Biochemical characteristics of organic matter in a guano concretion of late miocene or pliocene age from manchester parish in Jamaica.

The biogeochemical fate of organic matter (OM) entering soils is an important issue that must be examined to better understand its roles in nitrogen cycling and as a natural modulator of soil-atmospheric carbon fluxes. Despite these critical roles, there are uncertainties in estimating the contribution of this feedback mechanism due in part to a lack of molecular-level information regarding the origin and labile and refractory inventories of OM in soils. In this study, we used a multi-analytical approach to determine molecular-level information for the occurrence and stabilization of OM in a bird guano concretion of the Late Miocene or Pliocene age in Jamaica. We determined the specific organic structures persisting in the concretion and the possible contribution of fossil organic matter to the OM pool in modern environments. Our results indicate that aliphatic species, presumably of a highly polymethylenic nature [(CH2)n], may significantly contribute to the stable soil-C pool. Although not as significant, proteins and carbohydrates were also enriched in the sample, further suggesting that fossil organic matter may contribute to carbon and nitrogen pools in present day soil organic matter.

Introduction

Soil organic matter (SOM) is a complex heterogeneous mixture of various biomolecules predominantly of plant and microbial origin.1,2 Traditionally, studies on SOM have focused on its role in soil fertility and other related soil characteristics; however, in recent decades, the role of SOM as a natural modulator of soil-atmospheric carbon fluxes has emerged as a critical area of research. Despite this shift in the conventional paradigm, knowledge of the biochemical composition and dynamics of SOM, including the carbon and nitrogen biogeochemical cycles, is based on the prerequisite that organic matter (OM) occurring in soils originates exclusively from current biomass. Conversely, the contribution and biochemical fate of fossil organic matter (FOM) to the modern SOM inventory is less well-documented and is poorly understood.3–6 Therefore, to provide more accurate estimates of the soil-atmospheric carbon flux as well as the size and availability of the labile nitrogen pool to plants for predicting fertilizer requirements, it is important to first examine the biochemical contribution of FOM to the SOM inventory. FOM entering soil, sediment, and river environments is often released by the weathering and erosion of sedimentary and metamorphic rocks.3,7,8

Given the uncertainties regarding the elusive “missing carbon sinks”, the size of labile and refractory SOM pools, and the dynamics of carbon and nitrogen in these pools, it is important to delineate the possible contribution of FOM to the SOM pool. Further, it has been suggested that increases in CO2 levels are expected to continue in the next decades, even if stringent cuts in fossil fuel emissions are implemented worldwide.8 Therefore, accurate molecular-level information about the origin of FOM, its role in the biogeochemical cycling of carbon, and processes involved in its release and transformation is necessary to provide better estimates of soil-atmospheric CO2 fluxes. It is important to note that in addition to inputs, the composition and dynamics of biomolecules in soils are influenced by a wide range of biotic and abiotic factors. These include bioturbation, oxidation, microbial- and photo-degradation, hydrolysis, and weathering.9

Many of the biomolecules present in OM are reactive and are subjected to readily discernible modifications to their original molecular structure as a consequence of degradation reactions, thus allowing biogeochemical reaction sequences to be examined.10,11 As an example, lipids demonstrate a strong preservation potential, structural specificity, and readily discernable structural modifications in OM,11,12 and may be used to trace the origin, chemical history, and biogeochemical dynamics of OM in soils. Similarly, Copard et al3 used fossilized geochemical markers to confirm the contribution of fossilized organic carbon (FOC) in present-day soil and river environments. Together, this information may be used to provide clues about the processes underpinning carbon and nitrogen cycling.

