- Open Access
Changes in mouse whole saliva soluble proteome induced by tannin-enriched diet
Proteome Science volume 8, Article number: 65 (2010)
Previous studies suggested that dietary tannin ingestion may induce changes in mouse salivary proteins in addition to the primarily studied proline-rich proteins (PRPs). The aim of the present study was to determine the protein expression changes induced by condensed tannin intake on the fraction of mouse whole salivary proteins that are unable to form insoluble tannin-protein complexes. Two-dimensional polyacrylamide gel electrophoresis protein separation was used, followed by protein identification by mass spectrometry.
Fifty-seven protein spots were excised from control group gels, and 21 different proteins were identified. With tannin consumption, the expression levels of one α-amylase isoform and one unidentified protein increased, whereas acidic mammalian chitinase and Muc10 decreased. Additionally, two basic spots that stained pink with Coomassie Brilliant Blue R-250 were newly observed, suggesting that some induced PRPs may remain uncomplexed or form soluble complexes with tannins.
This proteomic analysis provides evidence that other salivary proteins, in addition to tannin-precipitating proteins, are affected by tannin ingestion. Changes in the expression levels of the acidic mammalian chitinase precursor and in one of the 14 salivary α-amylase isoforms underscores the need to further investigate their role in tannin ingestion.
Saliva is an important fluid that rapidly adjusts to changes in dietary conditions. Salivary glands are mainly under nervous system control, and the composition of salivary secretions is rapidly altered over a wide range in response to various stimuli. Saliva serves as a physiological buffer against variations between the external and internal milieus. Such variations may be reflected in different salivary protein profiles resulting from different dietary habits. It was proposed that saliva protein composition varies also considerably among species, reflecting diverse diets and modes of digestion . Animals using identical feeding niches may present similarities in their salivary protein composition, whereas the presence of particular proteins may be specific for particular feeding niches. For example, salivary amylase levels correlate with starch levels in each animal species' diet . Moreover, salivary protein composition is modulated by diet. One example is the induction of salivary cystatins in rats ingesting capsaicin-containing diets . Studies in humans have demonstrated changes in the salivary proteome induced by different basic tastes .
Several other studies on the adaptation of salivary protein composition to diet have investigated tannins (for review, see ). Tannins are plant secondary metabolites (PSMs) found in most food and drinks of vegetable origin, with a high capacity to bind proteins, polysaccharides, carbohydrates, and other macromolecules. Particularly with proteins, tannins may form stable complexes that tend to precipitate . Tannins highly influence diet selection, and their presence may result in food avoidance attributable to either their astringent properties or detrimental post-ingestive effects .
Feeding tannins to mice and rats induces a considerable amount of a particular group of salivary proteins--the proline-rich proteins (PRPs) [8, 9]--that protect animals against the negative post-ingestive effects of tannin and appear to reduce the aversive bitter or astringent properties of tannins [8–10].
Although PRPs, and particularly those belonging to the basic subgroup, appear to be the most effective tannin-binding salivary proteins  and the first line of defense to tannin ingestion, other less abundant salivary proteins may also be affected by tannin consumption. For example, histatins constitute a group of relatively small proteins with high tannin affinity. However, their presence was only found in saliva from humans and some primates . The presence of tannin-binding salivary proteins other than PRPs has also been suggested in some herbivores, although these proteins have not been characterized .
Our group has been developing research on the relationship between salivary protein composition and dietary choice. In our previous one-dimensional electrophoresis study , we observed an increase in the expression level of one α-amylase isoform, suggesting that the effects of tannin ingestion on mouse salivary protein composition go beyond the increase in salivary PRPs. Our hypothesis is that expression of other salivary proteins would also change as a consequence of tannin ingestion. The present study sought to augment the knowledge of such putative changes in the salivary protein profile by using two-dimensional electrophoresis (2-DE) coupled with mass spectrometry. Such an approach has already been used in studies of human and small ruminant salivary proteomes, resulting in a high number of proteins identified and a more reliable protein expression comparison [14–17].
Although mouse has developed into a premier mammalian model system for exploring potential causes and treatments for human disease when human experimentation is not feasible or ethical, to our knowledge an overall characterization of this species' saliva proteome had not yet been made. Mouse saliva and salivary glands have been studied for diet-induced changes, and 2-DE maps of rodent saliva have been reported for rat parotid  and submandibular  saliva. However, no extensive protein characterization was performed in any of these studies. Mice have been used traditionally in studies concerning the complex physiological ingestive and digestive systems, and such protein characterization is important.
We used 2-DE coupled with mass spectrometry (matrix-assisted laser desorption ionization time-of-flight mass spectrometry [MALDI TOF MS] and MALDI TOF-TOF MS/MS) to characterize the mouse soluble fraction of whole saliva (SFWS) and to study the effects of tannin ingestion. The changes induced by tannin-enriched diets were assessed after tannin-protein insoluble complexes were removed. Histology of salivary gland morphology was performed to confirm the effects of tannin levels used in the experiments.
