More stories

  • in

    Impact of climate, rising atmospheric carbon dioxide, and other environmental factors on water-use efficiency at multiple land cover types

    Effects of multiple environmental factors on WUE
    An increasing EWUE trend was observed at the forest site with a change in climate (E1) which might be due to the increasing trend in precipitation (2.982 mm year−1) that enhanced carbon assimilation over the 30 years (Table 4). However, as precipitation decreased at the grassland and cropland sites (− 4.807 and − 2.338 mm year−1), it reduced carbon assimilation as well (Table 4), which in turn negatively affected EWUE. This relationship between precipitation and carbon assimilation is supported by the results of a previous study by Sun et al.30 and Zhao et al.32. The EWUE trend (E1) at the forest site in the first period (1981–2000, A1 in Fig. 1a) was lower than in the second period (2001–2010, A2 in Fig. 1a), indicating an increase in GPP due to rising temperature. The cropland and grassland sites (Fig. 1b, c) showed an increasingly negative trend in EWUE (in contrast to the forest site), as they were affected by climatic variables such as precipitation, temperature, and solar radiation (Table 4).
    Due to rising CO2 (E2–E1), EWUE increased at all three sites in both study periods due to its structural effect (where plant growth increased due to higher CO2 concentration and changed the plant structure with increasing LAI)3,31 (Fig. 1). The EWUE trends decreased due to the effect of aerosol concentration (E3-E1) at grassland and cropland sites. ET and carbon assimilation decreased due to the higher concentration of aerosols, which reduced the solar radiation reaching the earth’s surface23,31 (Table S4). The effect of nitrogen deposition at the forest site decreased in the second period (2001–2010, A2 in Fig. 1a, Table S4) but continued to exhibit a negative trend.
    Experiment E5 (ALL), which considered all climate and environmental factors, showed an increase in EWUE at the forest site, which was highly affected by CO2 fertilization and increased precipitation over the 3 decades (Fig. 1a, Table 4). However, at the grassland and cropland sites, EWUE decreased due to the negative precipitation trend and the positive trends in temperature and shortwave radiation over the 30-year period (Fig. 1b,c; Table 4). EWUE increased between the two study periods at the forest site but decreased at the grassland and cropland sites, likely due to the increase in CO2 and the effects of climatic variables.
    In Fig. 2, the trends for TWUE (Case E1, ‘CLIM’) were steeper than those of EWUE, due to lower Tr than ET and higher GPP in the forest ecosystem (Figs. 2a, S3). However, the negative trend of TWUE was lessened due to the minimal Tr effect in ET at the grassland site, corroborated by ET and Tr trends (Figs. 2b, S4). The cropland site also showed a slight reduction in the negative trend of TWUE compared with EWUE due to higher positive trend in Tr compared with ET (Figs. 1c, 2c, S5). The CO2 fertilization effect (E2–E1) played an important role in the increase in carbon assimilation at the forest site and ultimately increased the TWUE trend compared with those at the grassland and cropland sites with statistical significance (p  More

  • in

    Strontium and oxygen isotopes as indicators of Longobards mobility in Italy: an investigation at Povegliano Veronese

    For this study soil, tooth, and bone specimens of humans and animals were sampled for strontium isotope ratios (87Sr/86Sr), whereas teeth and bones of humans and animals were sampled for stable oxygen isotopes analysis δ(18O/16O). Sample collection, preparation and analysis was performed in accordance with relevant regulations for the treatment of ancient human remains. Permission to analyze the samples was granted by the local SABAP (Soprintendenza Archeologia, Belle Arti e Paesaggio per le province di Verona, Rovigo e Vicenza).
    Because of the bad state of preservation of some of the human teeth, sampling for isotopic study could not be consistent. We decided to use the tooth that was mostly represented. Hence, we preferentially sampled canines, with second and third molars as possible substitutes. The enamel of the canines forms from 4 months to six-seven years of life; whereas the second molar forms from three to seven-eight years and the third molar from seven-eight to more than twelve years representing late childhood-adolescence. For dental enamel sampling, we collected for both analyses approximately 50 mg of enamel powder, with a microdrill mounting a diamond burr, from the lingual surface of the tooth. The extracted enamel came from the lower half of the crown in order to prevent alterations due to metabolism in early formation phases23 and to reduce the noise in the data linked to random sampling.
    For the analysis of bone, we took approximately 50 mg of cortical bone tissue, mostly from ribs24. Several authors recommend to avoid analyzing bone for Sr isotope ratios because it is particularly prone to diagenetic processes12,25,26,27,28. However, in order to test possible diagenesis, and to observe the difference between tooth value and bone value in the same individual, we run two bone analyses for strontium and sixteen analyses for oxygen.
    In order to define the local range at Povegliano Veronese and to compare the data obtained from teeth and bones of humans and animals, we took soil samples from the burials of area H, namely: T 348, T 426, T 413, T 45 (Table 2).
    In total, 39 individuals were selected from 35 burials at Povegliano Veronese, while a grand total of 8 animal samples came from a midden excavated near the main concentration of burials and dated to the phase of use of the cemetery (G. De Zuccato pers. comm.). We selected all animal species determined within the midden (using a MNI criterion, Table 2 SI); both domesticated and wild species were available for analyses, namely: one individual of Equus caballus, two individuals of Bos taurus, two of Sus domesticus, two of Ovis vel Capra end one of Cervus elaphus (Table 1).
    The burials were selected according to position within the cemetery, dating of grave goods and typology of tomb structure17, we tried to keep a balance in the composition of the sample in accordance to sex and age at death of the individuals. In order to examine strontium and oxygen ratios in humans over time we chose 21 burials dated to phase 1, 9 burials of subsequent phases (2 and 3), and 4 burials with undetermined chronology. We further sampled individuals from 3 multiple burials, which despite not providing a date were considered worthy of investigation.
    In particular, the strontium isotopic ratio was measured in 39 enamel samples and 2 human bones, 4 soils samples (from area H), 4 animal teeth (from one Equus caballus, one Bos taurus, one Sus domesticus and one of Ovis vel Capra respectively) and 2 animal bones (from one Equus caballus and one Sus domesticus). Oxygen isotopic ratios were measured in 13 human teeth, 16 human bones, and 5 animal teeth (one specimen of Equus caballus, two specimens of Bos Taurus, two of Sus domesticus, one specimen of Ovis vel Capra) and 7 animal bones (one specimen of Equus caballus, two specimens of Bos taurus, two of Sus domesticus, two of Ovis vel Capra end one of Cervus elaphus) (Table 1).
    Strontium isotope ratio (87Sr/86Sr)
    After cleaning the surface of each tooth by abrasion with a diamond burr, 20–30 mg of enamel powered were extracted and digested in 1 ml concentrated ultrapure HCl. The samples were then evaporated to dryness and redissolved in 2 ml 2 M ultrapure HCl.
    For bone analysis, the samples were mechanically cleaned and authigenic carbonates removed with CH3COONH4 buffer at pH 5 in an ultrasonic bath. Approximately 5 g of cortical bone were reduced to ashes in a furnace at 800 °C for 10 h and then the material was homogenized in an agate mortar and dissolved with 6 N ultrapure HCl. Once the bone dissolution completed, the samples were evaporated to dryness, redissolved in 2 ml 2 N ultrapure HCl.
    Soil samples were leaching with 1 N CH3COONH4 at neutral pH to obtain the NH4-acetate extract that represents organically bound Sr29. The extracts were processed for Sr isotopic analysis following the procedure of bone analysis.
    Sr was separated from the matrix onto a preconditioned resin column with 2 mL of AG50W-X12 (200 − 400 mesh) following the procedure of Chao et al.30.
    Isotopic analyses were carried out at IGAG-CNR c/o Dipartimento di Scienze della Terra, as Sapienza, University of Rome using a FINNIGAN MAT 262RPQ multicollector mass spectrometer with W single filaments in static mode. Sr isotopic fractionations was corrected against 86Sr/88Sr = 0.1194. During the data acquisition, measured isotopic ratios of NBS 987 Sr standard, resulted as 87Sr/86Sr = 0.710285 ± 10 (2σ; n = 27). The within-run precision, expressed as 2se (standard errors), was better than 0.000012 for Sr. Total procedural blanks were below 2 ng.
    Stable oxygen isotopes analysis
    Stable oxygen isotopes δ(18O/16O)ph analyses on the phosphate group of teeth and bones of human and animal bioapatite (ph) were carried out at the Stable Isotope Laboratory of the University of Parma.
    To analyze the oxygen isotopic composition of the apatite phosphate group of bone and tooth of humans and animals we followed the protocol by Stephan31.
    The sample treatments were the following: samples reacted with 2.5% NaOCl for 24 h to oxidize organic substances; then, the samples were reacted with 0.125 M of NaOH for 48 h to dissolve humic substances, 2 M HF for 24 h, 2 M KOH and buffered amine solution. The solutions were then warmed at 70 °C for 3 h and filtered to collect the precipitated crystals of Ag3PO4. The crystals were analyzed by means of TC/EA, thermal conversion-elemental unit on line with a mass spectrometer (IRMS).
    According to IUPAC (International Union of Pure and Applied Chemistry), the isotope ratio 18O/16O is expressed as:

    $$ {{delta}}left( {^{18}} {text{O}}/^{16} {text{O}} right) = frac{(^{18} {text{O}}/^{16} {text{O}})_{{{text{sample}}}}}{(^{18} {text{O}}/^{16} {text{O}})_{{{text{V}} – {text{SMOW}}}} } – 1 = frac{left[ {1000 left( {frac{{(^{18} {text{O}}/^{16} {text{O}})_{{{text{sample}}}} }}{{(^{18} {text{O}}/^{16} {text{O}})_{{{text{V}} – {text{SMOW}}}} }}{ }{-}{ }1{ }} right)} right]}{1000} = frac{text{X}}{1000} = {text{X}};permil $$

    where δ18Osample and δ18OV-SMOV are the isotopic abundances in the sample in analysis and in the reference international standard V-SMOW (Vienna Standard Mean Oceanic Water), and ‰ = 1/1,000. The estimated analytical prediction uncertainty for 18δ is ≤ 0.35‰. Hereafter, for simplicity, we report δ18O in place of δ(18O/16O).
    In order to relate the values δ18Oph of the ({mathrm{P}mathrm{O}}_{4}^{3-}) anionic group of enamel and bone bioapatite to that, δ18Ow, of the drinking water, we used the following equations:
    for humans:
    δ18Ow = 1.847 δ18Oph − 0.0384 Iacumin and Venturelli 21
    for Capra:
    δ18Ow = 1.14 δ18Oph − 0.0274 Delgado Huertas et al.32
    for Ovis:
    δ18Ow = 0.676 δ18Oph − 0.0184 Delgado Huertas et al.33
    for Bos:
    δ18Ow = 0.990 δ18Oph − 0.0247 Delgado Huertas et al.33
    for Equus:
    δ18Ow = 1.41 δ18Oph − 0.0318 Delgado Huertas et al.33
    for Cervus:
    δ18Ow = 0.885 δ18Oph − 0.0227 D’Angela and Longinelli34
    δ18Ow = 1.16 δ18Oph − 0.0264 Longinelli13
    (It is noteworthy that the equations used for animals could not to be statistically different one from the other). More

  • in

    Effects of weaning age and housing conditions on phenotypic differences in mice

    1.
    Baker, M. 1,500 scientists lift the lid on reproducibility. Nature 533, 452–454 (2016).
    ADS  CAS  PubMed  Google Scholar 
    2.
    Begley, C. G. & Ellis, L. M. Drug development: Raise standards for preclinical cancer research. Nature 483, 531–533 (2012).
    ADS  CAS  Google Scholar 

