ruiz et al. (2002); Braissant et al. (2003); Weiner and Dove (2003); Dupraz et al. (2009); Benzerara and Menguy (2009); Cailleau et al. (2009); Bindschedler et al. (2014); McMahon and Comidis (2022), and Saldanha et al. (2023). This highlight the need to obtain morphological data (S and I) – all 1c articles used S data and approximately 83% I data; and inorganic compositional data (C) – all 1c articles. In respect to texture (T) – half of the articles assessed this; and Compositional mapping (M) was performed by roughly 33% of the total 1c articles (Figure 2B).

For 1a, morphology characterization is crucial, focusing on general shape, internal features, and population morphology range, best achieved through OM, SEM-EDS/FIB-SEM, nano or micro-CT (Buick, 1990; Javaux et al., 2003; Sugitani et al., 2007; McMahon et al., 2021). General size, population range, and morphometric consistency further support abiotic or biotic hypotheses (Figures 2C, 3). Details, ornamentation, and preservation textures can contribute secondarily, both obtained by nano- or micro-CT, PXCT or SEM (Hofmann et al., 2008; Dodd et al., 2017; Johannessen et al., 2020; Maldanis et al., 2020). Compositional analysis is less decisive due to potential confusion with abiotic objects (Brasier et al., 2002, 2004; Schiffbauer et al., 2007), as seen in the dispute over Apex Chert microfossils (Schopf et al., 2002; Brasier et al., 2004; Schopf and Kudryavtsev, 2012). Complementary analyses like RS, TEM, XANES, MS, LA-ICP-MS, GC-MS, are useful in such cases (Brasier et al., 2004; De Gregorio et al., 2009; Alleon et al., 2016; Dodd et al., 2017). Detecting kerogen associated with microbial morphologies may be relevant in specific contexts using RS, FT-IR or XANES (Schopf et al., 2002; 2005; Sugitani et al., 2007; Dodd et al., 2017; Gomes et al., 2019; Osterhout et al., 2021).

For 1b (Figures 2C, 3), microscopic features like filamentous morphologies and putative EPS, and ornamentations, diagnosed with OM and SEM-EDS/FIB-SEM (sometimes complemented by TEM or FIB-TEM, STXM or SRXTM), may be pertinent, although macroscopic forms are of secondary relevance, and size is less crucial (Noffke et al., 2001, 2003, 2006; Porada et al., 2008; De Gregorio et al., 2009; Inglez et al., 2021). Verifying composition is important, especially for organic matter detection (RS, XANES) and bioindicator elements (EDS, XRD, XRF or SR-XRF, RS, MS) (De Gregorio et al., 2009; Wacey, 2010; Allwood et al., 2018; Callefo et al., 2019b; Alleon et al., 2021; Klug et al., 2021). Caution is advised due to the ongoing debate on reliability of biomarkers (Brasier et al., 2002; Marshall et al., 2012; Schopf and Kudryavstev, 2012; Bower et al., 2015).

For 1c (Figures 2C, 3), it is necessary to identify general morphology, internal structures, mineral habit, and crystallinity, described mainly through OM, accompanied by SEM-EDS and Micro-CT for determining general shape and texture (Cailleau et al., 2009; Bindschedler et al., 2014; Tisato et al., 2015; Green, 2022; Saldanha et al., 2023). Secondarily, mineral orientation, crystalline defects, twinning, and habits are considered (Braissant et al., 2003; Cailleau et al., 2009; Saldanha et al., 2023), with good results coming out from OM, SEM-EDS, and CT if the object differs compositionally from the matrix. The composition is key for identifying minerals and assessing diagenetic modifications, obtained through EDS, XRF, XRD, RS, MS (Braissant et al., 2003; Cailleau et al., 2009; Tisato et al., 2015).