When considering the structural aspects of OM, it is important to examine the contribution of the various compound classes. Here we employ Fourier transform infrared (FT-IR) spectroscopy, high-resolution-magic angle spinning nuclear magnetic resonance (HR-MAS) spectroscopy, and gas chromatography mass spectrometry (GC-MS) to provide molecular-level information on the occurrence and stabilization of OM in a bird guano concretion of the Late Miocene or Pliocene age from the Manchester Parish in Jamaica. Particularly, we examined which specific organic structures persisted in the concretion and the possible contribution of FOM to the present-day OM pool. FT-IR spectroscopy has been successfully employed to study environmental matrices such as SOM16 and compost,17 and provides us with a non-destructive means to perform rapid molecular-level investigations of a sample. NMR spectroscopy is the single most powerful analytical technique that can be applied for the analysis of organic structures and their interactions in various environmental matrices,18 and provides useful complementary and confirmatory data regarding specific biochemical components that persist and are available for release into the environment. Although advanced spectroscopic approaches such as HR-MAS NMR are used to yield vital data about predominant species,18–20 these methods provide less information about exact molecular composition.2 Therefore, we also examined the chemical decomposition of OM to yield smaller units amenable to GC-MS, thus providing a means for performing more informative investigations about the biochemical nature of the OM pool in the sample.

Methods

Sample and sample preparation

A guano concretion, previously described in Garrett et al,21 was obtained from a goethite-rich bauxitic soil in Spitzbergen (18.1268°N, 77.4957 W and altitude 732 m) in the Manchester Parish, Jamaica. Upon receipt, the sample was thoroughly cleaned by consecutive washes with large amounts of distilled and deionized water and then oven-dried at 60 °C. Next, the concretion was subdivided, ground to a fine consistency, and sieved through a stainless steel sieve with a 2-mm aperture. Duplicate samples (15 g each) of the sieved homogenized guano concretion were exhaustively extracted with 0.1 M NaOH (each time using 30 mL), the extract filtered through 0.22-μm Durapore membrane filters (Millipore, Billerica, MA, USA) under nitrogen atmosphere, cation-exchanged [Amberlite (Rohm and Haas, Philadelphia, USA) IRC-50 (H)] to remove the Na+ and then freeze-dried.

FT-IR analysis

The FT-IR spectrum of the sample was recorded on a PerkinElmer FT-IR Spectrum GX Spectrometer (Waltham, MA, USA). Approximately 1.0 mg of freeze-dried OM extracted from the sample was homogenized in 100 mg of spectroscopic-grade KBr with a refractive index of 1.559 and a particle size of 5–20 μm (Sigma, St. Louis, MO, USA) and used to create a disc-like potassium bromide (KBr) pellet for analysis. Background KBr spectra were obtained and spectra were compared to the background. Spectra were recorded by accumulating 256 scans (to increase the signal-to-noise ratio) in the 4000 to 400 cm−1 mid-infrared spectral range in the absorbance mode with a resolution of 4 cm−1. Baseline correction was conducted using the automatic baseline correction method. Samples were analyzed immediately after preparation to minimize water absorption onto the hydroscopic KBr that may have obscured key signals from the sample or lead to misinterpretation of signals.22

High-resolution magic angle spinning (HR-MAS) NMR

Thoroughly dried organic extract (~15 mg) was placed in a 4 mm zirconium oxide rotor and 1 mL D2O was added and titrated to pH 13.1 using NaOD (40% by wt) to ensure complete solubility. It is essential to dry the samples thoroughly and use only ampules of NaOD or D2O to prevent a large water peak often centered at ~3.3 ppm that can obscure many actual OM signals. After homogenization of the sample using a stainless steel mixing rod, the rotor was doubly sealed using a Kel-F (Bruker) sealing ring and a Kel-F rotor cap. 1H HR-MS NMR spectra were acquired using a Bruker 500 MHz Avance spectrometer (Billerica, MA, USA) fitted with a 4-mm triply tuned 1H-13C-15 N HR-MS probe fitted with an actively shielded Z gradient at a spinning speed of 10 kHz. 1H NMR was acquired while simultaneously decoupling both 13C 15 N nuclei. Scans (256) were acquired with a 2-s delay between pulses, a sweep width of 20 ppm, and 8 K time domain points. Basic spectral assignments were verified by two-dimensional (2D) experiments such as heteronuclear single quantum coherence (HSQC) and 1H–1H total correlation spectroscopy (TOCSY) of actual biopolymers (data not shown). Spectral predictions were also carried out using Advanced Chemistry Development’s ACD/SpecManager and ACD/2D NMR Predictor using Neural Network Prediction algorithms (version 10.02). Parameters used for prediction including line shape, spectral resolution, sweep width, and spectrometer frequency were set to match those of the real datasets as closely as possible.18