    3.
    Prinz, F., Schlange, T. & Asadullah, K. Believe it or not: How much can we rely on published data on potential drug targets?. Nat. Rev. Drug Discov. 10, 712 (2011).
    CAS  PubMed  Google Scholar 

    4.
    Bailoo, J. D., Reichlin, T. S. & Würbel, H. Refinement of experimental design and conduct in laboratory animal research. ILAR J. 55, 383–391 (2014).
    CAS  PubMed  Google Scholar 

    5.
    Richter, S. H., Garner, J. P. & Würbel, H. Environmental standardization: Cure or cause of poor reproducibility in animal experiments?. Nat. Methods 6, 257–261 (2009).
    CAS  PubMed  Google Scholar 

    6.
    Voelkl, B., Vogt, L., Sena, E. S. & Würbel, H. Reproducibility of preclinical animal research improves with heterogeneity of study samples. PLoS Biol. 16, e2003693 (2018).
    PubMed  PubMed Central  Google Scholar 

    7.
    Amrhein, V., Trafimow, D. & Greenland, S. Inferential statistics as descriptive statistics: There is no replication crisis if we don’t expect replication. Am. Stat. 73(sup1), 262–270 (2019).
    MathSciNet  Google Scholar 

    8.
    Bohlen, M. et al. Experimenter effects on behavioral test scores of eight inbred mouse strains under the influence of ethanol. Behav. Brain Res. 272, 46–54 (2014).
    ADS  CAS  PubMed  PubMed Central  Google Scholar 

    9.
    Corrigan, J. K. et al. A big-data approach to understanding metabolic rate and response to obesity in laboratory mice. bioRxiv https://doi.org/10.1101/839076 (2019).
    Article  Google Scholar 

    10.
    Crabbe, J. C., Wahlsten, D. L. & Dudek, B. C. Genetics of mouse behavior: Interactions with laboratory environment. Science (80-). 284, 1670–1672 (1999).
    ADS  CAS  Google Scholar 

    11.
    Wahlsten, D. et al. Different data from different labs: Lessons from studies of gene-environment interaction. J. Neurobiol. 54, 283–311 (2003).
    PubMed  Google Scholar 

    12.
    Richter, S. H. et al. Effect of population heterogenization on the reproducibility of mouse behavior: A multi-laboratory study. PLoS ONE 6, e16461 (2011).
    ADS  CAS  PubMed  PubMed Central  Google Scholar 

    13.
    Voelkl, B. & Würbel, H. Reproducibility crisis: Are we ignoring reaction norms?. Trends Pharmacol. Sci. 37(7), 509–510 (2016).
    CAS  PubMed  Google Scholar 

    14.
    Terranova, M. L. & Laviola, G. Delta opioid modulation of social interactions in juvenile mice weaned at different ages. Physiol. Behav. 73, 393–400 (2001).
    CAS  PubMed  Google Scholar 

    15.
    Ladd, C. O., Owens, M. J. & Nemeroff, C. B. Persistent changes in corticotropin-releasing factor neuronal systems induced by maternal deprivation. Endocrinology 137, 1212–1218 (1996).
    CAS  PubMed  Google Scholar 

    16.
    Berry, A. et al. Social deprivation stress is a triggering factor for the emergence of anxiety- and depression-like behaviours and leads to reduced brain BDNF levels in C57BL/6J mice. Psychoneuroendocrinology 37, 762–772 (2012).
    CAS  PubMed  Google Scholar 

    17.
    Kanari, K., Kikusui, T., Takeuchi, Y. & Mori, Y. Multidimensional structure of anxiety-related behavior in early-weaned rats. Behav. Brain Res. 156, 45–52 (2005).
    PubMed  Google Scholar 

    18.
    Kikusui, T., Nakamura, K., Kakuma, Y. & Mori, Y. Early weaning augments neuroendocrine stress responses in mice. Behav. Brain Res. 175, 96–103 (2006).
    CAS  PubMed  Google Scholar 

    19.
    Francis, D. D., Champagne, F. A., Liu, D. & Meaney, M. J. Maternal care, gene expression, and the development of individual differences in stress reactivity. Ann. N. Y. Acad. Sci. 896, 66–84 (1999).
    ADS  CAS  PubMed  Google Scholar 

    20.
    Bailoo, J. D., Jordan, R. L., Garza, X. J. & Tyler, A. N. Brief and long periods of maternal separation affect maternal behavior and offspring behavioral development in C57BL/6 mice. Dev. Psychobiol. 56, 674–685 (2013).
    PubMed  Google Scholar 

    21.
    Bailoo, J. D., Varholick, J. A., Garza, X. J., Jordan, R. L. & Hintze, S. Maternal separation followed by isolation-housing differentially affects prepulse inhibition of the acoustic startle response in C57BL/6 mice. Dev. Psychobiol. 58, 937–944 (2016).
    PubMed  Google Scholar 

    22.
    Macrí, S., Mason, G. J. & Würbel, H. Dissociation in the effects of neonatal maternal separations on maternal care and the offspring’s HPA and fear responses in rats. Eur. J. Neurosci. 20, 1017–1024 (2004).
    PubMed  Google Scholar 

    23.
    Krackow, S. & Hoeck, H. N. Sex ratio manipulation, maternal investment and behaviour during concurrent pregnancy and lactation in house mice. Anim. Behav. 37, 177–186 (1989).
    Google Scholar 

    24.
    König, B. & Markl, H. Maternal care in house mice. Behav. Ecol. Sociobiol. 20, 1–9 (1987).
    Google Scholar 

    25.
    König, B. Components of lifetime reproductive success in communally and solitarily nursing house mice: A laboratory study. Behav. Ecol. Sociobiol. 34, 275–283 (1994).
    Google Scholar 

    26.
    Hall, F. S. Social deprivation of neonatal, adolescent, and adult rats has distinct neurochemical and behavioral consequences. Crit. Rev. Neurobiol. 12, 129–162 (1998).
    CAS  PubMed  Google Scholar 

    27.
    Richter, S. H. et al. A time to wean? Impact of weaning age on anxiety-like behaviour and stability of behavioural traits in full adulthood. PLoS ONE 11, e0167652 (2016).
    PubMed  PubMed Central  Google Scholar 

    28.
    Curley, J. P. et al. The meaning of weaning: Influence of the weaning period on behavioral development in mice. Dev. Neurosci. 31, 318–331 (2009).
    CAS  PubMed  PubMed Central  Google Scholar 

    29.
    Bechard, A. & Mason, G. Leaving home: A study of laboratory mouse pup independence. Appl. Anim. Behav. Sci. 125, 181–188 (2010).
    Google Scholar 

    30.
    Kikusui, T. & Mori, Y. Behavioural and neurochemical consequences of early weaning in rodents. J. Neuroendocrinol. 21, 427–431 (2009).
    CAS  PubMed  Google Scholar 

    31.
    Kikusui, T., Kiyokawa, Y. & Mori, Y. Deprivation of mother-pup interaction by early weaning alters myelin formation in male, but not female, ICR mice. Brain Res. 1133, 115–122 (2007).
    CAS  PubMed  Google Scholar 

    32.
    Nakamura, K., Kikusui, T., Takeuchi, Y. & Mori, Y. Changes in social instigation- and food restriction-induced aggressive behaviors and hippocampal 5HT1B mRNA receptor expression in male mice from early weaning. Behav. Brain Res. 187, 442–448 (2008).
    CAS  PubMed  Google Scholar 

    33.
    Nakamura, K., Kikusui, T., Takeuchi, Y. & Mori, Y. The influence of early weaning on aggressive behavior in mice. J. Vet. Med. Sci. 65, 1347–1349 (2003).
    PubMed  Google Scholar 

    34.
    Würbel, H. & Stauffacher, M. Age and weight at weaning affect corticosterone level and development of stereotypies in ICR-mice. Anim. Behav. 53, 891–900 (1997).
    Google Scholar 

    35.
    Latham, N. R. & Mason, G. J. Maternal deprivation and the development of stereotypic behaviour. Appl. Anim. Behav. Sci. 110, 84–108 (2008).
    Google Scholar 

    36.
    Kikusui, T., Ichikawa, S. & Mori, Y. Maternal deprivation by early weaning increases corticosterone and decreases hippocampal BDNF and neurogenesis in mice. Psychoneuroendocrinology 34, 762–772 (2009).
    CAS  PubMed  Google Scholar 

    37.
    Franklin, T. B. et al. Epigenetic transmission of the impact of early stress across generations. Biol. Psychiatry 68, 408–415 (2010).
    PubMed  Google Scholar 

    38.
    Olsson, I. A. S. & Westlund, K. More than numbers matter: The effect of social factors on behaviour and welfare of laboratory rodents and non-human primates. Appl. Anim. Behav. Sci. 103, 229–254 (2007).
    Google Scholar 

    39.
    Cacioppo, S., Capitanio, J. P. & Cacioppo, J. T. Toward a neurology of loneliness. Psychol. Bull. 140, 1464–1504 (2014).
    PubMed  PubMed Central  Google Scholar 

    40.
    Krohn, T. C., Sorensen, D. B., Ottesen, J. L. & Hansen, A. K. The effects of individual housing on mice and rats: A review. Anim. Welf. 15, 343–352 (2006).
    CAS  Google Scholar 

    41.
    Brain, P. What does individual housing mean to a mouse?. Life Sci. 16, 187–200 (1975).
    CAS  PubMed  Google Scholar 

    42.
    Valzelli, L. The ‘isolation syndrome’ in mice. Psychopharmacologia 31, 305–320 (1973).
    CAS  PubMed  Google Scholar 

    43.
    Albin, R. L., Young, A. B. & Penney, J. B. The functional anatomy of basal ganglia disorders. Trends Neurosci. 12, 366–375 (1989).
    CAS  PubMed  Google Scholar 

    44.
    Deroche, V., Piazza, P. V., Moal, M. L. & Simon, H. Social isolation-induced enhancement of the psychomotor effects of morphine depends on corticosterone secretion. Brain Res. 640, 136–139 (1994).
    CAS  PubMed  Google Scholar 

    45.
    Piazza, P. V. et al. Suppression of glucocorticoid secretion and antipsychotic drugs have similar effects on the mesolimbic dopaminergic transmission. Proc. Natl. Acad. Sci. 93, 15445–15450 (2002).
    Google Scholar 

    46.
    Van Loo, P. L. P. P., Van Zutphen, L. F. M. M. & Baumans, V. Male management: Coping with aggression problems in male laboratory mice. Lab. Anim. 37, 300–313 (2003).
    PubMed  Google Scholar 

    47.
    Gerlach, G. Dispersal mechanisms in a captive wild house mouse population (Mus domesticus Rutty). Biol. J. Linn. Soc. 41, 271–277 (1990).
    Google Scholar 

    48.
    Gerlach, G. Emigration mechanisms in fetal house mice: A laboratory investigation of the influence of social structure, population density, and aggression. Behav. Ecol. Sociobiol. 39, 159–170 (1996).
    Google Scholar 

    49.
    Berry, R. J. & Bronson, F. H. Life history and bioeconomy of the house mouse. Biol. Rev. Camb. Philos. Soc. 67, 519–550 (1992).
    CAS  PubMed  Google Scholar 

    50.
    Jansen, R. G., Wiertz, L., Meyer, E. S. & Noldus, L. P. J. J. Reliability analysis of observational data: Problems, solutions, and software implementation. Behav. Res. Methods Instrum. Comput. 35, 391–399 (2003).
    PubMed  Google Scholar 

    51.
    Pellow, S., Chopin, P., File, S. & Briley, M. Validation of open: Closed arm entries in an elevated plus-maze as a measure of anxiety in the rat. J. Neurosci. Methods 14, 149–167 (1985).
    CAS  PubMed  Google Scholar 