The biogenicity arguments for 1a are based on the interpretation of biological morphologies, such as walls and hollow features, ornamentation, periodicity, and branching (Buick, 1990). This includes assessing consistent morphologies, normal distribution of population sizes, and taphonomic variations to identify globular, filamentous, or even colonial forms (Buick, 1990; Javaux et al., 2003; Sugitani et al., 2007; Maldanis et al., 2020; McMahon et al., 2021). Evidencing the organic/kerogen composition is desirable, but requires great caution in its interpretation, avoiding erroneous conceptions of abiotic origin or diagenetic modifications (Schopf et al., 2002, 2005; Brasier et al., 2002, 2004; Schiffbauer et al., 2007; Sugitani et al., 2007; Dodd et al., 2017; Gomes et al., 2019). For 1b, the biogenicity criteria are interpreted from textural relationships, diagnostics of filamentous features, and their distribution in the framework (Noffke et al., 2001). Mineral orientation may also be relevant (e.g., Noffke et al., 2001, 2003; Inglez et al., 2021). Verifying composition is important, especially for detecting organic matter and bioindicator elements (Brasier et al., 2002; Marshall et al., 2012; Schopf and Kudryavtsev, 2012; Bower et al., 2015). For 1c, the detection of crystal defects, variations in mineral habit, degree of crystallinity, and distinct matrix composition aids in discussing the biogenicity of biomineral dubiofossils (Braissant et al., 2003; Cailleau et al., 2009; Bindschedler et al., 2014; Tisato et al., 2015; Saldanha et al., 2023). Composition is key for identifying minerals and assessing diagenetic modifications (Braissant et al., 2003; Tisato et al., 2015). However, composition alone cannot serve as the main biogenicity argument, as no mineral species or characteristics are uniquely tied to life (Weiner and Dove, 2003; Benzerara and Menguy, 2009; Benzerara et al., 2019). Figure 3 summarizes a protocol of how to proceed using techniques to obtain specific data (result and information) aiming to test hypotheses (discussion).

The discussion of the biogenicity of any dubiofossil is typically conducted in four steps (compiled from Buick, 1990; García-Ruiz et al., 2002; Brasier et al., 2002; Schopf et al., 2002; Brasier et al., 2004; Westall, 2008; Noffke, 2009, 2021; Slater, 2009; Wacey, 2010; Brasier and Wacey, 2012; Schopf and Kudryavtsev, 2012; McLoughlin and Grosch, 2015; Callefo et al., 2019a; Gomes et al., 2019; Neveu et al., 2018; McMahon et al., 2021; Rouillard et al., 2021; Saldanha et al., 2023), presented in Figure 3, from the technique used to obtain the data and results relate to more specific information until reaching the steps to discuss and decipher the origin of the dubiofossil: 1) Deciphering syngenicity and indigeneity: evaluating the relationships of cutting, inclusion, and subsequent modifications to establish the timing of the processes and ensure there is no contamination (Buick, 1990; Wacey, 2009; McLoughlin and Grosch, 2015; Rouillard et al., 2021). 2) Understanding diagenetic history: detailing all the processes that may have transformed the material, throughout the entire trajectory from immediately after its deposition/formation until collection. 3) Reconstructing the original scenario: based on additional information about the environment, age, and context, this step involves hypothesizing the possible environmental processes that formed the material. 4) Integrating information: this final step involves evaluating the most plausible hypotheses about the origin of the object, discarding less likely processes. This evaluation is based mainly on the interpretations of the results and comparisons with similar modern and/or fossil objects and processes (Figure 3). It is recommended to use biotic versus abiotic hypotheses with equal weights (Hofmann, 1972; Buick, 1990; Benzerara and Menguy, 2009; McMahon et al., 2021; Rouillard et al., 2021). After the discussion, the object can be included as a fossil or a pseudofossil if it has sufficient evidence or alternatively remain as a dubiofossil (Hofmann, 1972).

It is well-established that authigenic mineralization resulting in fossilization depends on microorganisms, which decay organic matter, inducing mineral precipitation (e.g., Briggs, 2003). However, evidence for such direct mediation is rarely presented and is guided mainly by actualistic taphonomic experiments. Due to the number of articles on the various modes of fossil preservation and to reduce the overlap among experimental articles, some main and review articles were selected to compose Category 2 (Supplementary Material 2; Tables 1, 2). We consider that the very first step is to compile strategies, relying on analytical approach, to assess these challenges, thus aiming to guide future studies.