Sequential solvent extraction

Solvent extraction

Total solvent extraction of the concretion followed the protocol described by Otto et al23 with some modifications. Powdered sample (15 g) was sonicated twice for 15 min, each time with 30 mL double-distilled water to remove highly polar water-soluble compounds. Water extracts were centrifuged at 1048 xg for 30 min, decanted, and the combined extracts freeze-dried and stored at −20 °C for further analyses. The water extracted residue was freeze-dried to remove excess water and then extracted with solvents as follows: samples were sonicated twice for 15 min with 30 mL methanol, then 30 mL dichloromethane:methanol (1:1; v/v), followed by 30 mL dichloromethane. The combined total solvent extracts (“free lipids”) were filtered through glass fiber filters (Whatman GF/A, Kent, UK) using a Buchner apparatus, concentrated by rotary evaporation, and dried completely in 2 mL glass vials under a constant stream of nitrogen gas. Solvent-extracted residues were air-dried in preparation for base hydrolysis.

Base hydrolysis

Air-dried solvent-extracted residues were refluxed for 3 h using 30 mL of 1 N methanolic KOH. The samples were allowed to cool, centrifuged for 30 min at 1048 xg, and the supernatant decanted into a glass round-bottom flask and kept at 4 °C. Each residue was then extracted twice by sonication for 15 min with 30 mL of dichloromethane:methanol (1:1; v/v). The suspensions were centrifuged as described above and the combined supernatants were acidified to pH 1 using 6 M HCl. The extracts were dried by rotary evaporation at 40 °C under vacuum and the dried extracts resuspended in 30 mL of Milli-Q water. Base hydrolyzed products were recovered from the water phase by liquid-liquid extraction in a separation funnel with diethyl ether. Anhydrous Na2SO4 was added to the combined ether phases to remove water. The extracts were concentrated by rotary evaporation, transferred to 2-mL glass vials, and dried under a nitrogen atmosphere. The base hydrolyzed residues were air-dried and stored at −20 °C.24

Derivatization and GC-MS analysis

Derivatization of total solvent extracts was performed as described below. Dried solvent extracts were redissolved in 500 μL of dichloromethane:methanol (1:1; v/v) and aliquots of the reconstituted extracts (50 μL) were evaporated to dryness under nitrogen atmosphere. The dried residues were then converted to trimethylsilyl (TMS) derivatives in a 50 μL reaction using N,O-bis-(trimethylsilyl)trifluoroacetamide (BSTFA) and pyridine (9:1); the reaction incubated for 2 h at 70 °C. After cooling, 50 μL of hexane was added to dilute the extracts. Gas chromatography-mass spectrometry (GC-MS) analysis of the derivatized extracts was carried out an Agilent model 6890 N gas chromatograph equipped with an Agilent 5975C InertXL mass selective detector with Triple-Axis Detector (Agilent Technologies, Santa Clara, CA, USA). Individual components were separated on a HP-5MS chemically bonded fused-silica capillary column (Hewlett-Packard, Palo Alto, CA, USA). The stationary phase consisted of 5% phenyl-95% methylpolysiloxane, and the column dimensions were as follows; 0.25 mm i.d., 0.25 μm film thickness, and 30 m length. The GC operating profile consisted of an initial temperature of 65 °C for 2 min, which was ramped at 6 °C min−1 up to 300 °C and held for 20 min. Separation was achieved using high purity helium (99.9995%) as the carrier gas at a flow rate of 1.0 mL min−1. Approximately 1 μL of sample was autoinjected (Agilent 7683B autosampler) into the front inlet port of the GC with a 1:2 split ratio. The temperature of the port was maintained at 280 °C. The mass spectrometer was operated in standard electron impact mode (EI) at a scan range of m/z 50–650, the ion source and interface temperatures were set at 230 °C and 280 °C, respectively. Data acquisition and processing was carried out using the Agilent Chemstation G1701DA software package. Individual compounds were then identified using the NIST and Wiley MS data libraries incorporated with TMS derivatives.23