Materials and methods
Twelve inbred male Balb/c mice, five weeks of age, were obtained from the licensed bioterium of Instituto Gulbenkian de Ciência (Oeiras, Portugal). The animals were housed in type IV mouse cages (Techniplast; six mice per cage), according to European Union recommendations and the revision of Appendix A of the European Convention for the Protection of Vertebrate Animals used for Experimental and Other Scientific Purposes (ETS No. 123). Animals were maintained on a 12 h/12 h light/dark cycle at a constant temperature of 22°C with ad libitum access to water and a standard diet with 21.86% crude protein (dry basis) in the form of pellets (RM3A-P; Dietex International, Essex, UK). The animals were subjected to a 7 day acclimation period to minimize the effects of stress associated with transportation, followed by a 7 day pretrial period to allow adaptation to the ground diet used during the feeding trials. The standard pellet diet was ground daily with a blender . Before the feeding trial period, the animals were individually weighed and allocated to two experimental groups, with no significant differences in body mass (25.5 ± 1.7 g). All animal procedures were approved by the scientific committee, were supervised by a scientist trained by the Federation of European Laboratory Animal Science, and conformed with Portuguese law (Portaria 1005/92), which followed European Union Laboratory Animal Experimentation Regulations.
A 10 day experimental period was initiated immediately after the pretrial period. The control group (n = 6) received a tannin-free diet consisting of the same standard ground diet administered during the pretrial period. The quebracho group (n = 6) received the standard ground diet enriched with quebracho. Quebracho (Tupafin-Ato, SilvaChimica SRL, Cuneo, Italy) is a natural extract obtained directly from quebracho wood and is sold commercially, mainly for use in the leather industry. These extracts are commonly used in herbivore feeding studies as a model of condensed tannins (e.g., ). According to the manufacturer's information, the extract contains 72 ± 1.5% condensed tannins with a small amount of simple phenolics. This product was added to the standard diet to obtain a mixture that contained 7 g tannin/100 g wet weight, which is a dosage previously found to induce PRPs in mouse salivary glands . The diets were prepared daily, and food and water were provided ad libitum.
Saliva and salivary gland collection and sample preparation
After the 10 day feeding trial (day 11) individual mouse whole saliva secretion was induced with an intraperitoneal injection of pilocarpine and collected by aspiration from the mouth as described elsewhere . Prior to protein quantification, saliva samples were centrifuged at 16,000 × g for 5 min at 4°C to remove particulate matter and salivary proteins that could be precipitated because they form a complex with tannins. Only the soluble fraction was used for further analyses. After saliva collection, the animals were euthanized with an overdose of xylazine hydrochloride combined with ketamine hydrochloride. The parotid glands were dissected, washed briefly with 0.1 M phosphate buffer, pH 7.4, and fixed in 10% neutral buffered formalin for routine histology.
To confirm that the quebracho doses used in this study did, in fact, affect the salivary glands, parotid morphology was observed by light microscopy using a Nikon Eclipse 600 microscope (Kanagawa, Japan). After embedding the fixed parotid glands in paraffin wax using routine procedures, a series of 5 μm thick sections were cut with a microtome, and the slides were stained with hematoxylin and eosin. For each animal, 10 digital pictures from random areas of the parotid glands were collected with a Nikon DN 100 camera (Kanagawa, Japan) at 200× magnification. For each animal, the areas and perimeters of a minimum of 100 acini were randomly chosen and measured using SigmaScan Pro 5.0 software (SPSS, Chicago, IL, USA).
Separation by two-dimensional gel electrophoresis (2-DE)
The soluble fraction of whole saliva (SFWS) protein concentration was determined using the bicinchoninic acid method (Pierce, Rockford, IL, USA), with bovine serum albumin (BSA) as the standard.
Individual mouse SFWS samples (n = 6) containing 100 μg total protein were mixed with rehydration buffer . Samples were subjected to isoelectric focusing (IEF: first dimension) at 20°C in 13 cm IPG strips, pH 3-10, NL (Amersham Biosciences Europe GmbH, Freiburg, Germany) using an IPGphor Isoelectric Focusing System (Amersham Biosciences Europe GmbH, Freiburg, Germany). The following IEF program was used: 2 h at 0 V, 12 h at 30 V (active rehydration), 1 h at 200 V, 1 h at 500 V, 1 h at 1000 V, 1 h at a 1000-8000 V linear gradient, and 6 h at 8000 V. After focusing, proteins in the IPG strips were equilibrated and horizontally applied on top of a 12% sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE: second dimension) gel (1 × 160 × 200 mm) . Broad range molecular mass markers (Ref 161-0317; BioRad, CA, USA) were run simultaneously with the samples to calibrate the molecular masses of protein spots. Gels were stained with Coomassie Coloidal G-250 . Additionally, a PRP-specific stain/destain procedure  was used in some gels to assess the induction of these proteins by tannins.