Considering Class 2a (silicification), it is noted that most studies rely on modern models of silica precipitation in association with microorganisms. Imaging and geochemical techniques are used to characterize, respectively, external structure (S), crystal morphology and texture (T) – both with approximately 75% of the total 2a articles; inorganic composition (C) – half of the 2a articles and less relevant biofilms (I) and organic (O), and isotopic (i) compositions (Table 2, Figure 4). Silica precipitation in microorganisms has a biotic component, with formation of polysaccharide as polymers evidenced by FT-IR, facilitating silica formation, and an inorganic component that is spherical nanosilica precipitation showed by SEM (Benning et al., 2004). This agrees with this habit occurring in biofilms and can be used to identify fossilized biofilms (Benning et al., 2004). Moore et al. (2021) indicated that silicification is facilitated by (1) bacterial EPS (FT-IR and EDS showed that sulphate-rich EPS facilitates silica precipitation; Si quantified by nanoSIMS); by (2) photosynthesis-based pH induces silica formation (SEM/EDS and FT-IR showed silica increase); (3) by Mg²⁺; and (4) by silica in solution. This study indicates that it is worth searching for life in silica deposits with Mg (both terrestrial and in other planets), and that combination of silica and Mg in ancient microbialite candidates can be evidence for their biogenicity. Melim et al. (2023) interpreted silicified biofilm coating trilobite sclerites as biologically mediated silicification using SEM to describe crystal morphology and identify biofilms.

Class 2b (preservation by carbonate) comprises mainly calcitization, which is fossilization by calcite and less frequently the formation of dolomite, aragonite or other carbonate minerals. All the reviewed articles from 2b used data on external morphology (S) and inorganic composition (C), and half assessed internal morphology (I) and compositional distribution (M), these being the main data to discuss the biogenicity of fossilization by carbonates (Table 2; Figure 4). The investigation of modern environments and taphonomic experiments indicate that the bacterial surface has an affinity to Ca²⁺ and to Mg²⁺, creating a coating (observed by SEM and optical microscopy) and thus preservation of bacteria by calcite (Van Lith et al., 2003). The authors suggested that this could be a criterion for bacterial mediation in calcitization. Mähler et al. (2020) performed a taphonomic experiment of muscle calcitization with associated bacteria. SEM and micro-CT showed microfabric details, while the former technique imaged soft tissues and bacteria, and Raman yielded composition.

In an extensive review, Dhami et al. (2023) compiled the biological (microbial) mediation in the formation of calcium carbonate, iron carbonate and phosphatic concretions, which comprise our Class 2c (concretions). Several imaging, geochemical, microbiology and omic techniques were reviewed to explore their potential as indicators for microbial processes mediating concretion formation (Table 2; Figure 4).

The evaluation of Class 2d (phosphatization) provides one of the most explored fossilization modes. The works comprise several geological periods and experimental taphonomy also play an important role in understanding and testing the biogenicity of phosphatization. SEM was used to characterize preserved soft tissues (S and I, respectively 80 and 60% of the articles in class 2d; Table 2; Figure 4) and associated microfabrics (Wilby and Briggs, 1997), phosphate-rich microbial mats mediating phosphatization (Wilby et al., 1996). In this latter study, total rock elemental analysis showed phosphate enrichment in microbial levels. SEM showed calcium phosphate microspheres preserving polychaete muscles and pits left after possible bacteria degradation (Wilson et al., 2016). Gäb et al. (2024) employed SEM and TEM to show that apatite formed by phosphatase enzymes resemble that found in fossils. Crosby and Bailey (2012) showed that sulfide-oxidizing bacteria form modern phosphorite deposits, though a protocol for their identification in the geological record has not been established yet.

It is long considered that biological processes play a role in the preservation by clay minerals (Class 2e). Data of external structure (S) and composition (C) are more relevant for discussing compositions (Table 2, Figure 4). Butterfield (1995) suggested that enzymatic activity during decay is hampered by clay minerals, which would have facilitated the aluminosilicification of Cambrian fossils. Taphonomic experiments are consistent in showing that certain clay minerals are more efficient in soft-tissue preservation, specifically kaolinite (Wilson and Butterfield, 2014), as it slows decay in preventing bacterial proliferation (Briggs and McMahon, 2016, and references therein). This observation explains Burgess Shale-type preservation preferentially in originally kaolinite facies (Anderson et al., 2018, 2021). Corthésy et al. (2024) further used microbial community characterization/genetic sequence associated with decaying shrimps in different clay substrates, to show that kaolinite has the lowest bacterial diversity, particularly of bacteria that efficiently decay polysaccharides of the skeletons. Becker-Kerber et al. (2021) applied a suit of techniques to Ediacaran macrofossils, suggesting microbial mediation of clay mineral precipitation after volcanic material alteration.