Results and Discussion

FT-IR spectroscopy

Extractable OM represents a complex heterogeneous mixture of biomolecules. Therefore, unlike pure compounds with characteristic sharp absorption peaks, OM extracted from the guano concretion is characterized by a series of broad bands resulting from the overlap of the absorptions of many similar functional groups (Fig. 1). In the present study, spectral assignments were consistent with those reported in the literature and represent the predominant species (not all species) in a given region, which are outlined below.

Figure 1

FT-IR spectrum of fossil organic matter extracted from a bird guano concretion of Late Miocene or Pliocene age. Major spectral assignments are consistent with data from published literature and represent the predominant species (not all species) in a given region and are assigned in the text.

A strong broad band positioned at 3427–3308 cm−1 is attributed to the presence of an abundance of v(O–H) of alcoholic or phenolic groups and v(N–H) of amide A in the sample.25 A band of weak to moderate absorption observed in the aliphatic C–H stretching region 3000–2700 cm−1 (most likely from lipids) comprises vasC–H of methyl groups (2961 cm−1), vasC–H (2929 cm−1 ), and vC–H (2856 cm−1) from methylene groups.26 A strong overlapping peak (1740–1600 cm−1 region) with a peak maximum near 1653 cm−1 can be assigned to aldehydes, v(O–C=O) of esters and carboxylic acid or v(C=O) of ketones, v(C=C) in aromatics, v(O–C=O) of metal-coordinate carboxylates, H-bonded v(C=O)27,28 and/or v(C=O) of amides, amide I band of proteins or peptides.25,29 The infrared spectrum also revealed a strong overlapping band at 1545 cm−1 attributed to the N-H in-plane bending vibration of amide II in proteins.28 A weak shoulder near 1460 cm−1 is assigned to C-H bending of CH2 and C(CH3)2 bending vibration of lipid and/or protein.25,29 Taken together, the methylene stretching and bending bands (2929–2856 and 1460 cm−1, respectively) and a weak methylene rocking band (720 cm−1) indicate a long-chain linear aliphatic structure.26,28,30 The fingerprint region from 1200–1000 cm−1 with a peak maximum at 1085 cm−1 is assigned to sugars, as well as signals (or overlaps with signals) resulting from other motions such as P=O symmetric stretching vibration of DNA.29 Note that bands downfield of 1000 cm−1 are primarily of an aromatic nature.

HR-MAS NMR spectroscopy

FT-IR spectroscopy provides a good overview of the major biochemical components present in the sample (Fig. 1). However, due to the vast spectral overlap from the heterogeneity of compounds in natural organic matter, we have applied HR-MAS NMR to clarify and confirm the assignments made from the IR spectrum. The HR-MAS NMR spectrum of guano concretion-derived OM is presented in Figure 2 and provides substantial complementary details of the major biochemical components that have been preserved in the sample. Spectral regions in Figure 2 have been assigned.20,31 The regions highlighted in brackets represent the predominant species (similar contributions from other species are present in some areas) and are broadly defined as contributions from: (1) amide signals in peptides and signals from aromatic rings including aromatic amino acid residues, some amide signals in peptides may also resonate in this area; (2) overlap region of anomeric protons from carbohydrates, protons associated with esters, protons on α carbon in peptides and double bonds; (3) other protons in carbohydrates, protons α to an ester, ether, and hydroxyl in aliphatic chains will also resonate in this region; (4) signals from various substituted methylenes and methines β to a functionality in hydrocarbons, signals from some amino acid side chains will also resonate here; (5) CH2, main chain methylene in lipids; and (6) CH3 groups. When a spectrum has a very strong protein contribution, the CH3 signal is derived mainly from methyl rich amino acids residues such as leucine, isoleucine, and valine; however, when the sample is dominated by aliphatic chains, for example in Figure 2, a considerable contribution is from aliphatic substances.20,31