Digital 2-DE gel images were acquired using a scanning densitometer with internal calibration (Molecular Dynamics, Amersham Biosciences Europe GmbH, Freiburg, Germany) with LabScan software (Amersham Biosciences Europe GmbH, Freiburg, Germany). Gel analysis was performed using Image Master Platinum v.6 software (Amersham Biosciences Europe GmbH, Freiburg, Germany). Spot volume normalization in the various 2-DE maps was performed using relative spot volumes (% vol). Spot detection was first performed in automatic mode, followed by manual editing for spot splitting and noise removal. The gel containing the greatest number of protein spots for each diet condition was chosen as the reference gel. All other gels from the same experimental condition were matched to the reference gel by placing user landmarks on approximately 10% of the visualized protein spots to assist in automatic matching. After completion of automatic matching, all matches were checked for errors by manual editing.
Stained spots were excised, washed in acetonitrile, and dried in a SpeedVac. The proteins were digested with trypsin as previously described .
Peptide mass fingerprinting
Peptide mass fingerprinting was performed as described elsewhere , with mass spectra obtained by matrix-assisted laser desorption/ionization-time of flight mass spectrometry (MALDI TOF MS) using a Voyager-DE STR (Applied Biosystems, Foster City, CA, USA) MALDI TOF mass spectrometer in the positive ion reflectron mode. Database searches were performed against SwissProt, MSDB, and NCBInr following the same criteria described previously , both to perform the search and to accept the identification.
Protein identification using MALDI TOF-TOF data
Protein identification was performed by MALDI TOF-TOF analysis using an Applied Biosystems 4800 Proteomics Analyzer (Applied Biosystems, Foster City, CA, USA) in both MS and MS/MS mode. Positively charged ions were analyzed in the reflectron mode over the m/z range of 800-3500 Da, typically using 800 laser shots per spectra and a fixed laser intensity of 3500 V. External calibration was performed using the 4700 Calibration Mix (Applied Biosystems). The 10 best s/n precursors from each MS spectrum were selected for MS/MS analysis by Collision-Induced Dissociation assisted with air using a collision energy of 1 kV and a gas pressure of 1 × 106 torr. Two thousand laser shots were collected for each MS/MS spectrum using a fixed laser intensity of 4500 V. Raw data were generated by 4000 Series Explorer v3.0 RC1 software (Applied Biosystems, Foster City, CA, USA). All contaminant m/z peaks were included in the exclusion list used to generate the peptide mass list for the database search. The generated mass spectra were used to search UniProtKB (released July 7, 2009) and Uniref100 (released July 7, 2009). Searches were conducted using two algorithms: Paragon from Protein Pilot v.2.0 software (Applied Biosystems, MDS Sciex) and Mowse from MASCOT-demon v.2.1.0 software (Matrix-Science, London, UK). Protein identifications were accepted with a probability filter cutoff of 99% (Prot Score ≥ 2.0) for Paragon and 95% (p < 0.05) for Mowse. For Protein Pilot, the search parameters were the following: enzyme (trypsin), Cys alkylation (iodoacetamide), special factor (urea denaturation), species (none), and ID focus (biological modification). For Mascot, the interpretation of the combined MS+MS/MS data was performed using GPS Explorer v.3.5 software (Applied Biosystems, Foster City, CA, USA), with the following parameters: missed-cleavage (one), peptide tolerance (75 ppm), fragment mass tolerance (0.25 Da), fixed modification (carbamidomethylation of cysteine), and variable modification (methionine oxidation). Additionally, all MS/MS spectra were further analyzed with Peaks Studio v.4.5 software (Bioinformatics Solutions, Waterloo, ON, Canada) for automatic de novo sequencing combined with database searching, selecting trypsin as the enzyme and a parent and fragment mass error tolerance of 0.08 U.
Prediction of post-translational modifications
For salivary α-amylase, which was identified in several spots for which apparent molecular masses and pI differed, potential post-translational modifications (PTMs) were predicted as described previously . Briefly, FindMod (http://www.expasy.ch/tools/findmod/; accessed June 17, 2010), NetPhos 2.0 (http://www.cbs.dtu.dk/services/NetPhos/; accessed June 17, 2010), and Signal IP 3.0 (http://www.cbs.dtu.dk/services/SignalP/; accessed June 17, 2010) search engines were used. Glycosylation and phosphorylation information present in the SwissProt database were also considered. Only the predicted PTMs associated with peptides not matched to the identified protein were considered.