    52.
    File, S. E. & Seth, P. A review of 25 years of the social interaction test. Eur. J. Pharmacol. 463, 35–53 (2003).
    CAS  PubMed  Google Scholar 

    53.
    Bailoo, J. D., Bohlen, M. O. & Wahlsten, D. L. The precision of video and photocell tracking systems and the elimination of tracking errors with infrared backlighting. J. Neurosci. Methods 188, 45–52 (2010).
    PubMed  PubMed Central  Google Scholar 

    54.
    Möstl, E. & Palme, R. Hormones as indicators of stress. Domest. Anim. Endocrinol. 23, 67–74 (2002).
    PubMed  Google Scholar 

    55.
    Touma, C. & Palme, R. Measuring Fecal glucocorticoid metabolites in mammals and birds: The importance of validation. Ann. N. Y. Acad. Sci. 1046, 54–74 (2005).
    ADS  CAS  PubMed  Google Scholar 

    56.
    Palme, R. Non-invasive measurement of glucocorticoids: Advances and problems. Physiol. Behav. 199, 229–243 (2019).
    CAS  PubMed  Google Scholar 

    57.
    Touma, C., Sachser, N., Möstl, E. & Palme, R. Effects of sex and time of day on metabolism and excretion of corticosterone in urine and feces of mice. Gen. Comp. Endocrinol. 130, 267–278 (2003).
    CAS  PubMed  Google Scholar 

    58.
    Touma, C., Palme, R. & Sachser, N. Analyzing corticosterone metabolites in fecal samples of mice: A noninvasive technique to monitor stress hormones. Horm. Behav. 45, 10–22 (2004).
    CAS  PubMed  Google Scholar 

    59.
    Kikusui, T., Takeuchi, Y. & Mori, Y. Early weaning induces anxiety and aggression in adult mice. Physiol. Behav. 81, 37–42 (2004).
    CAS  PubMed  Google Scholar 

    60.
    Iwata, E., Kikusui, T., Takeuchi, Y. & Mori, Y. Fostering and environmental enrichment ameliorate anxious behavior induced by early weaning in Balb/c mice. Physiol. Behav. 91, 318–324 (2007).
    CAS  PubMed  Google Scholar 

    61.
    Benton, D. & Brain, P. F. Behavioral and adrenocortical reactivity in female mice following individual or group housing. Dev. Psychobiol. 14, 101–107 (1981).
    CAS  PubMed  Google Scholar 

    62.
    Goldsmith, J. F., Brain, P. F. & Benton, D. Effects of the duration of individual or group housing on behavioural and adrenocortical reactivity in male mice. Physiol. Behav. 21, 757–760 (1978).
    CAS  PubMed  Google Scholar 

    63.
    Faggin, B. M. & Palermo-Neto, J. Differential alterations in brain sensitivity to amphetamine and pentylenetetrazol in socially deprived mice. Gen. Pharmacol. 16, 299–302 (1985).
    CAS  PubMed  Google Scholar 

    64.
    Cairns, R. B., Hood, K. E. & Midlam, J. On fighting in mice: Is there a sensitive period for isolation effects?. Anim. Behav. 33, 166–180 (1985).
    Google Scholar 

    65.
    de Catanzaro, D. & Gorzalka, B. B. Sexual arousal in male mice: Effects of brief periods of isolation or grouping. Behav. Neural Biol. 28, 442–453 (1980).
    PubMed  Google Scholar 

    66.
    Einon, D. F., Humphreys, A. P., Chivers, S. M., Field, S. & Naylor, V. Isolation has permanent effects upon the behavior of the rat, but not the mouse, gerbil, or guinea pig. Dev. Psychobiol. 14, 343–355 (1981).
    CAS  PubMed  Google Scholar 

    67.
    Misslin, R., Herzog, F., Koch, B. & Ropartz, P. Effects of isolation, handling and novelty on the pituitary-adrenal response in the mouse. Psychoneuroendocrinology 7, 217–221 (1982).
    CAS  PubMed  Google Scholar 

    68.
    Rodgers, R. J. & Cole, J. C. Influence of social isolation, gender, strain, and prior novelty on plus-maze behaviour in mice. Physiol. Behav. 54, 729–736 (1993).
    CAS  PubMed  Google Scholar 

    69.
    Kikusui, T., Nakamura, K. & Mori, Y. A review of the behavioral and neurochemical consequences of early weaning in rodents. Appl. Anim. Behav. Sci. 110, 73–83 (2008).
    Google Scholar 

    70.
    Kikusui, T. et al. Early weaning increases anxiety via brain-derived neurotrophic factor signaling in the mouse prefrontal cortex. Sci. Rep. 9, 3991 (2019).
    ADS  PubMed  PubMed Central  Google Scholar 

    71.
    Weinstock, M. The long-term behavioural consequences of prenatal stress. Neurosci. Biobehav. Rev. 32, 1073–1086 (2008).
    CAS  PubMed  Google Scholar 

    72.
    Archer, J. E. & Blackman, D. E. Prenatal psychological stress and offspring behavior in rats and mice. Dev. Psychobiol. 4, 193–248 (1971).
    CAS  PubMed  Google Scholar  More

  • in

    Chemical weathering and CO2 consumption rates of rocks in the Bishuiyan subterranean basin of Guangxi, China

    Physicochemical parameters and total concentrations of dissolved ions
    The pH of all of the water samples ranged from 6.68 to 8.33 (Table 1), indicating that the waters were circumneutral to alkaline. Conductivity values ranged from 21.1 to 331 μs/cm. The conductivity values of the R1 and R2 samples were relatively low (21.1–65.4 μs/cm), and reflected waters came from the granite host rock area. These values were also consistent with conductivity values measured upstream in the Zengjiang (42.7–66.9 μs/cm) and Pearl (27.2–78.6 μs/cm) Rivers29. The conductivity values of water samples in the carbonate area (G1, G2) and waters flowing through the carbonate zone (R3) were relatively higher (93.9–331 μs/cm). The result illustrated that the weathering rate of carbonate was higher than the weathering rate of silicate lead to the significant different of physicochemical parameters in samples30.
    Table 1 Hydro-chemical measurements of water samples from the Bishuiyan subterranean basin.
    Full size table

    In natural waters, the total number of cations (Ca2+, Mg2+, Na+, and K+) produced during mineral weathering is nearly equivalent to that of anions produced in aggressive medium31,32. The total cation concentrations of waters analyzed here ranged from 347 to 4,072 μEq/L, in which the result was similar to 60 rivers in the world (TZ+ = 300–10,000 μEq/L)21. The average value of TZ+ is 1855 μEq/L, which is higher than the global average value for rivers (1,250 μEq/L)33 and Qiantangjiang River (1357 μEq/L)34. The total anion concentrations of water samples ranged from 352–3,732 μEq/L, with an average value of 1803 μEq/L, which was significant higher than the Qiantangjiang River (1,363 μEq/L)34. Equilibrium coefficients (NIBC = (TZ+ − TZ−)/TZ+) ranged from − 9.97 to  + 9.80% with an average value of 1.26%. The typical range of NIBC values is − 10 to  + 10%.
    The spatial distribution of primary ionic components
    Comparison of water chemical compositions from each cross section of the Bishuiyan subterranean basin indicated that upstream waters were significantly different from those downstream. Cation concentrations of R1, R2, and Q1 upstream waters exhibited trends of Ca2+ (0.11–0.31 mmol/L)  > Na+ + K+ (0.07–0.15 mmol/L)  > Mg2+ (0.01–0.08 mmol/L). The cationic composition was similar to that of Qiantangjiang River basin and Songhua River basin which were mainly composed of exposed silicate9,34. In contrast, the cation concentrations of G1, G2, R3, and Q2 waters followed trends of Ca2+ (0.31–1.45 mmol/L)  > Mg2+ (0.10–0.64 mmol/L)  > Na+ + K+ (0.07–0.19 mmol/L). This was similar to that of Wujiang River basin which was mainly composed of carbonate35. HCO3− was the primary anion for all of the river waters, and accounted for 66.7%–95.0% of total anions. HCO3− ranged from 0.30–0.63 mmol/L in R1, R2, and Q1 and 0.30–3.07 mmol/L for G1, G2, R3, and Q2. The other anions (in descending concentration) were NO3−, SO42−, and Cl−. Ionic concentrations in upstream waters were significantly lower than that in the carbonate area, indicating that corrosion of carbonate considerably influenced the chemical properties of river waters.
    Qualitative analysis of ion sources
    Chemical analysis of river waters
    Water chemical properties can reflect different sources or varying chemical conditions, as exhibited by particular elemental ratios36. Nearly all of the water samples fell above the equilibrium line of Na:Cl = 1 (Fig. 2a). These solute concentrations are influenced by marine aerosols, in addition to other factors37. In particular, the ratio of Ca2+ + Mg2+ and HCO3- is typically used to identify carbonate weathering. The concentration of Ca2+ + Mg2+ was higher than that of HCO3− in most of the samples (Fig. 2c). These results implicate the influence of acid from other sources in the weathering of carbonate38.
    Figure 2

    Relationships among major ions within waters of the Bishuiyan river basin.

    Full size image

    In addition to the erosive effect of H2CO3 derived from the atmospheric CO2, H2SO4 and HNO3 also make contributions to the rock weathering process (Fig. 2d). Previous studies showed that the chemical weathering by sulfuric acid played an important role in the chemical weathering of karst basin39,40,41. The sulfuric acid mainly come from atmospheric deposition, evaporate formation (gypsum/anhydrite and MgSO4) and oxidation of sulfides (pyrite)37. SO42− was positively correlated with NO3− and Cl− in Bishuiyan River waters, while SO42− was not obviously correlated with HCO3−. Further, SO42− and NO3− were positively correlated with Na+ (Fig. 2b), indicating a similar source of SO42− and NO3− as Cl−. Since there is no evaporates in the research area, the source of SO42− was not evaporates. It is likely that the allogenic acids in the river primarily derive from human activities and the oxidation of sulfides.
    Assuming that the allogenic acids (H2SO4 and HNO3) derived from human activities or sulfide oxidation were only used to balance Ca2+ and Mg2+ concentrations in the water, then [Ca2+ + Mg2+]*([Ca2+ + Mg2+]* = [Ca2+ + Mg2+] − [SO42− + NO3−]) originates from the weathering of carbonate and silicate. Therefore, the ratio of [Ca2+ + Mg2+]* to [HCO3−] represents the relative concentration of Ca2+ and Mg2+ from the weathering of carbonate and silicate, which should exhibit a ratio of less than 1.0. Similarly, the [Na+ + K+]*([Na+ + K+]* = [Na+ + K+] − [Cl−]) in the river results from the weathering of carbonate and silicate. Consequently, variation in the ratios of [Ca2+ + Mg2+]*/[HCO3−] and [Na+ + K+]*/[HCO3−] reflect the relative contribution of carbonate weathering and silicate weathering to solutes in the river water. The ratios for R1, R2, and Q1 waters fall on both sides of the 1:1 line, indicating that the water chemistry of the tributary water was influenced primarily by the weathering of silicate (Fig. 3). In contrast, water from the Chuanyan tributary and the exposed underground river in the carbonate area exhibited ratios of [Ca2+ + Mg2+]*/[HCO3−] = 1 and [Na+ + K+]*/[HCO3−] = 0, indicating that the water chemistry of the underground river was mainly controlled by the weathering of carbonate42. The [Ca2+ + Mg2+]* and [Na+ + K+]* values were higher than those for HCO3- in the first quadrant of the graph, suggesting that excessive cations were not derived from the weathering of silicate and carbonate, but rather may be contributed by human activities. Consequently, it is likely that the anthropogenic contribution to cation concentrations was very small.
    Figure 3

    Relative contribution to water solute chemistry from silicate and carbonate weathering by carbonic acid.