Figure 2

1-D 1H HR-MAS spectra of (A) fossil organic matter extracted from a bird guano concretion of Late Miocene or Pliocene age, with that of bovine serum albumin presented for comparison (B). General regions are highlighted in brackets and may be broadly defined as: (1) amide signals in peptides and signals from aromatic rings including aromatic amino acid residues, some amide signals in peptides may also resonate in this area; (2) overlap region of anomeric protons from carbohydrates, protons associated with esters, protons on α carbon in peptides and double bonds; (3) other protons in carbohydrates, protons α to an ester, ether, and hydroxyl in aliphatic chains will also resonate in this region; (4) signals from various substituted methylenes and methines β to a functionality in hydrocarbons, signals from some amino acid side chains will also resonate here; (5) CH2, main chain methylene in lipids; (6) CH3 groups; aa = amino acids; and (i) mainly aromatic residues.

It is evident that the 1-D NMR spectrum is dominated by signals from aliphatic lipids (regions 5 and 6), suggesting these compounds are selectively preserved and may be a major contributor to the soil-C pool. This enrichment of aliphatic lipids in the sample may be due in part to their hydrophobic nature, which prevents transport and as a result, lowers the contact with degrading microbes and other biotic and abiotic factors, allowing them to remain in the sample for longer periods of time. Additionally, aliphatic enrichment may be due in part to the degradability of the readily bioavailable dissolved or water-extractable OM fraction. This is consistent with the observation that alkyl-C, such as those in polymethylenic structures, is the most recalcitrant form of organic carbon found in non-living SOM.32,33 Such structures have also been found in the resistant biopolymers of algae.34 Further, several recent studies focusing on the adsorption of OM to clay mineral surfaces have demonstrated the aliphatic nature of clay-organo interactions.35–38 Such interactions should not be excluded from the enrichment of aliphatic species in the sample. Although not as significant as aliphatic lipids, there is some evidence to suggest that carbohydrates have been preserved in the sample. This is somewhat surprising since the conventional view is that labile substrates such as carbohydrates are rapidly mineralized by degrading microbes. It is probable that the preservation of carbohydrates in the sample is linked to modifications by other biomolecules such as lipids or proteins. For instance, recalcitrant lipopolysaccharides are thought to be a large component of the surviving carbohydrates entering the SOM pool.2,18,31

Similarly, the presence of proteins/peptides (region 1) in the sample is somewhat unexpected. Proteins/peptides have been confirmed by the spectral similarity shown in Figure 2B (protein standard bovine serum albumin) to that of the 1D 1H NMR spectrum of the sample (Fig. 2A), for which contributions from protein/peptide structures such as amide (N-H), aromatic amino acids (aa), and α-protons are easily distinguished. Traditionally, proteins are thought to be labile in the environment; therefore, it is not immediately clear whether specific proteins presented here are resistant to degradation due to their intrinsic molecular structure, as is the case for membrane proteins,39 or environmentally induced modifications of their quaternary structures and physico-chemical (charge and hydrophobicity/hydrophilicity) and biochemical characteristics. For example, the biorefractory nature of signals resonating from lipoproteins (region 4) has previously been demonstrated.31 Additionally, protein preservation could include abiotic processes such as condensation reactions, which are known to reduce degradability.42 Similarly, sorptive protection offered by mineral matrix may be an important factor in the long-term stabilization of proteins/peptides. It has been suggested that this form of association with clay minerals may result in OM being isolated in microenvironments where it could be protected from decomposers.43 It is also intriguing to suggest that proteins/peptides survived as products of humification catalyzed clay-mediated reactions before concretion of the sample. This suggestion is favored since proteins/peptides are structurally and biochemically versatile biomolecules (they contain both cationic and anionic functional groups as well as hydrophilic and hydrophobic residues) and have demonstrated a strong affinity for clay mineral surfaces.37,38 Additionally, anoxic soil conditions may have also contributed to the overall stability of OM in the sample as fossilization occurred. Whatever the case, these results further suggest that FOM may be an important contributor to carbon and nitrogen pools in present-day SOM.