Class 2f (pyritization) is also a well-explored taphonomic process, much focused on the understanding of microbial mediation in mineralization. To this end, more than half of the articles use data on external morphology (S) and inorganic composition (C), aided to a lesser extent by texture (T) and mapping data (M) (Table 2; Figure 4). Taphonomic experiments have been focused on understanding geochemical conditions controlling distinct pyrite habits and textures formed during plant decay with the mediation of sulphate-reducing bacteria in anoxic conditions (Grimes et al., 2001; Brock et al., 2006). Experiments showed the formation of FeS black films coating shrimp carcasses under microbial consortium of sulphate-reducing, sulphide-oxidizing, and fermentative bacteria (Sagemann et al., 1999). The controlled decay of carcasses simulating the preservation of Ediacaran soft-bodied macrofossils enlightened the role of biofilms in mediating the precipitation of authigenic combination of Fe/S (iron sulphides)? and Al/K/Mg (aluminosilicates)? (Darroch et al., 2012), as shown in the fossil record (Laflamme et al., 2011). In this study, SEM was applied to determine crystal morphology (S and T) and EDS and XPS to characterize chemical composition (C).

Associated to class 2f, the high-resolution characterization of mineral textures in association to biofilms, Class 2g, is still poorly-explored, with the exception of a few studies like that of MacLean et al. (2008), that employed SEM/EDS and FIB-SEM to describe the textural relationship between biofilms and pyrite nanocrystals forming framboids and biofilms (Class 2g), plus STXM, NEXAFS and XPEEM to yield the organic composition (O) of biofilms and sulphur isotopic (i) composition of pyrite, altogether confirming pyrite biogenicity. Several studies have used sulphur isotopes to test the biogenicity of pyritization, and to describe the sequence of pyritization (Briggs et al., 1991; Farrell et al., 2009; Schiffbauer et al., 2014; Georgieva et al., 2022). In some of these studies, SIMS has been proved to be a powerful tool in enabling in situ nano-/micro-measurements. Xiao et al. (2010) showed that rapid pyrite precipitation dropped pH yielding silicification, then forming chert nodules encasing fossil embryos. SEM work in fossil insects from the Jehol Biota (China) and from the Crato Formation (Brazil) has demonstrated preservation by framboidal pyrite in association with biofilms (Wang et al., 2012; Osés et al., 2016; Dias and Carvalho, 2022).

Preservation by Category 2h (Fe (III) (oxyhydr(oxides)) has demonstrably been attributed to biological mediation, for this, three quarters of the articles used morphology (S and I) and composition (C) data. Li et al. (2013) demonstrated that Fe (II)-oxidizing bacteria can precipitate iron (III) (oxyhydr)oxides, either mineralizing EPS or the bacteria themselves. Experiments using TEM and geochemical techniques showed that the formation and excretion of Fe, in association with organic polymers, prevents cell encrustation of iron (II)-oxidizing bacteria (Chan et al., 2011). These biosignatures can be applied to iron (II)-oxidizing bacteria candidates in the geological record, which also has implications for Astrobiology. Miot et al. (2011) found Fe-binding/oxidizing sites at the outermost region of cell membranes. SEM was used to show biofilms in plants fossilized by iron (III) oxyhydr(oxides) (Martins et al., 2022).

Evidence of biogenicity in fossilization processes (Figure 5), in general, is inferred from coating/biofilm features associated with bacterial degradation in fossil tissues (Wilson et al., 2016). Specific morphologies such as microspheres or filaments and specific habits such as framboidal pyrite (see Grimes et al., 2001; Brock et al., 2006), mineral excretions, mineral growth patterns and microfabrics can help in defining induced or influenced mineralization and possible biofilms (Wilby et al., 1996; Wilby and Briggs, 1997; Benning et al., 2004; Van Lith et al., 2003; Chan et al., 2011; Mähler et al., 2020; Melim et al., 2023). The discussion can still be complemented by organic composition or isotopic fractionation to characterize biosynthesis and metabolic processes of fossilizing microorganisms (Briggs et al., 1991; Maclean et al., 2008; Farrell et al., 2009; Schiffbauer et al., 2014; Georgieva et al., 2022). Figure 5 summarizes a protocol of how to proceed to assess biogenicity of several fossilization modes.

To test the participation of life in fossilization processes (Figure 5), the strategy could be as follows: 1) track the diagenetic history, defining which processes have led to fossilization and which occurred later; 2) evaluate whether the substrate was consumed and allowed the proliferation of biomineralizing microorganisms by means of the description of preserved biofilms, mineral textures and geochemistry; and 3) retrieve data on the original environmental conditions using an integrated stratigraphic, sedimentological and geochemistry approach, which can shed light on biogeochemical cycles conducive to fossilization. If there is sufficient evidence, the fossilization process should be defined as biotically induced/influenced.