    Full size image

    Identification of rock weathering source material
    Triangular component compositional figures can aid analysis of water chemical data by aiding identification of water chemical compositions, the estimation of relative contributions of primary ions, and also help distinguish sources of solutes and their potential controls. Importantly, the relative contribution of chemical weathering of various rock minerals to dissolved solute loads of waters can be estimated through such analyses43. Triangular ionic compositional analysis of small rivers in the Bishuiyan subterranean basin (Fig. 4) indicated that cations were near the Ca2+ endmember at the exit of the Bishuiyan subterranean basin (G1, G2), while anions were reflective of an endmember water from carbonate weathering by H2CO3. The main cation in Taiping region water (R1, R2, and Q1) was Ca2+, and was also shifted towards the [Na+ + K+] endmember, while anions fell between the H2CO3-weathered carbonate and H2CO3-weathered silicate endmembers. The main cation of the Chuanyan region water (R3, Q2) was Ca2+, with a more minor contribution of Mg2+. However, the anion composition of these water was more atypical, reflecting the common influence from H2CO3-weathered carbonate in addition to H2CO3-weathered silicate and the H2SO4-weathered carbonate. These observations indicated that the solutes of the river water in the Bishuiyan basin were mainly controlled by carbonate weathering, silicate weathering, and atmospheric precipitation. Allogenic acids due to human activity also likely contributed from atmospheric precipitation. In addition, chemical weathering of the rock was primarily due to H2CO3-weathered carbonate, followed by H2CO3-weathered silicate. The effect of allogenic acids on rock weathering was mainly evident for carbonate, with little apparent effect on silicate.
    Figure 4

    Triangle plots for major cations and anions of Bishuiyan river basin waters.

    Full size image

    Quantitative estimation of water chemical constituents in the Bishuiyan river basin
    Atmospheric input
    The contributions of atmospheric inputs to different river sections of the Bishuiyan subterranean basin were calculated (Table 2). Cation components in the river water clearly varied among regions. Estimated atmospheric contribution rates to the R1, R2, R3, G1, and G2 water were 19.5–45.3% (average 33.2%), 19.7–35.9% (average 26.9%), 4.26–7.94% (average 5.26%), 4.53–5.58% (average 4.93%), and 4.94–10.1% (average 7.99%), respectively. The upper reaches were most affected by atmospheric inputs, while such influences were minimal in water in the carbonate area. In addition, the underground river was more resistant to contributions from atmospheric input compared to the surface river, as indicated by a smaller influence in ionic composition.
    Table 2 Contributions from different inputs to cation contents in water samples from the Bishuiyan Basin.
    Full size table

    Silicate weathering
    The average contributions of silicate weathering to the cation content of water samples in the research area were estimated for R1, R2, R3, G1, and G2 waters as 38.9%, 37.5%, 5.59%, 6.45%, and 10.1%, respectively (Table 2). The R1 sample was from water that were primarily granite-hosted. Hence, the influence of silicate weathering was significantly larger in R1, and the corresponding contribution change was larger than that of other river section water. This result was consistent with those described above, indicating that the weathering rate of silicate was greatly affected by seasonal changes.
    Carbonate weathering
    The average contribution of carbonate weathering to the cation content of R1, R2, R3, G1, and G2 samples were 27.3%, 35.0%, 89.3%, 88.5%, and 81.7%, respectively (Table 2). The results clearly indicated that during river runoff, increased contact with carbonate resulted in a gradual increase of carbonate components to the river water. Quantitative analysis also indicated that the water chemistry of the surface water or the underground river in the carbonate area was mainly controlled by the carbonate.
    In summary, the analyses indicated differences in relative contributions of different endmembers to the solutes of different sections of the river. Silicate contributed most to the R1 and R2 water, followed by carbonate and then atmospheric input. Although there was only a small amount of carbonate in peripheral areas of R1, while the contributions of carbonate weathering and silicate weathering to the river solute were similar, due to the rapid dissolution44 or mixed dissolution45,46. The water chemistry of R1 and R2 may be typically controlled by silicate and carbonate weathering. In contrast, R3, G1, and G2 were primarily influenced by carbonate, silicate, and then atmospheric input. These results are consistent with the geological setting of the Bishuiyan subterranean basin, wherein water chemistry exhibits obvious regional characteristics. Lastly, the water chemistry of the Chuanyan branch water and the exposed underground river in the carbonate area (R3, G1, and G2), were mainly controlled by the weathering of carbonate.
    The chemical weathering rate of rocks in the Bishuiyan basin and the consumption of atmospheric CO2
    The chemical weathering rate of rock minerals (t/(km2 year)) is generally reflective of the embodiment of the weathering product of the rock minerals in the solutes of the river per unit area. Chemical weathering of carbonate and silicate was the primary control on the water chemical composition of the Bishuiyan subterranean basin. Relevant water chemistry and river flow data for the basin could then be used to calculate the weathering rate of silicate and carbonate, in addition to the consumption of atmospheric CO2, following previously described methods9,47 as indicated below.
    Silicate weathering rate (SWR):

    $$ {text{SWR}} = {{left( {left[ {{text{Na}}} right]_{{{text{sil}}}} + left[ {text{K}} right]_{sil} + left[ {{text{Ca}}} right]_{{{text{sil}}}} + left[ {{text{Mg}}} right]_{sil} + left[ {{text{SiO}}_{{2}} } right]} right) times {text{Q}}_{{{text{annual}}}} } mathord{left/ {vphantom {{left( {left[ {{text{Na}}} right]_{{{text{sil}}}} + left[ {text{K}} right]_{sil} + left[ {{text{Ca}}} right]_{{{text{sil}}}} + left[ {{text{Mg}}} right]_{sil} + left[ {{text{SiO}}_{{2}} } right]} right) times {text{Q}}_{{{text{annual}}}} } {text{A}}}} right. kern-nulldelimiterspace} {text{A}}} $$
    (13)

    Carbonate weathering rate (CWR):

    $$ {text{CWR}} = {{left( {left[ {{text{Ca}}} right]_{{{text{carb}}}} + left[ {{text{Mg}}} right]_{{{text{carb}}}} + 1/2left[ {{text{HCO}}_{{3}} } right]_{{{text{carb}}}}^{{}} } right) times {text{Q}}_{{{text{annual}}}} } mathord{left/ {vphantom {{left( {left[ {{text{Ca}}} right]_{{{text{carb}}}} + left[ {{text{Mg}}} right]_{{{text{carb}}}} + 1/2left[ {{text{HCO}}_{{3}} } right]_{{{text{carb}}}}^{{}} } right) times {text{Q}}_{{{text{annual}}}} } {text{A}}}} right. kern-nulldelimiterspace} {text{A}}} $$
    (14)

    CO2 consumption rate during silicate and carbonate weathering:

    $$ phi {text{CO}}_{{2}_{text{sil}}} = ({text{Na}}_{sil} + {text{K}}_{sil} + 2{text{Mg}}_{sil} + 2{text{Ca}}_{sil} ) times {text{Q}}_{text{annual}}/{text{A}}$$
    (15)

    $$ phi {text{CO}}_{{2}_{{{text{car}}}}} = {{({text{Mg}}_{{{text{car}}}} + {text{Ca}}_{car} ) times {text{Q}}_{{{text{annual}}}} } mathord{left/ {vphantom {{({text{Mg}}_{{{text{car}}}} + {text{Ca}}_{car} ) times {text{Q}}_{{{text{annual}}}} } {text{A}}}} right. kern-nulldelimiterspace} {text{A}}} $$
    (16)

    The cations produced by the weathering of carbonate and silicate can be calculated from Eqs. (3)–(10). To calculate the weathering rate of carbonate, the corresponding (left[ {{text{HCO}}_{{3}} } right]_{{{text{carb}}}}^{{}}) value is first obtained. When the weathering rate of H2CO3-weathered carbonate and CO2 consumption are calculated, it is necessary to deduct the (left[ {{text{HCO}}_{{3}}^{ – } } right]_{{{text{carb}}}}^{{{text{H}}_{2} {text{SO}}_{4} + {text{HNO}}_{3} }}) released by allogenic acid due to [HCO3−]carb. If the ions are balanced in the process of silicate solution and erosion by H2CO3, then the following equation can be used:

    $$ left[ {{text{HCO}}_{3}^{ – } } right]_{{{text{sil}}}} = {text{CO}}_{{{2}}_{{{text{sil}}}}} = left[ {{text{Na}}^{ + } } right]_{{{text{sil}}}} + left[ {{text{K}}^{ + } } right]_{{{text{sil}}}} + 2left[ {{text{Ca}}^{2 + } } right]_{{{text{sil}}}} + 2left[ {{text{Mg}}^{2 + } } right]_{{{text{sil}}}} $$
    (17)

    where the [HCO3−]sil is the HCO3− produced by silicate that is dissolved and eroded by H2CO3 in the water and CO2sil refers to the atmospheric CO2 that is consumed in the process of dissolution and erosion.
    To determine the [HCO3−]carb produced during weathering of carbonate (including carbonic acid and allogenic acid dissolution and erosion), the following equation can be used:

    $$ begin{aligned} left[ {{text{HCO}}_{{3}}^{ – } } right]_{carb} &= left[ {{text{HCO}}_{{3}}^{ – } } right]_{carb}^{{{text{H}}_{2} {text{CO}}_{3} }} + left[ {{text{HCO}}_{{3}}^{ – } } right]_{carb}^{{{text{H}}_{2} {text{SO}}_{4} + {text{HNO}}_{3} }} \ & = left[ {{text{HCO}}_{{3}}^{ – } } right]_{total} – left[ {{text{HCO}}_{{3}}^{ – } } right]_{sil} \ end{aligned} $$
    (18)

    where [HCO3−]total is the total HCO3− of the water; [HCO3−]carb is the HCO3- produced by dissolution and erosion of carbonate in the water; (left[ {{text{HCO}}_{{3}}^{ – } } right]_{carb}^{{{text{H}}_{2} {text{CO}}_{3} }}) is the HCO3− produced by carbonate that are dissolved and eroded by H2CO3; and (left[ {{text{HCO}}_{{3}}^{ – } } right]_{carb}^{{{text{H}}_{2} {text{SO}}_{4} + {text{HNO}}_{3} }}) is the HCO3- produced by carbonate dissolution and erosion by allogenic acids (H2SO4 and HNO3) in the water.
    The quantity of HCO3− from various sources and the influence of various acids on the weathering of carbonate can be assessed via Eqs. (6) and (7). The weathering rate of H2CO3-weathered silicate, the weathering rate of carbonate eroded by carbonic acid and allogenic acids in the Bishuiyan subterranean basin, and the consumption of CO2 in corresponding process can be calculated using Formulas (2)–(8) (Table 3).

    $$ begin{aligned} left[ {{text{HCO}}_{3}^{ – } } right]_{{{text{carb}}}}^{{{text{H}}_{2} {text{CO}}_{3} }} &= 2 times left[ {{text{Ca}}^{2 + } + {text{Mg}}^{2 + } } right]_{{{text{carb}}}}^{{{text{H}}_{2} {text{CO}}_{3} }} \ & = 2 times left( {left[ {{text{HCO}}_{3}^{ – } } right]_{{{text{carb}}}} – left[ {{text{Ca}}^{{{2} + }} + {text{Mg}}^{{{2} + }} } right]_{{{text{carb}}}} } right) \ end{aligned} $$
    (19)

    Table 3 Weathering rates and CO2 consumption in the Bishuiyan subterranean basin waters.
    Full size table