Lipid analysis

To further understand the nature of the dominant lipid fraction in the sample, we performed GC-MS analysis of silylated lipid extracts. The major classes of compounds contained in the fractions obtained from sequential extraction of the sample included a series of n-alkanoic acids (n-C7, n-C16, n-C18), α-alkanedioic acids (C3–C9) with a slight even-over-odd predominance, and α-hydroxyalkanoic acids (C3–C6) with both normal- and iso-branched structures. Branched-chain [iso-(C4) and anteiso-(C5)] fatty acids were also detected in the base-hydrolyzed sample at relatively low levels (Table 1). Other compounds detected in the sample in trace amounts included two proteinogenic amino acids (L-enantiomers), glycine and proline, the amino acid degradation product urea, the branched chain fatty alcohol 5-nonanol, a low-molecular- weight organic acid (acetic acid), and a series of normal and substituted benzoic acid (phenylalkanoic acids). The dominant compound in the extracts was C3 alkanedioic acid (Fig. 3), while α-alkanedioic acids represent the dominant class of compounds in the sample.

Table 1

Occurrence of identified compounds in fractions obtained from sequential extraction of a fossilized bird guano.

Compound	MW	Compositiona	CAS number
n-Alkanoic acids
Heptanoic acid	130	C7H14O2	111-14-8
Hexadecanoic acid	256	C16H32O2	57-10-3
Octadecanoic acid	284	C18H36O2	57-11-4
n-Alkanedioic acids
Propanedioic acid	104	C3H4O4	141-82-2
Butanedioic acid	118	C4H6O4	110-15-6
2-Methylbutanedioic acid	132	C5H8O4	498-21-5
3-Methylpentanedioic acid	146	C6H10O4	626-51-7
Hexanedioic acid	146	C6H10O4	124-04-9
Octanedioic acid	174	C8H14O4	505-48-6
Nonanedioic acid	188	C9H16O4	123-99-9
Hydroxyalkanoic acids
α-Hydroxypropanoic acid	90	C3H6O3	50-21-5
2-Methy-2-hydroxypropanic acid	104	C4H8O3	594-61-6
3-Methylpentanoic acid	116	C6H12O2	105-43-1
4-Methylpentanoic acid	116	C6H12O2	646-07-1
4-Methyl-2hydroxypentaanoic acid	132	C6H12O3	13748-90-8
α-Hydroxyhexanoic acid	132	C6H12O3	6064-43-7
Other compounds
Urea	60	CH4N2O	57-13-6
Acetic acid	60	CH4N2O	64-19-7
Glycine	75	C2H5NO2	56-40-6
Proline	115	C5H9NO2	147-85-3
Benzamide	121	C7H7NO	55-21-0
Benzoic acid	122	C7H6O2	65-85-0
4-Hydroxybenzoic acid	138	C7H6O3	99-96-7
5-Nonanol	144	C9H20O	623-93-8
Benzenepropanoic acid	150	C9H10O2	501-52-0

Note:

Compounds are presented without the TMS group for simplicity and ease of interpretation.

Figure 3

Representative GC-MS chromatograms (TIC) of fractions obtained from sequential solvent extraction of a bird guano concretion of Late Miocene or Pliocene age. (A) Free lipids and (B) bound lipids (base hydrolysate). * denotes n-alkanoic acids and • denotes n- alkanedioic acids.