Category 3 includes a wealth of published data that builds a toolkit to evaluate biogenicity of minerals found in fossilized skeletal metazoans. For this purpose, data are mainly required on surface morphology (S) and inorganic and organic composition (C and O) – approximately 57% of total Category 3 articles requires this type of data; complemented by texture (T), 28% of Category 3 (Table 2; Figure 6). RS and FT-IR are well-used techniques, as well as SEM-EDS and EBSD (Trueman, 2013; Cusack, 2016; Gilbert et al., 2019; Osés et al., 2022). FT-IR can be used to assess the crystallinity of biominerals to evaluate diagenesis and, consequently, the use of biominerals to biological and paleoenvironmental studies (Trueman, 2013). EBSD has been largely used to modern and extinct taxa to characterize the mineralogy and the crystallographic orientation of crystals, giving information on the biological control of biomineralization (Cusack, 2016). Osés et al. (2022) employed a multitechnique characterization of Ediacaran fossils (with OM, CL, micro-CT, SEM, RS, EBSD and EPMA), tracking diagenesis to show a primary aragonite skeletal composition, precipitated under biological control, by using EBSD and EPMA. Pérez-Huerta et al. (2018) reviewed the application of CL and of EPMA to the evaluation of diagenesis in biomineralization studies. The organic components of biomineralized skeletons have also been analyzed to test their biogenicity. Stern (1996) applied GC/GC-MS spectrometry to identify lipids found in shells of fossil mollusks, and Osés et al. (2022) used micro-Raman spectra to show amorphous carbon associates to skeleton calcite. (plus see a compilation of articles reporting organic matter preservation and isotope research of organics in fossils by Pérez-Huerta et al., 2018).

When aiming to test biomineralizing metazoan candidates, it is generally necessary to gather evidence to assess two main aspects of biomineralization in the fossil record, that are primary composition of mineralized skeletons and biological control of biomineralization (Figure 7). The first goal deals with characterizing mineral habit, size, texture, and elemental and mineralogical composition. This allows for tracking diagenesis, to rule out secondary, alteration composition and give clues of primary mineralogy or, at least, aid in targeting less altered regions to be further investigated (e.g., Zhuravlev et al., 2012; Cusack, 2016; Wood et al., 2017; Pérez-Huerta et al., 2018; Pruss et al., 2018; Osés et al., 2022). The second goal aims to differ biomineralization control from biomineralization through passive action of the organism (e.g., Pérez-Huerta et al., 2018; Osés et al., 2022). This involves interpreting to what extent texture and microstructure are linked, yielding consistent patterns in allometric studies. The second goal also involves establishing the spatial relationship between organic matter and crystals that would suggest biomineral growth at an organic template, the identification of biomolecules involved in biomineralization, the type of skeletal microstructure, nanostructure of crystals and finding evidence for a preferential orientation of crystals (Pérez-Huerta et al., 2018; Osés et al., 2022). This approach could be complemented by the identification of macromolecules, organic compounds, and their distribution within the object of study (Stern, 1996; Cusack, 2016; Osés et al., 2022), in order to understand a genetic relationship between the organic and mineral components of a fossil (Figure 7).

Therefore, this approach can be followed in three steps, as summarized in Figure 7: 1) Understand the diagenetic history: identify the processes that have modified mineral composition, morphologies, and textures, or even formed new minerals. 2) Identifying the original mineralogy. 3) Discussing the biological control of mineralization by assessing textural evidence and other lines of evidence. If there is sufficient supporting information, the fossil can be interpreted as having been formed by biominerals either formed by biologically controlled growth, or as a poorly controlled mineralization (as soft tissue-mediated mineral agglutination) or with an inconclusive biomineralizing skeletogenesis. Otherwise, preserving skeletal minerals can be proved to be totally diagenetic in origin.