    The quantitative calculation of water chemistry resulted in an estimated rock weathering rate for the basin of 73.3 t/(km2 year), and an atmospheric CO2 consumption flux of 668 × 103 mol/(km2 year), which are significant higher than the global rock weathering rate of 36 t/(km2 year) and the global atmospheric CO2 consumption flux of 246 × 103 mol/(km2 year)21. The weathering rate and CO2 consumption flux in this study were slightly higher than the values in Yangtze basin, which were 85 t/(km2 year) and 611 × 103 mol/(km2 year), respectively21. There are obvious climatic regional difference in the weathering rate and corresponding carbon sink capacity of the basin. For instance, Bishuiyan subterranean basin was subtropical monsoon climate, where the chemical weathering rate and atmospheric CO2 consumption flux were similar to the Pearl River basin and some tributaries of the Amazon basin (tropical rainforest climate)18,48. However, the corresponding values were significant lower than those in the Lesser Antilles (hot and humid climate, average annual temp. 24–28 ℃, average annual rainfall 2,400–4,600 mm), where the rock weathering rate and atmospheric CO2 consumption flux were (100–120 t/(km2 year)) and ((1,100–1,400) × 103 mol/(km2 year)), respectively49. Meanwhile, the corresponding values in this study were lower than those in northern Okinawa Island (subtropical and humid climate, average annual temp. 22.2℃, average annual rainfall above 2000 mm) with the fluxes of CO2 consumed by silicate ((334–471) × 103 mol/(km2 year))50. The rock weathering rate and atmospheric CO2 consumption flux of the basin located in the plateau climate and arid and semi-arid climate regions (low rainfall) were lower than those in hot and humid climate (high rainfall). The weathering rate and atmospheric CO2 consumption flux in Xinjiang rivers (average annual temp. 7–8 ℃, average annual rainfall 100–276 mm) were 0.12–93.6 t/(km2 year) and (0.19–284) × 103 mol/(km2 year), respectively29. The weathering rate of rock and atmospheric CO2 consumption flux in the Songhua River basin (average annual temp. 3–5 ℃, average annual rainfall 500 mm) were (5.79 t/(km2 year)) and 190 × 103 mol/(km2 year), respectively9. The atmospheric CO2 consumption flux in upper Yellow River in the Qinghai-Tibet Plateau (average annual temp. 1–8 ℃, average annual rainfall 434 mm) was 268 × 103 mol/(km2 year)51.
    Compared to the other small karst watersheds of in the similar climate, the atmospheric CO2 consumption flux in the study area was lower than that in Xiangxi Dalongdong underground river (819 × 103 mol/(km2 year), average annual rainfall 1,800 mm) and four underground rivers in upstream of Wushui (878 × 103 mol/(km2 year), average annual rainfall 1,444 mm). Meanwhile, the corresponding value was similar to that of Wanhuayan underground river (705 × 103 mol/(km2 year), average annual rainfall 1565 mm)52. However, compared with the north karst of China53,54, the CO2 consumption flux in the study area was higher, resulting in the greater contribution to the rock weathering.
    The comparison with other climatic zones in the world showed that the CO2 consumption caused by chemical weathering in the hot and humid climate zone is an important part of regulating atmospheric CO2 and constituting the global carbon balance. Besides, the small basins in karst (subtropical) area had relatively higher CO2 consumption. Therefore, the potential of chemical weathering carbon sink in some small subtropical basins with a wide distribution of carbonate is worth additional attention, which would provide some new insights for the scientific assessment of carbon sink effects caused by chemical weathering. Overall, the weathering of carbonate accounts for 71.2% (476 × 103 mol/(km2 year)) of the carbon sink flux of weathered rocks in the Bishuiyan basin, while the weathering of silicate only accounts for 28.3% (192 × 103 mol/(km2 year)). It indicates that more attention should be paid to the accurate assessment of the carbonate carbon sink intensity at the global and regional scales, the role and status of carbonate chemical weathering actively involved in the geological carbon cycle, is worth further study. More

  • in

    Juvenile hormone regulates the shift from migrants to residents in adult oriental armyworm, Mythimna separata

    1.
    Chapman, J. W., Reynolds, D. R. & Wilson, K. Long-range seasonal migration in insects: mechanisms, evolutionary drivers and ecological consequences. Ecol. Lett. 18, 287–302 (2015).
    PubMed  Google Scholar 
    2.
    Zera, A. J. & Tiebel, K. C. Brachypterizing effect of group rearing, juvenile hormone-III, and methoprene on wing length development in the wingdimorphic cricket, Gryllus rubens. J. Insect. Physiol. 34, 489–498 (1988).
    CAS  Google Scholar 

    3.
    Mittler, T. E. Juvenile hormone and aphid polymorphism. In: Morphogenetic Hormones of Arthropods (ed Gupta, A. P.). vol. 3. Rutgers Univ, New Brunswick. 453-474 (1991).

    4.
    Nijhout, H. F. Control mechanisms of polyphenic development in insects. Biosci 49, 181–192 (1999).
    Google Scholar 

    5.
    Rankin, M. A. & Rankin, S. Some factors affecting presumed migratory flight activity of the convergent ladybeetle, Hippodamia convergens (Coccinellidae: Coleoptera). Biol. Bull. 158(3), 356–369 (1980).
    Google Scholar 

    6.
    Wang, F. Y., Zhang, X. X. & Zhai, B. P. Flight and re-migration capacity of the rice leaf folder moth, Cnaphalocrocis medinalis (Guenée) (Lepidoptera: Crambidae). Acta Entomol. Sin 53(11), 1265–1272 (2010).
    Google Scholar 

    7.
    Nakasuji, F. & Nakano, A. Flight activity and oviposition characteristics of the seasonal form of a migrant skipper, Parnara guttata guttata (Lepidoptera: Hesperiidae). Res. Pop. Ecol. 32, 227–233 (1990).
    Google Scholar 

    8.
    Shirai, Y. Flight activity, reproduction, and adult nutrition of the beet webworm, Spoladea recurvalis (Lepidoptera: Pyralidae). Appl. Entomol. Zool. 41, 405–414 (2006).
    Google Scholar 

    9.
    Cheng, Y. X., Luo, L. Z., Jiang, X. F. & Sappington, T. W. Synchronized oviposition triggered by migratory flight intensifies larval outbreaks of beet webworm. PLOS ONE 7, e31562, https://doi.org/10.1371/journal.pone.0031562 (2012).
    ADS  CAS  Article  PubMed  PubMed Central  Google Scholar 

    10.
    Zhang, L., Pan, P., Sappington, T. W., Lu, W. X. & Luo, L. Z. Accelerated and synchronized oviposition induced by flight of young females may intensify larval outbreaks of the rice leaf roller. PLoS ONE. 8(5), e63554 (2015).
    Google Scholar 

    11.
    Zera, A. J. & Denno, R. F. Physiology and ecology of dispersal polymorphism in insects. Annu. Rev. Entomol. 42, 207–231 (1997).
    CAS  PubMed  Google Scholar 

    12.
    Zera, A. J. The endocrine regulation of wing polymorphism in insects: state of the art, recent surprises, and future directions. Integr. Comp. Biol. 43, 607–616 (2004).
    Google Scholar 

    13.
    Zera, A. J. Evolutionary genetics of juvenile hormone and ecdysteroid regulation in Gryllus: A case study in the microevolution of endocrine regulation. Comp. Biochem. Physiol. A 144, 365–379 (2006).
    Google Scholar 

    14.
    Zera, A. J. Endocrine analysis in evolutionary-developmental studies of insect polymorphism: hormone manipulation versus direct measurement of hormonal regulators. Evol. Dev 9, 499–513 (2007).
    CAS  PubMed  Google Scholar 

    15.
    Hardie, J. Juvenile hormone and photoperiodically controlled polymorphism in Aphis fabae: prenatal effects on presumptive oviparae. J. Insect Physiol. 27, 257–265 (1981).
    CAS  Google Scholar 

    16.
    Hardie, J., Honda, K., Timar, T. & Varjas, L. Effects of 2, 2-dimethylchromene derivatives on wing determination and metamorphosis in the pea aphid, Acyrthosiphon pisum. Arch. Insect Biochem. Physiol. 30, 25–40 (1995).
    CAS  Google Scholar 

    17.
    Ayoade, O., Morooka, S. & Tojo, S. Enhancement of short wing formation and ovarian growth in the genetically defined macropterous strain of the brown planthopper, Nilaparvata lugens. J. Insect Physiol. 45, 93–100 (1999).
    CAS  PubMed  Google Scholar 

    18.
    Sun, B. B. et al. Methoprene influences reproduction and flight capacity in adults of the rice leaf roller, Cnaphalocrocis Medinalis (Guenée) (Lepidoptera: Pyralidae). Arch. Insect Biochem. Physiol. 82(1), 1–13 (2013).
    CAS  PubMed  Google Scholar 

    19.
    Tanaka, S. Endocrine control of ovarian development and flight muscle histolysis in a wing dimorphic cricket, Modicogryllus confirmatus. J. Insect Physiol. 40, 483–490 (1994).
    CAS  Google Scholar 

    20.
    Zera, A. J. & Cisper, G. Genetic and diurnal variation in the juvenile hormone titer in a wing-polymorphic cricket: implications for the evolution of life histories and dispersal. Physiol. Biochem. Zool. 74, 293–306 (2001).
    CAS  PubMed  Google Scholar 

    21.
    Socha, R. & Kula, J. Differential allocation of protein resources to flight muscles and reproductive organs in the flightless wing-polymorphic bug, Pyrrhocoris apterus (L.) (Heteroptera). J. Comp. Physiol. B. 178, 179–188 (2008).
    CAS  PubMed  Google Scholar 

    22.
    Lu, K. et al. Nutritional signaling regulates vitellogenin synthesis and egg development through juvenile hormone in Nilaparvata lugens (Stål). Int. J. Mol. Sci. 17, 269 (2016).
    Google Scholar 

    23.
    Han, E. N. & Gatehouse, A. G. Effect of temperature and photoperiod on the calling behaviour of a migratory insect, the oriental armyworm Mythimna separata. Physiol. Entomol. 16, 419–427 (1991).
    Google Scholar 

    24.
    Luo, L. Z., Li, G. B., Cao, Y. Z. & Hu, Y. The influence of larval rearing density on flight capacity and fecundity of adult oriental armyworm, Mythimna separata (walker). Acta Entomol. Sin 38, 38–45 (1995).
    Google Scholar 

    25.
    Cao, Y. Z., Luo, L. Z. & Guo, J. Performance of adult reproduction and flight in relation to larval nutrition in the oriental armyworm, Mythimna separate (Walker). Acta Entomol. Sin 39, 105–108 (1996).
    Google Scholar 

    26.
    Jiang, X. F., Luo, L. Z. & Hu, Y. Influences of rearing temperature on flight and reproductive capacity of adult oriental armyworm, Mythimna separata (Walker). Acta Entomol. Sin 20, 288–292 (2000).
    Google Scholar 

    27.
    Jiang, X. F., Luo, L. Z. & Hu, Y. Genetic characteristics of pre-oviposition period in the oriental armyworm Mythimna separata (Walker). Acta Entomol. Sin 25, 68–72 (2005).
    Google Scholar 

    28.
    Jiang, X. F., Luo, L. Z. & Zhang, L. Amplified fragment length polymorphism analysis of the oriental armyworm, Mythimna separata (Walker) geographic and melanic laboratory populations in China. J. Econ. Entomol 100, 1525–1532 (2007).
    CAS  PubMed  Google Scholar 

    29.
    Wang, Y. Z. & Zhang, X. X. Studies on the migratory behaviours of oriental armyworm, Mythimna separata (Walker). Acta Ecol. Sin 21, 772–779 (2001).
    Google Scholar 