All data were analyzed for normality using the Kolmogorov-Smirnoff test and homoscedasticity using the Levene test. The values of salivary protein concentration were normally distributed, and independent sample t-tests were performed to assess differences between diet treatments. Spot relative volume (% vol) and parotid acinar areas and perimeters did not present normal distributions or homoscedasticity. Consequently, the differences in the expression levels between the control and quebracho groups for each protein spot and for histomorphometric data were determined using the nonparametric Mann-Whitney test. Means were considered significantly different when p < 0.05. All statistical analyses were performed using SPSS v.15.0 software (SPSS, Chicago, IL, USA).
The acinar area and perimeter of the parotid glands from the animals fed a quebracho-enriched diet were significantly higher than the control group (Table 1). Levels of 7 g tannin per 100 g wet weight in the diet produced hypertrophy of parotid gland secretory tissue (Figure 1).
Pattern of soluble fraction of whole saliva (SFWS) proteins
After the 10 day feeding trial, the protein concentration of the soluble fraction of whole saliva, measured after centrifugation and precipitate removal, was significantly lower in the quebracho group than in the control group (Table 1), indicating that a smaller amount of salivary proteins remains soluble after tannin ingestion.
A two-dimensional map of mouse SFWS was constructed with a non-linear pI range of 3-10 and a molecular mass ranging from approximately 10 to 100 kDa (Figure 2). A total of 86 protein spots were reproducibly displayed in Coomassie Colloidal G-250-stained gels, from which the 57 most intense ones were analyzed by mass spectrometry. From these, 48 protein spots, corresponding to 21 polypeptides, were identified by peptide mass fingerprinting and MS/MS (Table 2). Some proteins were identified in a high number of spots, namely salivary amylase (14 different spots), androgen binding proteins (6 different spots), and several forms of kallikreins (8 different spots). Concerning salivary amylase, glycosylation and deamidation are predicted PTMs, according to the analysis of the mass spectra and presence of consensus regions (Table 3).
Effects of quebracho consumption on SFWS protein patterns
Three protein spots were found to change significantly in terms of relative volume (Table 4). The levels of one isoform of α-amylase (spot 62) and one unidentified protein (spot 24) increased in the quebracho group, whereas the levels of acidic mammalian chitinase (spot 38) decreased. Two new protein spots (Q1 and Q2), which were not observed in the control group gels, were consistently present in the gels from the quebracho group, whereas spot 30, corresponding to Muc 10, was absent (Figure 3). For other protein spots, no statistical significant differences were determined due to high variability between individuals in their expression levels.
When both the control and quebracho gels were subjected to the Coomassie Brilliant Blue R-250 modified staining procedure for PRPs , the Q1 and Q2 spots, present at the basic extremity of the gels and with apparent molecular masses of 42 and 64 kDa, respectively, appeared with a slightly dark pink color, whereas the remaining spots appeared as blue spots in both gels (Additional file 1: supplementary Figure S1).
Using 2-DE and MS/MS, a proteome profile of mouse SFWS comprising 21 different proteins was established, extending knowledge and aiding studies on ingestive physiology and salivary secretion physiology using a mouse model.
Williams et al.  obtained 2-DE maps from rat parotid saliva using a pI range similar to that used in the present study (pH 3-10). Comparisons with our gels indicate a similar distribution for some spots, notably those we identified as α-amylase, deoxyribonuclease, parotid secretory protein, and demilune cell and parotid protein. However, several differences observed between the two patterns are not surprising because they stem from distinct genotypes (rat vs. mice) and different glandular origin secretions (parotid vs. whole saliva). The presence of basic and acidic PRPs was suggested in a rat parotid saliva 2-DE pattern . These proteins are not constitutively expressed in mouse salivary glands , but rather induced by isoproterenol administration or tannin ingestion [5, 9], which can also explain the failure to detect them in our control samples.
In the present study, different spots resulted in the identification of the same protein (Figure 2; Table 2). A similar feature was also observed in the human saliva proteome  and recently by us in small ruminant parotid saliva . This observation may be attributable to the presence of isoforms, protein fragments, or PTMs, among which glycosylation and phosphorylation were reported to be a common feature of salivary proteins [25, 26].
Fourteen spots were identified as salivary α-amylase. A high number of salivary α-amylase spots with a similar distribution has also been observed in human whole saliva [15, 16, 27], suggesting similarities between humans and mice in the digestive functions of saliva, in contrast to ruminants, which lack salivary α-amylase [17, 22]. The apparent molecular masses were approximately 58 kDa, and the pI ranged from 3.4 to 6.2. The theoretical molecular mass of the native form of α-amylase is 56 kDa, with a pI of 6.4. Glycosylation with neutral and acidic (sialic acid) oligosaccharides and spontaneous post-secretion deamidation of salivary α-amylase have been previously demonstrated [27, 28]. The consensus sequence for glycosylated asparagine residues is Asn-X-Ser/Thr; therefore, two possible N-glycosylation sites for mouse α-amylase are 427-429 and 475-477 (Table 3). These two sites were also previously mentioned for human [27, 28] salivary α-amylase. The described glycosylations may explain the higher apparent molecular mass of the α-amylase isoforms compared with the native α-amylase form and the pI differences between the several protein spots. Moreover, from the MS spectra analysis of the several spots identified as α-amylase, the absence of one or both peptides containing the consensus region for N-glycosylation was apparent, suggesting the possibility of such a PTM. No potential phosphorylations were observed for the protein spots identified as α-amylase, and the presence of the signal peptide was predicted for all of the spots.