Although the study objects and goals differ across the three biogenicity categories, they share a common framework for assessment (Figures 3, 5, 7), with deciphering diagenesis as the central element and the starting point. Interpreting diagenetic history – including indigenicity and syngenicity, especially for dubiofossils – is essential for evaluating biogenicity rocks (Gargaud et al., 2015; Rouillard et al., 2021). Diagenesis, understood as a biogeochemical continuum involving processes such as compaction, recrystallization, dissolution, and, in some cases, low-grade metamorphism (Milliken et al., 1978; Worden and Burley, 2009), acts as both a preservative and a transformative force, capable of incorporating abiotic and biotic signals into the rock record or erasing them entirely. Its complexity arises from the wide range of overlapping physicochemical processes (e.g., compaction, recrystallization, authigenesis) and the prolonged timescales involved, which often lead to overprinted or ambiguous signatures (Milliken et al., 1978; Briggs, 2003; Worden and Burley, 2009; Schiffbauer et al., 2007; Boggs, 2009; Knoll, 2013; Muscente et al., 2017; Saldanha et al., 2023). This complexity makes replicating diagenetic pathways in laboratory settings particularly difficult (Briggs and McMahon, 2016). The following discussion explores how these challenges manifest across the categories analyzed in this review.

This compilation highlights the pivotal role of paleometry in studies of biogenicity. Notably, only a small fraction of the reviewed articles relies solely on one category of data (Table 2). Among these, only the 2d class is characterized by the exclusive use of morphological data (see Table 2; Supplementary Material 2). Moreover, fewer than one-quarter of the studies employed one or no high-resolution analytical technique (Table 1), emphasizing the broader value of paleometry, of in employing more than one high-resolution technique and the need to integrate data to extract more precise information from the fossil record (Riquelme et al., 2009; Delgado et al., 2014).

As emphasized in Section 4.1, reconstructing the diagenetic history is a fundamental step in assessing the biogenicity of any paleobiological material. Traditionally, interpretations of sedimentary rock diagenesis are grounded in petrographic analysis using OM, often complemented by SEM (e.g., Ketzer et al., 2003; Worden and Burley, 2009; Worden and Morad, 2003; Cardoso et al., 2024). Reconstructing the original conditions (original scenario, original biogeochemical conditions, or original mineralogy) requires integrating stratigraphic, geochemical, and sedimentological context (e.g., variations in grain size, texture, and sedimentary structures) with results from high-resolution analytical techniques. Methods commonly used for diagenetic and geochemical characterization include OM, CL, SEM-EDS, XRD, and XRF. In the specific context of biogenicity, additional tools such as RS, FT-IR, and compositional analysis via EDS provide critical morphological, textural, and chemical data, both for the fossil and its surrounding host rock. These integrated datasets enhance our understanding of depositional environments, post-depositional weathering, and fossil-diagenetic conditions (e.g., Osés et al., 2017), thus supporting more robust and nuanced interpretations of biogenicity (Figures 3, 5, 7).

The assessment of biogenicity in paleobiological materials relies heavily on the integration of S and I and C, O, i, s data, associated secondarily with T and M providing important but secondary support (Table 2; Figure 1B). This emphasis helps explain the widespread application of high-resolution techniques such as OM, SEM-EDS, µ-RS, FT-IR, and, to a lesser extent, µ-CT. OM offers insights into I, T, M, and O; SEM-EDS covers S, I, M, and C; µ-RS and FT-IR provide C and O data linked to T and M; µ-CT enables 3D imaging of S, I, T and can infer C and M via grayscale. (see Supplementary Material 1). Most of these techniques operate at the microscale and are favored not only for their versatility in generating multiple data types, but also due to their widespread availability in academic and research settings. They typically involve minimal sample preparation, are non-destructive or minimally destructive, and offer relatively low cost and rapid processing and interpretation, features that have made them standard in paleontological research (Carlson et al., 2003; Delgado et al., 2014; Borgwardt and Wells, 2017; Pan et al., 2019).

The integration of these high-resolution methods is thus central to current biogenicity protocols. However, when microscale tools reach their resolution limits, nanoscale methods become essential (Callefo et al., 2019b; Maldanis et al., 2020). This is where synchrotron radiation (SR)-based techniques become indispensable. Techniques such as PXCT, SR-XRF, STXM, SRXTM, NEXAFS, XPEEM, SR-FT-IR, and XANES offer non-destructive, high-resolution, and low-detection-limit analyses that do not require complex sample preparation or vacuum conditions. For example, these methods can detect trace and rare earth elements in minute concentrations, aiding both in biogenicity assessments (e.g., Allwood et al., 2018) and in reconstructing paleoenvironmental and diagenetic histories (Gueriau et al., 2014; Prado et al., 2021). Beyond synchrotron-based tools, other advanced methods, such as electron microprobe, EPMA, PIXE, bulk, isotopic studies, mass spectrometry (MS, LA-ICP-MS, ICP-MS), gas chromatography (GC, GC-MS), NanoSIMS, sulfur isotope analysis, FIB, TEM, DNA sequencing, and protein sequencing (LC–MS/MS), are less frequently used but provide essential insights into biomolecular preservation and fossil diagenesis (e.g., McLean et al., 2008; Table 1). Though more specialized, these techniques significantly enhance our ability to detect and validate biogenic signals and warrant greater application in future paleobiological studies.