    30.
    Zhang, L., Luo, L. Z., Jiang, X. F. & Hu, Y. Influences of starvation on the first day after emergence on ovarian development and flight potential in adults of the oriental armyworm, Mythimna separata (Walker) (Lepidopterea: Noctuidae). Acta Entomol. Sin 49, 895–902 (2006).
    Google Scholar 

    31.
    Zhang, L., Luo, L. Z. & Jiang, X. F. Starvation influences allatotropin gene expression and juvenile hormone titer in the female adult oriental armyworm, Mythimna separata. Arch Insect Biochem. Physiol. 68, 63–70 (2008a).
    CAS  PubMed  Google Scholar 

    32.
    Zhang, L., Jiang, X. F. & Luo, L. Z. Determination of sensitive stage for switching migrant oriental armyworms into residents. Environ. Entomol 37, 1389–1395 (2008b).
    PubMed  Google Scholar 

    33.
    Jiang, X. F. & Luo, L. Z. Comparison of behavioral and physiological characteristics between the emigrant and immigrant populations of the oriental armyworm, Mythimna separata (Walker). Acta Entomol. Sin 48, 61–67 (2005).
    Google Scholar 

    34.
    Jiang, X. F., Luo, L. Z., Zhang, L., Sappington, T. W. & Hu, Y. Regulation of migration in the oriental armyworm, Mythimna separata (Walker) in China: A review integrating environmental, physiological, hormonal, genetic, and molecular factors. Environ. Entomol. 40(3), 516–533 (2011).
    CAS  PubMed  Google Scholar 

    35.
    Li, K. B. et al. Influences of flight on energetic reserves and juvenile hormone synthesis by corpora allata of the oriental armyworm, Mythimna separata (Walker). Acta Entomol. Sin 48, 155–160 (2005).
    CAS  Google Scholar 

    36.
    Luo, L. Z., Li, K. B., Jiang, X. F. & Hu, Y. Regulation of flight capacity and contents of energy substances by methoprene in the moths of oriental armyworm, Mythimna separata. Acta Entomol. Sin 8, 63–72 (2001).
    CAS  Google Scholar 

    37.
    Teal, P. E. A., Gomez-Simuta, Y. & Proveaux, A. T. Mating experience and juvenile hormone enhance sexual signaling and mating in male Caribbean fruit flies. Proc. Natl. Acad. Sci. USA 97, 3708–3712 (2000).
    ADS  CAS  PubMed  Google Scholar 

    38.
    Rafaeli, A., Zakharova, T., Lapsker, Z. & Jurenka, R. A. The identification of an age- and female- specific putative PBAN membrane-receptor protein in pheromone glands of Helicoverpa armigera: possible up-regulation by Juvenile Hormone. Insect Biochem. Mol. Biol. 33, 371–380 (2003).
    CAS  PubMed  Google Scholar 

    39.
    Zera, A. J., Zhao, Z. & Kaliseck, K. Hormones in the field: evolutionary endocrinology of juvenile hormone and ecdysteroids in field populations of the wingdimorphic cricket Gryllus firmus. Physiol. Biochem. Zool. 80, 592–606 (2007).
    CAS  PubMed  Google Scholar 

    40.
    Nijhout, H. F. Development and evolution of adaptive polyphenisms. Evol. Dev. 5, 9–18 (2003).
    PubMed  Google Scholar 

    41.
    Roy, S., Saha, T. T., Zou, Z. & Raikhel, A. S. Regulatory pathways controlling female insect reproduction. Annu. Rev. Entomol. 63, 489–511 (2018).
    CAS  PubMed  Google Scholar 

    42.
    Barbora, K. & Marek, J. Juvenile hormone resistance gene Methoprene-tolerant controls entry into metamorphosis in the beetle Tribolium castaneum. Proc. Natl. Acad. Sci. USA 104, 10488–10493 (2007).
    Google Scholar 

    43.
    Baumann, A., Barry, J., Wang, S., Fujiwara, Y. & Wilson, T. G. Paralogous genes involved in juvenile hormone action in Drosophila melanogaster. Genetics 185, 1327–1336 (2010).
    CAS  PubMed  PubMed Central  Google Scholar 

    44.
    Riddiford, L. M., Truman, J. W., Mirth, C. K. & Shen, Y. C. A role for juvenile hormone in the prepupal development of drosophila melanogaster. Development 137, 1117–1126 (2010).
    CAS  PubMed  PubMed Central  Google Scholar 

    45.
    Abdou, M. A. et al. Drosophila met and gce are partially redundant in transducing juvenile hormone action. Insect Biochem. Mol. Biol. 41, 938–945 (2011).
    CAS  PubMed  Google Scholar 

    46.
    Charles, J. P. et al. Ligand-binding properties of a juvenile hormone receptor, Methoprene-tolerant. Proc. Natl. Acad. Sci. USA 108, 21128–21133 (2011).
    ADS  CAS  PubMed  Google Scholar 

    47.
    Li, M., Mead, E. A. & Zhu, J. Heterodimer of two bHLH-PAS proteins mediates juvenile hormone- induced gene expression. Proc. Natl. Acad. Sci. USA 108, 638–643 (2011).
    ADS  CAS  PubMed  Google Scholar 

    48.
    Bernardo, T. J. & Dubrovsky, E. B. The Drosophila juvenile hormone receptor candidates Methoprene-tolerant (Met) and germ cell-expressed (gce) utilize a conserved LIXXL motif to bind the FTZ-F1 nuclear receptor. J. Biol. Chem. 287, 7821–7833 (2012).
    CAS  PubMed  PubMed Central  Google Scholar 

    49.
    Bernardo, T. J. & Dubrovsky, E. B. Molecular mechanisms of transcription activation by juvenile hormone: a critical role for bHLH-PAS and nuclear receptor proteins. Insects 3, 324–338 (2012).
    PubMed  PubMed Central  Google Scholar 

    50.
    Zhang, Z. L., Xu, J., Sheng, Z., Sui, Y. & Palli, S. R. Steroid receptor co-activator is required for juvenile hormone signal transduction through a bHLH-PAS transcription factor, Methoprene tolerant. J. Biol. Chem. 286, 8437–8447 (2011).
    CAS  PubMed  Google Scholar 

    51.
    Jindra, M., Uhlirova, M., Charles, J. P., Smykal, V. & Hill, R. J. Genetic evidence for function of the bHLH-PAS protein Gce /Met as a juvenile hormone receptor. PLoS. Genet. 11(7), e1005394 (2015).
    PubMed  PubMed Central  Google Scholar 

    52.
    Parthasarathy, R. & Palli, S. R. Molecular analysis of nutritional and hormonal regulation of female reproduction in the red flour beetle. Tribolium castaneum. Insect Biochem. Mol. Biol 41, 294–305 (2011).
    CAS  PubMed  Google Scholar 

    53.
    Guo, W. et al. Juvenile hormone-receptor complex acts on Mcm4 and Mcm7 to promote polyploidy and vitellogenesis in the migratory locust. PLOS Genet. 10, e1004702 (2014).
    PubMed  PubMed Central  Google Scholar 

    54.
    Luo, M. et al. Juvenile hormone differentially regulates two Grp78 genes encoding protein chaperones required for insect fat body cell homeostasis and vitellogenesis. J. Biol. Chem. 292, 8823–34 (2017).
    CAS  PubMed  PubMed Central  Google Scholar 

    55.
    Song, J., Wu, Z., Wang, Z., Deng, S. & Zhou, S. Krüppel-homolog 1 mediates juvenile hormone action to promote vitellogenesis and oocyte maturation in the migratory locust. Insect Biochem. Mol. Biol. 52, 94–101 (2014).
    CAS  PubMed  Google Scholar 

    56.
    Wu, Z., Guo, W., Xie, Y. & Zhou, S. Juvenile hormone activates the transcription of cell-division-cycle 6 (Cdc6) for polyploidy-dependent insect vitellogenesis and oogenesis. J. Biol. Chem. 291, 5418–27 (2016).
    CAS  PubMed  PubMed Central  Google Scholar 

    57.
    Wang, Z., Yang, L., Song, J., Kang, L. & Zhou, S. An isoform of Taiman that contains a PRD-repeat motif is indispensable for transducing the vitellogenic juvenile hormone signal in Locusta migratoria. Insect Biochem. Mol. Biol. 82, 31–40 (2017).
    CAS  PubMed  Google Scholar 

    58.
    Cruz, J., Martin, D., Pascual, N., Maestro, J. L. & Piulachs, M. D. Quantity does matter: juvenile hormone and the onset of vitellogenesis in the German cockroach. Insect Biochem. Mol. Biol. 33, 1219–25 (2003).
    CAS  PubMed  Google Scholar 

    59.
    Gujar, H. & Palli, S. R. Juvenile hormone regulation of female reproduction in the common bed bug, Cimex lectularius. Sci. Rep 6, 35546 (2016).
    ADS  CAS  PubMed  PubMed Central  Google Scholar 

    60.
    Marchal, E., Hult, E. F., Huang, J., Pang, Z. & Stay, B. Methoprene-tolerant (Met) knockdown in the adult female cockroach, Diploptera punctata, completely inhibits ovarian development. PLOS ONE 9, e106737 (2014).
    ADS  PubMed  PubMed Central  Google Scholar 

    61.
    Luo, L. Z., Jiang, X. F., Li, K. B. & Hu, Y. Influences of flight on reproduction and longevity of the oriental armyworm, Mythimna separata (Walker). Acta Entomol. Sin 42, 150–158 (1999).
    Google Scholar 

    62.
    Luo, L. Z. & Li, G. B. Ultrastructure of the flight muscle of adult oriental armyworm, Mythimna separata (Walker). Acta Entomol. Sin 39(2), 141–148 (1996).
    ADS  Google Scholar 

    63.
    Luo, L. Z. An ultrastructural study on the development of flight muscle in adult oriental armyworm, Mythimna separata (Walker). Acta Entomol. Sin 39(4), 366–374 (1996).
    MathSciNet  Google Scholar 

    64.
    Socha, R. & Šula, J. Flight muscles polymorphism in a flightless bug, Pyrrhocoris apterus (L.): Developmental pattern, biochemical profile and endocrine control. J. Insect Physiol. 52, 231–239 (2006).
    CAS  PubMed  Google Scholar 

    65.
    SAS Institute. SAS/STAT User’s Guide, Release 6.03 Ed. SAS Instisute, Cary, NC. (1988). More

  • in

    Mid and long-term ecological impacts of ski run construction on alpine ecosystems

    1.
    Rixen, C. et al. Winter tourism and climate change in the Alps: an assessment of resource consumption snow reliability and future snowmaking potential. Mt. Res. Dev. 31, 229–236 (2011).
    Google Scholar 
    2.
    Vanat, L. International Report on Snow & Mountain Tourism: Overview of the Key Industry Figures for Ski Resorts, 10th edition (2018).

    3.
    Negro, M. et al. Differential responses of ground dwelling arthropods to ski-piste restoration by hydroseeding. Biodivers. Conserv. 22, 2607–2634 (2013).
    Google Scholar 

    4.
    Körner, C. The Alpine life zone under global change. Gayana Bot. https://doi.org/10.4067/S0717-66432000000100001 (2000).
    Article  Google Scholar 

    5.
    Garcı́a-Llorente, M. et al. What can conservation strategies learn from the ecosystem services approach? Insights from ecosystem assessments in two Spanish protected areas. Biodivers. Conserv. 27, 1575–1597 (2016).