Eight protein spots, from acidic to neutral and with several different molecular masses, were identified as five different kallikrein forms. These proteins belong to a family of serine proteases that are involved in hormone and growth factor processing . The tremendous amount and diversity of kallikreins present in mouse saliva was not previously observed using SDS-PAGE . Some authors already reported the expression of several kallikreins in mouse submandibular glands . Besides, these salivary proteins were also found in humans  and rats . The relative proportion of the various tissue kallikreins secreted by rat submandibular glands was found to be differentially influenced by the two branches of the autonomic nervous system: kallikreins in sympathetic-induced saliva were derived by exocytosis of pre-packaged granules in granular tubules, whereas kallikreins in parasympathetic-induced saliva were likely secreted through a constitutive vesicular route . In the present study, we used pilocarpine to stimulate mouse saliva secretion, and we hypothesize that the identified forms derive mainly from a constitutive vesicular route. This may be important for future studies that apply parasympathetic agonists to stimulate salivary flow and collect saliva.
When tannins were introduced in the diet, changes in mouse SFWS 2-DE profiles were observed. Tannins are generally believed to be synthesized by plants to act as deterrents because of their bitter and astringent properties [34, 35]. The challenge is to ingest plant-derived foods without suffering the ill effects of tannins. Saliva components are the first defense line against tannins, partially by minimizing their unpalatable astringent properties . Hypertrophy of parotid glands was reported in rats and mice, which coincided with a dramatic increase in salivary PRP production after 2-3 days of tannin ingestion [8, 9]. Similar results were found in the present study, where a significant increase in acinar size was observed in animals fed quebracho tannin-enriched diets.
The protein concentration of the SFWS from the quebracho group was lower compared with the control group, suggesting that the stable insoluble complexes formed between salivary proteins and dietary tannins in the mouth  were lost during the centrifugation step during sample preparation, which was intentional and allowed us to analyze the minor expressed salivary proteins.
In the present work, only one mucin was identified in mouse SFWS. Mucins represent a high proportion of salivary proteins (approximately 16% of the total proteins in human whole saliva), play a protective role, and contribute to oral coating and lubrication . The failure to identify mucins may be related to the difficulty of assessing these proteins because of their large molecular mass, high viscosity, and poor solubility in aqueous solvents . The Muc10 spot, although present in the control group, was absent in the 2-DE profile of mouse SFWS from the quebracho group. Salivary mucins can also form complexes with tannins , and Muc10-tannin complexes may have been removed during the centrifugation step.
The level of chitinase decreased in the quebracho group. The presence of this protein in mouse saliva was already observed by one-dimensional electrophoresis, but its level did not change after tannin consumption . This protein has been reported in mice  and humans [41, 42], and a digestive or defensive role against chitinous pathogens [40–42] has been proposed. Future studies may clarify the biological role of this protein in tannin ingestion.
From the protein spots that newly appeared in the quebracho group, spots Q1 and Q2 stained dark pink (Additional file 1: supplementary Figure S1), suggesting that these may be PRPs . The proteins present in these two spots were not identified by mass spectrometry. A failure in identifying PRPs by mass spectrometry was previously reported , which the authors attributed to the particular characteristics of this family of proteins. Identification of PRPs by mass spectrometry is challenging because of the primary sequence of these proteins, for which tryptic digests produce only a reduced number of high m/z values . This behavior also causes difficulties when extracting the peptides from the gel. In fact, the peptide maps for both spots are similar and poor with regard to the number of m/z peaks detected. The location of the Q1 and Q2 spots at the basic extremity of the gels is consistent with studies arguing that basic PRPs act as a defense mechanism against dietary tannins [6, 36]. Moreover, their induction was observed in salivary glands of polyphenol-fed rats  and BALB/c mice . Salivary basic PRPs have a very high affinity for tannins, leading to the formation of insoluble complexes . The observation of pink spots even after centrifugation also demonstrates the presence of free PRPs or PRP-tannin soluble complexes .