It has been hypothesized that, in the environment, the reactivity and therefore lability of aliphatic chains increases with their degree of unsaturation; hence, it is not surprising that we did not detect n-alkenoic acids in the combined lipid extracts. Hydroxylation of unsaturated carbon centers may have resulted in the disappearance of n-alkenoic acids and a concomitant increase in the number of hydroxyl FAs in the sample. If this hypothesis is correct, it would account in part for the hydroxyl FAs detected in the sample (Table 1). Additionally, unsaturated FAs may have been oxidized to their respective epoxy acids (epoxidation). However, epoxides have been found to be very labile,45 which may therefore explain why they were not detected in the sample. Epoxides may further undergo hydrolysis to yield mono- and/or di-hydroxyacids; however, we did not detect di-hydroxyacids in the sample. Similarly, the lack of compounds of the class n-alkanes in the sample was not unexpected since compounds of this class are typically among the first to degrade. The dominance of compounds ≤12 C long in the sample was somewhat surprising as it has been demonstrated that the degradation rate constant of short-chain FAs is twice that of their longer-chain counterparts.47

Although not present in significant diversity or relative abundance, there is still sufficient evidence to support the recalcitrance of guano-derived lipids in this study. This recalcitrance may be due in part to the molecular structure, cross linkages, and various mechanisms of protection offered by minerals. The roles of specific mineral components (Fe, Al, and Si) in clay-organo interactions have been previously suggested.38 Further, selective preservation of shorter chain FAs after degradation may be linked to chemical modification by polar cellular components, such as amino acids and carbohydrates, as is consistent with lipoproteins and lipopolysaccharides, respectively. Such biomolecules have been shown to resist decomposition in soil microbial biomass and leachates.31 The biorefractory nature of n-C16, n-C18 in dissolved organic matter (DOM) and soil has been previously demonstrated48 and may explain the relative abundance of these compounds detected in the sample. Further, hexadecanoic acid (n-C16) may have accumulated since it is a key intermediate of oleic acid (n-C18) degradation.

Conclusion

The biochemical contribution of FOM to the SOM inventory is important and must be considered in order to provide more accurate estimates of the soil-atmospheric carbon flux as well as size and availability of the labile nitrogen pool to plants so as to predict fertilizer requirements aimed at improving nitrogen use efficacy. Molecular-level investigations were carried out to determine the possible contribution of FOM to the OM pool in soils. The results indicate the occurrence of major biochemical components (proteins, carbohydrates, and various classes of lipids) in a guano concretion. Although not a quantitative approach, this study provides a useful molecular-level descriptor of FOM components preserved in a concretion synonymous with that of sedimentary rocks. Therefore, it is probable that fossil components preserved in the concretion are available for release by weathering and erosion, eventually becoming integrated into the recent SOM pool. These findings also further highlight uncertainties in our knowledge of SOM inventory and its role in regulating natural and anthropogenic changes to global carbon and nitrogen biogeochemical cycles. Therefore, if we are to realistically address these and related concerns, further studies are needed to decipher the fate of FOM in the environment and establish a link between FOM in soils, sediments, and rivers as well as the carbon and nitrogen biogeochemical cycles.

Mass spectra of selected compounds (with and without TMS) identified from sequential solvent extraction of a guano concretion of Late Miocene or Early Pliocene age from Manchester Parish in Jamaica. (A) Nonanol-5-TMS showing characteristic fragment ion peaks at m/z 73 and 159 resulting from Si(CH3)3 and C8H19OSi fragment ions, respective; (B) 5-nonanol showing characteristic fragment ion peaks at m/z 69 and 87, and are attributed to C5H9 and C5H11O fragment ions, respectively; (C) octadecanoic acid-TMS showing prominent fragment ions at m/z 73 and 132 which have been generated by Si(CH3)3 and C5H12O2Si fragment ions, respectively; and (D) octadecanoic acid showing characteristic ion peaks at m/z 43 (C3H7), 73 (C3H5O), and 129 (C7H13O2).