    6.
    Egan, P. A. & Price, M. F. Mountain Ecosystem Services and Climate Change. A Global Overview of Potential Threats and Strategies for Adaptation (UNESCO, Paris, 2017).
    Google Scholar 

    7.
    MeijerzuSchlochtern, M. P., Rixen, C., Wipf, S. & Cornelissen, J. H. C. Management, winter climate and plant–soil feedbacks on ski slopes: a synthesis. Ecol. Res. 29, 583–592 (2014).
    CAS  Google Scholar 

    8.
    Gros, R., Monrozier, L. J., Bartoli, F., Chotte, J. L. & Faivre, P. Relationships between soil physico-chemical properties and microbial activity along a restoration chronosequence of alpine grasslands following ski run construction. Appl. Soil Ecol. 27, 7–22 (2004).
    Google Scholar 

    9.
    Barni, E., Freppaz, M. & Siniscalco, C. Interactions between Vegetation, Roots, and Soil Stability in Restored High-altitude Ski Runs in the Alps. Arct. Antarct. Alp. Res. 39, 25–33 (2007).
    Google Scholar 

    10.
    Pohl, M., Alig, D., Körner, C. & Rixen, C. Higher plant diversity enhances soil stability in disturbed alpine ecosystems. Plant Soil 324, 91–102 (2009).
    CAS  Google Scholar 

    11.
    Burt, J. W. & Rice, K. J. Not all ski slopes are created equal: Disturbance intensity affects ecosystem properties. Ecol. Appl. 19, 2242–2253 (2009).
    PubMed  Google Scholar 

    12.
    Van Andel, J., Bakker, J. P., Bakker, J. P. & Grootjans, A. P. Mechanism of vegetation succession: a review of concepts and perspectives. Acta Bot. Neerlandica 42, 413–433 (1993).
    Google Scholar 

    13.
    Styczen, M. E. & Morgan, R. P. C. Engineering properties of vegetation 5–58 (E and FN Spon, New York, 1995).
    Google Scholar 

    14.
    Gray, D. H. & Sotir, R. B. Biotechnical and Soil Bioengineering Slope Stabilization: A Practical Guide for Erosion Control (Wiley, New York, 1996).
    Google Scholar 

    15.
    Gray, D. H. & Leiser, A. T. Biotechnical Slope Protection and Erosion Control (Van Nostrand Reinhold Company, London, 1982).
    Google Scholar 

    16.
    Argenti, G. & Ferrari, L. Plant cover evolution and naturalisation of revegetated ski runs in an Apennine ski resort (Italy). Forest 2, 178–182 (2009).
    Google Scholar 

    17.
    Pintaldi, E. et al. Hummocks affect soil properties and soil-vegetation relationships in a subalpine grassland (North-Western Italian Alps). CATENA 145, 214–226 (2016).
    Google Scholar 

    18.
    Stokes, A. et al. Ecological mitigation of hillslope instability: ten key issues facing researchers and practitioners. Plant Soil 377, 1 (2014).
    CAS  Google Scholar 

    19.
    Burt, J. W. & Clary, J. J. Initial disturbance intensity affects recovery rates and successional divergence on abandoned ski slopes. J. Appl. Ecol. 53, 607–615 (2016).
    Google Scholar 

    20.
    Krautzer, B. et al. The influence of recultivation technique and seed mixture on erosion stability after restoration in mountain environment. Nat. Haz. 56, 547–557 (2011).
    Google Scholar 

    21.
    Pintaldi, E. et al. Sustainable soil management in ski areas: threats and challenges. Sustainability 9, 2150 (2017).
    Google Scholar 

    22.
    Pohl, M., Stroude, R., Buttler, A. & Rixen, C. Functional traits and root morphology of alpine plants. Ann. Bot. 108, 537–545 (2011).
    PubMed  PubMed Central  Google Scholar 

    23.
    Körner, C. Alpine Plant Life Functional Plant Ecology of High Mountain Ecosystems (Springer-Verlag, Berlin, 2003).
    Google Scholar 

    24.
    Mercalli, L. Atlante climatico della Valle d’Aosta (Società Meteorologica Italiana, Rome, 2003).
    Google Scholar 

    25.
    FAO-ISRIC. World Reference Base for Soil Resources 2014. World Soil Resources Reports No. 103 (FAO, 2014).

    26.
    Shannon, C. E. & Wiener, W. The Mathematical Theory of Communication (University Illinois Press, Champaign, 1963).
    Google Scholar 

    27.
    Van Andel, J. & Aronson, J. Restoration Ecology. The New Frontier 2nd edn. (Wiley-Blackwell, New York, 2012).
    Google Scholar 

    28.
    Landolt, E. et al. Flora Indicativa: Okologische Zeigerwerte und Biologische Kennzeichen zur Flora der Schweiz und der Alpen (Haupt, Bern, 2010).
    Google Scholar 

    29.
    Bovio, M. Lista Rossa e Lista Nera della flora vascolare della Valle d’Aosta (Italia, Alpi Nord-occidentali). Aggiornamento anno 2016. Rev. Valdôtaine Hist. Nat. 70, 57–74 (2016).
    Google Scholar 

    30.
    Rossi, G. et al. Lista Rossa della Flora Italiana. 1. Policy Species e Altre Specie Minacciate (Comitato Italiano IUCN e Ministero dell’Ambiente e della Tutela del Territorio e del Mare, Rome, 2013).
    Google Scholar 

    31.
    Aeschimann, P., Lauber, K., Moser, D. M. & Theurillat, J. P. Flora Alpina (Haupt Verlag, Bern, 2004).
    Google Scholar 

    32.
    Van Reeuwijk, L. P. Procedures for Soil Analysis. Technical Paper n. 9 (International Soil Reference and Information Centre, Wageningen, 2002).

    33.
    Zanini, E., Bonifacio, E., Alberston, J. D. & Nielsen, D. R. Topsoil aggregate breakdown under water-saturated conditions. Soil. Sci. 163, 288–298 (1998).
    ADS  CAS  Google Scholar 

    34.
    Kruskal, J. B. Nonmetric multidimensional scaling: a numerical method. Psychometrika 29, 115–129 (1964).
    MATH  MathSciNet  Google Scholar 

    35.
    Oksanen, J. et al. Vegan: community ecology package. R Package Version 2.0-0. ttp://CRAN.Rproject.org/package=vegan (2011).

    36.
    Bates, D., Mächler, M., Bolker, B. & Walker, S. Fitting linear mixed-effects models using lme4. J. Stat. Softw. 67, 1–48 (2015).
    Google Scholar 

    37.
    Wipf, S., Rixen, C., Fischer, M., Schmid, B. & Stoeckli, V. Effects of ski piste preparation on alpine vegetation. J. Appl. Ecol. 42, 306–316 (2005).
    Google Scholar 

    38.
    Roux-Fouillet, P., Wipf, S. & Rixen, C. Long-term impacts of ski piste management on alpine vegetation and soils. J. Appl. Ecol. 48, 906–915 (2011).
    Google Scholar 

    39.
    Delgado, R. et al. Impact of ski pistes on soil properties, a case study from a mountainous area in the Mediterranean region. Soil Use Manag. 23, 269–277 (2007).
    Google Scholar 

    40.
    Argenti, G., Merati, M., Staglianò, N. & Talamucci, P. Establishment and evolution of technical ski slope covers in an alpine environment. Riv. Agron. 34, 186–190 (2000).
    Google Scholar 

    41.
    Krautzer, B. et al. Site-specific high zone restoration in the Alpine region: the current technological development (HBLFA Raumberg-Gumpenstein, Irdning, 2006).
    Google Scholar 

    42.
    Burt, J. W. Developing restoration planting mixes for active ski slopes: a multi-site reference community approach. J. Environ. Manage. 49, 636–648 (2012).
    ADS  Google Scholar 

    43.
    Klug, B. Seed mixtures, seeding methods, and soil seed pools: major factors in erosion control on graded ski-runs. WSEAS Trans. Environ. Dev. 4, 454–459 (2006).
    Google Scholar 

    44.
    Barrel, A. et al. Native Seeds for the Ecological Restoration in Mountain Zone: Production and Use of Preservation Mixtures (Institut Agricole Régional, Aosta, 2015).
    Google Scholar 

    45.
    Hagen, D., Hansen, T.-I., Graae, B. J. & Rydgren, K. To seed or not to seed in alpine restoration: introduced grass species outcompete rather than facilitate native species. Ecol. Eng. 64, 255–261 (2014).
    Google Scholar 

    46.
    Gretarsdottir, J., Aradottir, A. L., Vandvik, V., Heegaard, E. & Birks, H. J. B. Long-term effects of reclamation treatments on plant succession in Iceland. Restor. Ecol. 12, 268–278 (2004).
    Google Scholar 

    47.
    Florineth, F. Pflanzen statt Beton (Handbuch zur Ingenieurbiologie und Vegetationstechnik, Berlin-Hannover, 2004).
    Google Scholar 

    48.
    Lichtenegger, E. Root distribution in some alpine plants. Acta Phytogeogr Suec. 81, 76–82 (1996).
    Google Scholar 

    49.
    Nagelmüller, S., Hiltbrunner, E. & Körner, C. Critically low soil temperatures for root growth and root morphology in three alpine plant species. Alp. Bot. 126, 11–21 (2016).
    Google Scholar 

    50.
    Khan, M. A., Gemenet, D. C. & Villordon, A. Root system architecture and abiotic stress tolerance: current knowledge in root and tuber crops. Front. Plant Sci. 7, 1584 (2016).
    CAS  PubMed  PubMed Central  Google Scholar 

    51.
    Tracy, S. R. et al. Quantifying the impact of soil compaction on root system architecture in tomato (Solanum lycopersicum) by X-ray micro-computed tomography. Ann. Bot. 110, 511–519 (2012).
    PubMed  PubMed Central  Google Scholar 

    52.
    Poorter, H. et al. Biomass allocation to leaves, stems and roots: meta-analyses of interspecific variation and environmental control. New Phytol. 193, 30–50 (2012).
    CAS  PubMed  Google Scholar 

    53.
    Bardgett, R. D., Mommer, L. & De Vries, F. T. Going underground: root traits as drivers of ecosystem processes. Trends Ecol. Evol. 29, 692–699 (2014).
    PubMed  Google Scholar 

    54.
    Hudek, C., Stanchi, S., D’Amico, M. & Freppaz, M. Quantifying the contribution of the root system of alpine vegetation in the soil aggregate stability of moraine. Int. Soil Water Conserv. Res. 5, 36–42 (2017).
    Google Scholar 

    55.
    Gould, I. J., Quinton, J. N., Weigelt, A., De Deyn, G. B. & Bardgett, R. D. Plant diversity and root traits benefit physical properties key to soil function in grasslands. Ecol. Lett. 19, 1140–1149 (2016).
    PubMed  PubMed Central  Google Scholar 

    56.
    Solly, E. F. et al. Unravelling the age of fine roots of temperate and boreal forests. Nat. Commun. 9, 3006 (2018).
    ADS  PubMed  PubMed Central  Google Scholar 

    57.
    Rixen, C., Freppaz, M., Stöckli, V., Huovinen, C. & Wipf, S. Altered snow density and chemistry change soil nitrogen mineralization and plant growth. Arct. Antarct. Alp. Res. 40, 568–575 (2008).
    Google Scholar 

    58.
    Miransari, M. Plant growth promoting Rhizobacteria. J. Plant Nutr. 37, 2227–2235 (2014).
    CAS  Google Scholar 

    59.
    Stokes, A., Atger, C., Bengough, A. G., Fourcaud, T. & Sidle, R. C. Desirable plant root traits for protecting natural and engineered slopes against landslides. Plant Soil 324, 1–30 (2009).
    CAS  Google Scholar 

    60.
    Freppaz, M. et al. Soil Properties on Ski-Runs. In Impacts of Skiing and Related Winter Recreational Activities on Mountain Environments p (eds Rixen, C. & Rolando, A.) 45–64 (Bentham Science Publisher, Sharjah, 2013).
    Google Scholar 

    61.
    Locher Oberholzer, N. et al. Linee Guida per Il Rinverdimento ad Alta Quota; AGHB Bollettino n2 (Luglio, Verein für Ingenieurbiologie, 2008) ((In Italian)).
    Google Scholar 

    62.
    Graf, F. & Brunner, I. Natural and synthesized ectomycorrhizas of the alpine dwarf willow Salix herbacea. Mycorrhiza 6, 227–235 (1996).
    Google Scholar 

    63.
    Graf, F. Ectomycorrhiza in alpine eco-engineering. Rev. Valdôtaine Hist. Nat. 52, 314–323 (1997).
    MathSciNet  Google Scholar 

    64.
    Graf, F. & Gerber, W. Der Einfluss von Mykorrhizapilzen auf die Bodenstruktur und deren Bedeutung für den Lebendverbau Schweiz. Z. Forstwes 11, 863–886 (1997).
    Google Scholar 

    65.
    Frei, M. et al. Quantification of the influence of vegetation on soil stability. In Proceeding of the International Conference on Slope Engineering (Department of Civil Engineering, 2003).