As observed in Figure 8, most studies analyzing fossilization processes over time primarily on the Ediacaran onwards, with some works restricted to the Mesoproterozoic These fossils, often exceptionally preserved, enable the application of various techniques at both micro- and macro-scales to understand fossilization.

The concentration of Category 1a and 1b dubiofossil studies in the Paleoarchean reflects efforts to detect early life (graphs 1a and 1b in Figure 8). However, two major obstacles hinder biogenicity recognition: (1) extensive geological overprinting (e.g., metamorphism, tectonic recycling), and (2) divergence between Archean and Phanerozoic life forms, which challenge comparisons and require more robust criteria (Buick, 1990; Wacey, 2009; McLoughlin and Grosch, 2015b; McMahon et al., 2021; Rouillard et al., 2021). These challenges fueled significant debate over early biosignatures (e.g., Brasier et al., 2002, 2004, 2015; Schopf et al., 2002, 2005, 2007, 2017; Schopf and Kudryavtsev, 2012).

Studies on silicification (graph 2a in Figure 8) concentrate in the Ediacaran–Cambrian, driven by interest in “Ediacara-style preservation.” Recent work suggests early diagenetic siliceous cements enabled preservation of soft-bodied fossils (Tarhan et al., 2025; Liu et al., 2019). Furthermore, the persistence of Ediacara-style fossilization linked to authigenic silica cementation in Cambrian strata was considered to support the view that the disappearance of the Ediacara Biota at the end of the Ediacaran was due to evolutionary rather than taphonomic phenomena (Tarhan et al., 2025). Biofilms can promote the three-dimensional preservation of macroscopic organisms in siliciclastic deposits by facilitating silica precipitation and contributing to mouldic preservation of the organisms (Slagter et al., 2022; Melim et al., 2023). Precambrian oceans were enriched in silica as biomineralizers did not promote silica uptake, becoming an important silica reservoir with the diversification of radiolarians and sponges in the Ordovician, and of diatoms in the Cretaceous (Maliva et al., 2005; Butts, 2014).

Studies on the investigation of biotic role in carbonate precipitation focus on experimental approach. However, the mediation of microorganisms in carbonate concretion formation has been subject of investigation (Dhami et al., 2023). This fossilization mode has a high potential for exceptional preservation, and therefore for the preservation of soft tissues (McCoy, 2014; Cotroneo et al., 2016). When this process is sufficiently rapid, it decreases permeability and consequently protects organic matter from significant degradation, allowing the preservation of soft tissues in a ‘closed chemical system’ (Allison and Pye, 1994; Farmer and Des Marais, 1999; McCoy et al., 2015a). This has led to the fossilization and burial of soft parts of various organisms in concretions across a vast spatiotemporal range (Marshall and Pirrie, 2013; McCoy, 2014; Trinajstic et al., 2022); As observed in graph 2c in Figure 8, concretions have a wide distribution in geological time. A factor contributing to the extensive study of fossil concretions and biogenic aspects of the process is the existence of Lagerstätten bearing concretions restricted to the Phanerozoic. These are known for representing a variety of well-preserved fossils in different paleoenvironments, ranging from hypersaline to marine, estuarine to lacustrine, and freshwater to terrestrial (Marshall and Pirrie, 2013; McCoy, 2014), although most appear to belong to transitional environments, i.e., those at the interface between marine and terrestrial realms (McCoy et al., 2015a). This may explain in part the lack of this fossilization mode in the Ediacaran, when at least metazoans were restricted to oceans, rarely encompassing shallow settings.

Phosphatization studies (graph 2d in Figure 8) are concentrated in the Jurassic–Paleogene (graph 2c in Figure 8). This process represents a critical taphonomic pathway responsible for exceptionally well-preserved fossils, including soft tissues and cellular structures (Briggs, 2003). According to Dornbos (2011), phosphatization is an extremely rare taphonomic window that generally depends on the formation of favorable microenvironments except during the two major pulses of global phosphatization during the Phanerozoic: Cambrian-Ordovician and Cretaceous-Eocene. The latter coincides with widespread euxinic seas and Tethyan transgressions (Ahmed and Kurzweil, 2002), favoring phosphate preservation and resulting in several Konservat-Lagerstätten (Dornbos, 2011) and explaining the highest occurrence of research related to phosphatization processes is during the Mesozoic.