The increase in expression level of one α-amylase isoform was previously observed in mice fed tannin-enriched diets . This increase was suggested to be a co-adjuvant of the inhibition of tannin biological activity or as a response to counteract the amount of this enzyme that was potentially inactivated by tannin binding . Inhibition of salivary α-amylase by dietary polyphenols has been demonstrated , and a recent report revealed the mechanisms involved in the tannin/α-amylase interaction . The observation of changes in only one of the isoforms, previously  and in the present study, supports the hypothesis of different functional activities among the several isoforms. Further studies are needed to elucidate the functional differences between amylase isoforms.
The present study characterized the mouse saliva protein profile, which is an animal model used in studies of salivary gland physiology. Salivary protein composition correlates with systemic conditions, and the knowledge of its normal composition may elucidate the differences induced by treatments. Despite the similarities to the extensively studied human saliva protein profile, significant differences were also found, demonstrating the species specificity of saliva. Additionally, we demonstrated that mouse SFWS 2-DE profile changes in response to introducing quebracho tannins into diet, namely by increasing the expression of one salivary amylase isoform and decreasing the expression of the acidic mammalian chitinase precursor. Because these are proteins which did not precipitate tannins, they may act through an alternative mechanism to impede them to have negative effects in the digestive tract. These findings suggest that salivary proteins other than PRPs may play a role in the modulation of saliva composition according to the characteristics of ingested material. Proteomics will be useful in nutrition studies for monitoring changes in saliva composition induced by foods with particular characteristics.
Plant Secondary Metabolites
tandem mass spectrometry
- MALDI TOF:
Matrix assisted laser desorption ionization time-of-flight
bovine serum albumin
Immobilized pH gradient
Hematoxylin and Eosin
Sodium dodecyl sulphate polyacrylamide gel electrophoresis
Comassie Brilliant Blue
Soluble fraction of whole saliva
Young JA, Schneyer CA: Composition of saliva in mammalian. Aust J Exp Bio Med Sci 1981, 59: 1–53. 10.1038/icb.1981.1
Perry GH, Dominy NJ, Claw KG, Lee AS, Fiegler H, Redon R, Werner J, Villanea FA, Mountain JL, Misra R, Carter NP, Lee C, Stone AC: Diet and the evolution of human amylase gene copy number variation. Nat Genet 2007, 39: 1256–1260. 10.1038/ng2123
Katsukawa H, Shang Y, Nakashima K, Yang KH, Sugita D, Mishima K, Nakata M, Ninomiya Y, Sugimura T: Salivary cystatins influence ingestion of capsaicin-containing diets in the rat. Life Sci 2002, 71: 457–467. 10.1016/S0024-3205(02)01702-2
Neyraud E, Sayd T, Morzel M, Dransfield E: Proteomic analysis of human whole and parotid salivas following stimulation by different tastes. J Proteome Res 2006, 5: 2474–2480. 10.1021/pr060189z
Shimada T: Salivary proteins as a defense against dietary tannins. J Chem Ecol 2006, 32: 1149–1163. 10.1007/s10886-006-9077-0
Lu Y, Bennick A: Interaction of tannin with human salivary proline-rich proteins. Arch Oral Biol 1998, 43: 717–728. 10.1016/S0003-9969(98)00040-5
Iason G: The role of plant secondary metabolites in mammalian herbivory: ecological perspectives. Proc Nutr Soc 2005, 64: 123–131. 10.1079/PNS2004415
Mehansho H, Hagerman A, Clements S, Butler L, Rogler J, Carlson DM: Modulation of proline-rich protein biosynthesis in rat parotid glands by sorghums with high tannin levels. Proc Natl Acad Sci USA 1983, 80: 3948–3952. 10.1073/pnas.80.13.3948
Mehansho H, Clements S, Sheares BT, Smith S, Carlson DM: Induction of proline-rich glycoprotein synthesis in mouse salivary glands by isoproterenol and by tannins. J Biol Chem 1985, 260: 4418–4423.
Glendinning JI: Effect of salivary proline-rich proteins on ingestive responses to tannic acid in mice. Chem Senses 1992, 17: 1–12. 10.1093/chemse/17.1.1
Sabatini LM, Warner TF, Saitoh E, Azen EA: Tissue distribution of RNAs for cystatins, histatins, statherin, and proline-rich salivary proteins in human and macaques. J Dent Res 1989, 68: 1138–1145. 10.1177/00220345890680070101
Gehrke J: Investigations of tannin-binding salivary proteins of roe deer and other ruminants. PhD thesis. University of Potsdam, Potsdam (in German with English summary); 2001.