The study of the biogenicity of clay mineral preservation (graph 2e in Figure 8) concentrates in the Ediacaran (Becker-Kerber et al., 2021) and mostly in the Cambrian Burgess Shale-type preservation (Anderson et al., 2018, 2021). In the former case, the authors argued for the role of volcanic material to clay precipitation, while in the latter, diagenetic, paleogeographic and climatic controls favoured this preservational mode (Muscente et al., 2017; Anderson et al., 2018).

As previously stated, exceptionally well-preserved fossils tend to be studied more due to the amount of information that can be retrieved from them. This is the same for the process of pyritization, a rapid process that account for soft-tissue preservation in several Konservat-Lagerstätten (Cai et al., 2012; Briggs et al., 1991; Farrell et al., 2013; Farrell, 2014; Liu, 2016; Liu et al., 2019; Wang et al., 2012; Osés et al., 2016, 2017). Pyritization (graph 2f in Figure 8) is well represented in the Ediacaran, Ordovician, and Cretaceous, often preserving soft tissues via early authigenic pyrite (e.g., Liu, 2016; Briggs et al., 1991). Examples include the “death-mask” model (Callow and Brasier, 2009), Beecher’s Trilobite Bed (Farrell et al., 2013), and the pyritized fossils of the Araripe and Jehol biotas (Osés, 2016; Wang et al., 2012; Osés et al., 2016, 2017; Dias and Carvalho, 2022). Ocean redox evolution may explain temporal trends, with modern pyritization increasingly limited to anoxic freshwater settings (Bowyer et al., 2017; Thompson and Kah, 2012). The progressive ventilation of oceans through the Phanerozoic, pyritization became more restricted to lacustrine settings with anoxic conditions (Osés et al., 2017; Wang et al., 2012).

The investigation of the role of biofilms in fossilization (graph 2g in Figure 8) are focused on Cretaceous deposits bearing pyritized fossils (Wang et al., 2012; Osés et al., 2016). Meanwhile, studies on oxy(hydr)oxide preservation (graph 2h in Figure 8) remain limited, likely due to difficulties in distinguishing primary from secondary Fe-minerals (Martins et al., 2022).

Finally, biomineralization in metazoans (Figure 8) has been explored mainly in the Ediacaran (Wood et al., 2018), Cambrian (Marshall, 2006), and during the Great Ordovician Biodiversification Event (GOBE; Servais et al., 2023). These biological radiations necessitate refined biogenicity criteria for skeletal remains. Expanding this refinement to other geological periods, specifically the determination of primary mineralogy and the testing of biological controls on biomineralization, will deepen knowledge and determine its controlling factors on a geological scale.

The protocols proposed here offer a flexible and evolving framework to guide future discussions on the origin and biogenicity of materials, with the aim of deepening and structuring the debate across multiple scientific contexts. They support the identification of high-resolution analytical tools with broad applicability and help reveal methodological gaps, encouraging the integration of more specialized techniques where current approaches are insufficient.

Crucially, these protocols are not limited to paleontology. They can be applied to: (a) ancient fossil records; (b) modern and ancient abiotic structures; (c) experimental taphonomy; (d) studies on life in extreme environments; and (e) astrobiology and the search for extraterrestrial life. Their adoption promotes a systematic and reproducible approach to biogenicity, reducing reliance on isolated case studies and addressing the knowledge gap in abiotic products, which often limits balanced evaluation of biotic vs. abiotic origins (McMahon et al., 2021).

More specifically, the application of biogenicity assessment frameworks in modern extreme environments, such as ophiolites, hydrothermal vents, and acid lakes (McMahon and Ivarsson, 2019; Merino et al., 2019), can provide critical insights into the origin of mineralization processes and related products. Additionally, astrobiology would benefit from structured protocols to evaluate potential biosignatures on other planetary bodies. Dubiofossil-like features, including mineral structures, ichnofossil-like traces, or microfossil analogs, may eventually be detected elsewhere (e.g., Baucon et al., 2020), demanding a systematic and reproducible biogenicity assessment framework comparable to those used for dubiofossils on Earth. Ultimately, integrating these protocols into future research will not only refine biogenicity criteria but also contribute to a more robust and interdisciplinary dialogue, connecting paleobiology, geochemistry, experimental taphonomy, and planetary science.