da Costa G, Lamy E, Capela e Silva F, Andersen J, Sales Baptista E, Coelho AV: Salivary amylase induction by tannin-enriched diets as a possible countermeasure against tannins. J Chem Ecol 2008, 34: 376–387. 10.1007/s10886-007-9413-z
Huang CM: Comparative proteomic analysis of human whole saliva. Arch Oral Biol 2004, 49: 951–962. 10.1016/j.archoralbio.2004.06.003
Vitorino R, Lobo MJ, Ferrer-Correira AJ, Dubin JR, Tomer KB, Domingues PM, Amado FM: Identification of human whole saliva protein components using proteomics. Proteomics 2004, 4: 1109–1115. 10.1002/pmic.200300638
Walz A, Stühler K, Wattenberg A, Hawranke E, Meyer HE, Schmalz G, Blüggel M, Ruhl S: Proteome analysis of glandular parotid and submandibular-sublingual saliva in comparison to human whole saliva by two-dimensional gel electrophoresis. Proteomics 2006, 6: 1631–1639. 10.1002/pmic.200500125
Lamy E, da Costa G, Santos R, Capela e Silva F, Potes J, Pereira A, Coelho AV, Sales Baptista E: Sheep and goat saliva proteome analysis: a useful tool for ingestive behavior research? Physiol Behav 2009, 98: 393–401. 10.1016/j.physbeh.2009.07.002
Williams KM, Ekström J, Marshall T: High-resolution electrophoretic analysis of rat parotid salivary proteins. Electrophoresis 1999, 20: 1373–1381. 10.1002/(SICI)1522-2683(19990601)20:7<1373::AID-ELPS1373>3.0.CO;2-Z
Yamada A, Nakamura Y, Sugita D, Shirosaki S, Ohkuri T, Katsukawa H, Nonaka K, Imoto T, Ninomiya Y: Induction of salivary kallikreins by the diet containing a sweet-suppressive peptide, gurmarin, in the rat. Biochem Biophys Res Comm 2006, 346: 386–392. 10.1016/j.bbrc.2006.05.154
Voltura MB, Wunder BA: Physiological responses of the Mexican woodrat ( Neotoma mexicana ) to condensed tannins. Am Midl Nat 1994, 132: 405–409. 10.2307/2426598
Blakesley RW, Boezi JA: A new staining technique for proteins in polyacrylamide gels using coomassie brilliant blue G-250. Anal Biochem 1977, 82: 580–582. 10.1016/0003-2697(77)90197-X
Beeley JA, Khoo KS, Lamey PJ: Two-dmensional electrophoresis of human parotid salivary proteins from normal and connective tissue disorder subjects using immobilised pH gradients. Electrophoresis 1991, 12: 493–499. 10.1002/elps.1150120707
Lamy E, da Costa G, Capela e Silva F, Potes J, Coelho AV, Baptista ES: Comparison of electrophoretic protein profiles from sheep and goat parotid saliva. J Chem Ecol 2008, 34: 388–397. 10.1007/s10886-008-9442-2
Hirtz C, Chevalier F, Centeno D, Egea JC, Rossignol M, Sommerer N, de Périère D: Complexity of the human whole saliva proteome. J Physiol Biochem 2005, 61: 469–480. 10.1007/BF03168453
Ramachandran P, Boontheung P, Xie Y, Sondej M, Wong DT, Loo JA: Identification of N-linked glycoproteins in human saliva by glycoprotein capture and mass spectrometry. J Proteome Res 2006, 5: 1493–1503. 10.1021/pr050492k
Messana I, Inzitari R, Fanali C, Cabras T, Castagnola M: Facts and artifacts in proteomics of body fluids. What proteomics of saliva is telling us? J Sep Sci 2008, 31: 1948–1963. 10.1002/jssc.200800100
Hirtz C, Chevalier F, Centeno D, Rofidal V, Egea JC, Rossignol M, Sommerer N, Deville de Périère D: MS characterization of multiple forms of alpha-amylase in human saliva. Proteomics 2005, 5: 4597–4607. 10.1002/pmic.200401316
Bank RA, Hettema EH, Arwert F, Amerongen AV, Pronk JC: Electrophoretic characterization of posttranslational modifications of human parotid salivary alpha-amylase. Electrophoresis 1991, 12: 74–79. 10.1002/elps.1150120114
Blaber M, Isackson PJ, Bradshaw RA: A complete cDNA sequence for the major epidermal growth factor binding protein in the male mouse submandibular gland. Biochemistry 1987, 26: 6742–6749. 10.1021/bi00395a025
Blaber M, Isackson PJ, Holden HM, Bradshaw RA: Synthetic chimeras of mouse growth factor-associated glandular kallikreins. II. Growth factor binding properties. Protein Sci 1993, 2: 1220–1228. 10.1002/pro.5560020804
Jenzano JW, Su HW, Featherstone GL, Lundblad RL: Molecular diversity of tissue kallikrein in human saliva. Agents Actions Suppl 1992, 38: 137–144.
Bedi GS: The effects of autonomic drugs on the concentration of kallikrein-like proteases and cysteine-proteinase inhibitor (cystatin) in rat whole saliva. J Dent Res 1991, 70: 924–930. 10.1177/00220345910700051201
Garrett JR, Proctor GB, Zhang XS, Anderson LC, Shori DK: Constitutive secretion of kallikreins in vivo from rat submandibular glands. Eur J Morphol 1998, 36: 86–91.
Haslam E, Lilley TH: Natural astringency in food stuffs - a molecular interpretation. Crit Rev Food Sci Nutr 1988, 27: 1–40. 10.1080/10408398809527476
McArthur C, Hagerman AE, Robbins CT: Physiological strategies of mammalian herbivores against plant defenses. In Plant defenses against mammalian herbivory. Edited by: Palo RT, Robbins CT. Boca Raton: CRC Press; 1991:103–114.
Bennick A: Interaction of plant polyphenols with salivary proteins. Crit Rev Oral Biol Med 2002, 13: 184–196. 10.1177/154411130201300208
Rayment SA, Liu B, Offner GD, Oppenheim FG, Troxler RF: Immunoquantification of human salivary mucins MG1 and MG2 in stimulated whole saliva: factors influencing mucin levels. J Dent Res 2000, 79: 1765–1772. 10.1177/00220345000790100601
Veerman EC, van den Keijbus PA, Nazmi K, Vos W, van der Wal JE, Bloemena E, Bolscher JG, Amerongen AV: Distinct localization of MUC5B glycoforms in the human salivary glands. Glycobiology 2003, 13: 363–366. 10.1093/glycob/cwg037
Asquith TN, Uhlig J, Meansho H, Putman L, Carlson DM, Butler L: Binding of condensed tannins to salivary proline-rich glycoproteins: the role of carbohydrate. J Agric Food Chem 1987, 35: 331–334. 10.1021/jf00075a012
Goto M, Fujimoto W, Nio J, Iwanaga T, Kawasaki T: Immunohistochemical demonstration of acidic mammalian chitinase in the mouse salivary gland and gastric mucosa. Arch Oral Biol 2003, 48: 701–707. 10.1016/S0003-9969(03)00150-X
van Steijn GJ, Amerongen AV, Veerman EC, Kasanmoentalib S, Overdijk B: Chitinase in whole and glandular human salivas and in whole saliva of patients with periodontal inflammation. Eur J Oral Sci 1999, 107: 328–337. 10.1046/j.0909-8836.1999.eos107503.x
van Steijn GJ, Amerongen AV, Veerman EC, Kasanmoentalib S, Overdijk B: Effect of periodontal treatment on the activity of chitinase in whole saliva of periodontitis patients. J Periodontal Res 2002, 37: 245–249. 10.1034/j.1600-0765.2002.00330.x
Leymarie N, Berg EA, McComb ME, O'Connor PB, Grogan J, Oppenheim FG, Costello CE: Tandem mass spectrometry for structural characterization of proline-rich proteins: application to salivary PRP-3. Anal Chem 2002, 74: 4124–4132. 10.1021/ac0255835
Richard T, Lefeuvre D, Descendit A, Quideau S, Monti JP: Recognition characters in peptide-polyphenol complex formation. Biochim Biophys Acta 2006, 1760: 951–958.
Kandra L, Gyémánt G, Zajacz A, Batta G: Inhibitory effects of tannin on human salivary alpha amylase. Biochem Biophys Res Comm 2004, 319: 1265–1271. 10.1016/j.bbrc.2004.05.122
This work was supported by POCTI FCT/CVT/33039 scientific project; Elsa Lamy, Gonçalo da Costa and Catarina Franco were supported by FCT (Fundação para a Ciência e a Tecnologia of Ministério da Ciência, Tecnologia e Ensino Superior) PhD grants (SFRH/BD/6776/2001, SFRH/BD/14387/2003 and SFRH/BD/29799/2006, respectively). We acknowledge the generous offer of Tupafin Ato from the Silva Chimica Company (Italy).
The authors declare that they have no competing interests.
All authors contributed and approved the final manuscript. ESB and AVC were responsible for the conception and design of the study. GG and GC performed the protein separation and protein identification by PMF. CF performed the MALDI TOF-TOF protein identification. Histologic studies were performed by EL and FCS. EL and GG analyzed and interpreted the data. EL drafted the manuscript and ESB and AVC revised it critically for important content. All authors confirm that the content has not been published elsewhere and does not duplicate their published work.
Electronic supplementary material
Additional file 1: . Spots Q1 and Q2, which were only observed in 2-DE gels from quebracho group, appear dark pink following Beeley et al.24 CBB R-250 stainning protocol for PRPs. (JPEG 45 KB)
About this article
Cite this article
Lamy, E., Graça, G., da Costa, G. et al. Changes in mouse whole saliva soluble proteome induced by tannin-enriched diet. Proteome Sci 8, 65 (2010). https://doi.org/10.1186/1477-5956-8-65
- Protein Spot
- Salivary Protein
- Salivary Amylase
- Dietary Tannin