    66.
    Krautzer, B., Graiss, W. & Klug, B. Ecological Restoration of Ski-Runs. The Impacts of Skiing and Related Winter Recreational Activities on Mountain Environments 184–209 (Bentham e books, Sharjah, 2013).
    Google Scholar 

    67.
    Peratoner, G. Organic Seed Propagation of Alpine Species and Their Use in Ecological Restoration of Ski-Runs in Mountain Regions. Diss. Univ. Kassel. Kassel University Press, 238 (2003). More

  • in

    Time to revise the Sustainable Development Goals

    EDITORIAL
    14 July 2020

    The pandemic has set back efforts to achieve the original 2015 targets. The need for change to make them more attainable is stronger than ever.

    Lockdown home schooling in Mendoza province, Argentina. These children’s teachers drive 400 kilometres every month to deliver books and food to their students.Credit: Andres Larrovere/AFP/Getty

    The United Nations has confirmed an unwelcome suspicion: the coronavirus pandemic has put the Sustainable Development Goals (SDGs) out of reach. Most of the goals to end poverty, protect the environment and support well-being by 2030 were already off course. Now, what little progress had been made has been stopped in its tracks.
    This week, as government representatives join a virtual UN meeting to decide how best to achieve the goals, it cannot be business as usual for the 2030 agenda. Researchers both outside and inside the UN are questioning whether the goals are fit for the post-pandemic age. The goals’ ambition is as important as ever, but fresh thinking is needed on the best ways to achieve them.
    Of the 17 SDGs, just 2 — eliminating preventable deaths among newborns and under-fives, and getting children into primary schools — were close to being achieved pre-pandemic. But COVID-19 has turned back the clock. The UN’s 2020 report on the SDGs reveals that childhood vaccination programmes have stalled in 70 countries, and that school closures have kept 90% of the world’s students — some 1.57 billion children — out of school.
    The rise in domestic abuse brought about by lockdown measures has put paid to progress in the goal for gender equality and women’s empowerment. Many women have been unable to access sexual- and reproductive-health services, which could result in as many as 2.7 million extra unsafe abortions being carried out, according to Clare Wenham, a health-policy researcher at the London School of Economics, and her colleagues (C. Wenham et al. Nature 583, 194–198; 2020).

    At the same time, at least 270 million people face hunger, and the World Food Programme is preparing its biggest humanitarian response in history. More than 70 million people will be forced into extreme poverty this year — potentially wiping out recent gains. That’s in addition to the more than 750 million who were already living on less than US$1.90 a day.
    All in all, the goals to eliminate poverty, hunger and inequality, and to promote health, well-being and economic growth are headed for extinction. In many instances, countries will be unable to even record what is happening: according to a survey of 122 national statistics offices by the UN and the World Bank, 96% of such offices have fully or partially stopped face-to-face data collection.
    What, then, needs to be done? Even before the pandemic, ideas were being floated to find ways to make the goals more achievable. Under one proposal from a group of UN science advisers, the 17 SDGs and 169 associated targets would be redistributed into 6 “entry points”. These would be human well-being (which would include eliminating poverty and improving health and education); sustainable economies; access to food and nutrition; access to, and decarbonization of, energy; urban development; and the global environmental commons (combining biodiversity and climate change).
    A related proposal, but from a different group of advisers, the Sustainable Development Solutions Network (SDSN), also redistributes the 17 goals into 6, which it calls “transformations”. These are: education, gender and inequality; health, well-being and demography; energy decarbonization and sustainable industry; sustainable food, land, water and oceans; sustainable cities and communities; and digital revolution for sustainable development.

    In both cases, however, countries would still be required to meet the actual SDGs — and their targets. Guido Schmidt-Traub, the SDSN’s executive director, told Nature the SDGs should still guide post-COVID-19 recovery. “There is nothing else to replace the SDGs right now.”
    But such a measure is no longer realistic, according to Robin Naidoo, a lead scientist at the conservation group WWF-US in Washington DC, and Brendan Fisher, an environmental scientist at the University of Vermont in Burlington. Last week, they described how COVID-19 has irreparably altered at least some of the SDGs’ underpinning assumptions (R. Naidoo and B. Fisher Nature 583, 198–201; 2020).
    When the goals were set, in 2015, the picture was one of rising economic growth and positive international cooperation — which led to the Paris climate agreement — both essential to meeting many of the SDGs’ targets. Now that the world is reeling from coronavirus and is on the brink of a once-in-a-century depression, governments are cooperating much less; crucial international meetings on protecting the climate, biodiversity and wetlands have been postponed; and aid to help the poorest countries meet their goals is set to fall.
    Separate goals from growth
    A more radical overhaul of the SDGs is also being advocated from inside the UN. In an excoriating report, Philip Alston, until recently the organization’s special rapporteur on extreme poverty and human rights, urged the SDGs’ supporters to acknowledge that things have changed. “The official response to date has been that ‘the 2030 Agenda must be preserved, and the SDGs must be reached’,” he wrote. “But doubling down on an inadequate and increasingly out-of-date approach is especially problematic.” He’s right.
    One priority — as Alston, Naidoo and Fisher, among many others, advocate — is to decouple the SDGs from economic-growth targets. It is not just that growth is unachievable — at least for the foreseeable future — but that there is evidence to show that its benefits have not been equitably shared, and that it assigns value to undesirable things — what Naidoo and Fisher call “dangerous jobs, traffic jams and pollution”. Because of the way growth is measured, an increase in any of these three translates to positive growth figures. This creates perverse incentives for policymakers to put cars on the roads or invest further in fossil fuels.
    Yet without growth, where will funding be found to achieve the many transformations needed? Naidoo and Fisher respond by pointing to one eye-watering figure: in 2015, government subsidies to the fossil-fuel industry came to $4.7 trillion, a figure that probably now exceeds $5 trillion. Each year, citizens are paying the equivalent of the gross domestic product of Japan to prop up an industry that is among the principal causes of climate change and unsustainable development. This money should be spent on achieving the goals, not undermining them.
    Recalibrating the SDGs — especially in the current climate — won’t be easy. But the evidence that there is a need for a changed approach is accumulating. If the pandemic has shown us anything, it’s that countries can drastically change the way they think and act. The pandemic is radically altering economic and social realities. It shows that radical action can be taken to tackle poverty and inequality, health, education, biodiversity and climate.
    When country representatives and the UN’s science-advice teams wrap up their meeting this week, they must heed their own poverty adviser and “avoid sleepwalking towards assured failure, while pumping out endless bland reports”.

    Nature 583, 331-332 (2020)
    doi: 10.1038/d41586-020-02002-3

    Latest on:

    Biodiversity

    Climate change

    An essential round-up of science news, opinion and analysis, delivered to your inbox every weekday.

    Related Articles More

  • in

    Analysis of compositions of microbiomes with bias correction

    Notation
    The notations described in ANCOM-BC methodology are summarized in Table 1.
    Table 1 Summary of notations.
    Full size table

    Data preprocessing
    We adopted the methodology of ANCOM-II22 as the preprocessing step to deal with different types of zeros before performing DA analysis.
    There are instances where some taxa are systematically absent in an ecosystem. For example, there may be taxa present in a soil sample from a desert that might absent in a soil sample from a rain forest. In such cases, the observed zeros are called structural zeros. Let pij denote proportion non-zero samples of the ith taxon in the jth group, and let ({hat{p}}_{ij}=frac{1}{{n}_{j}}mathop{sum }nolimits_{k = 1}^{{n}_{j}}I({O}_{ijk}ne 0)) denote the estimate of pij. In practice, we declare the ith taxon to have structural zeros in the jth group if either of the following is true:
    (a)
    ({hat{p}}_{ij}=0.)

    (b)
    ({hat{p}}_{ij}-1.96scriptstyle{sqrt{frac{{hat{p}}_{ij}(1-{hat{p}}_{ij})}{{n}_{j}}}}le 0).

    If a taxon is considered to be a structural zero in an experimental group then, for that specific ecosystem, the taxon is not used in further analysis. Thus, suppose there are three ecosystems A, B, and C and suppose taxon X is a structural zero in ecosystems A and B but not in C, then taxon X is declared to be differentially abundant in C relative to A and B and not analyzed further. If taxon Y is a structurally zero in ecosystem A but not in B and C, in that case we declare that taxon Y is differentially abundant in B relative to A as well as differentially abundant in C relative to A. We then compare the absolute abundance of taxon Y between B and C using the methodology described in this section. Taxa identified to be structural zeros among all experimental groups are ignored from the following analyses.
    In a similar fashion, we address the outlier zeros as well as sampling zeros using the methodology developed in ANCOM-II22.
    Model assumptions
    Assumption 0.1.

    $$E({O}_{ijk}| {A}_{ijk})={c}_{jk}{A}_{ijk}\ Var({O}_{ijk}| {A}_{ijk})={sigma }_{w,ijk}^{2},$$
    (1)

    where ({sigma }_{w,ijk}^{2}) = variability between specimens within the kth sample from the jth group. Therefore, ({sigma }_{w,ijk}^{2}) characterizes the within-sample variability. Typically, researchers do not obtain more than one specimen at a given time in most microbiome studies. Consequently, variability between specimens within sample is usually not estimated.
    According to Assumption 0.1, in expectation the absolute abundance of a taxon in a random sample is in constant proportion to the absolute abundance in the ecosystem of the sample. In other words, the expected relative abundance of each taxon in a random sample is equal to the relative abundance of the taxon in the ecosystem of the sample.
    Assumption 0.2. For each taxon i, Aijk, j = 1, …, g, k = 1, …, nj, are independently distributed with

    $$E({A}_{ijk}| {theta }_{ij}) ={theta }_{ij}\ Var({A}_{ijk}| {theta }_{ij}) ={sigma }_{b,ij}^{2},$$
    (2)

    where ({sigma }_{b,ij}^{2}) = between-sample variation within group j for the ith taxon.
    The Assumption 0.2 states that for a given taxon, all subjects within and between groups are independent, where θij is a fixed parameter rather than a random variable.
    Regression framework
    From Assumptions 0.1 and 0.2, we have:

    $$E({O}_{ijk}) ={c}_{jk}{theta }_{ij}\ Var({O}_{ijk}) =f({sigma }_{w,ijk}^{2},{sigma }_{b,ij}^{2}):= {sigma }_{t,ijk}^{2}.$$
    (3)

    Motivated by the above set-up, we introduce the following linear model framework for log-transformed OTU counts data:

    $${y}_{ijk}={d}_{jk}+{mu }_{ij}+{epsilon }_{ijk},$$
    (4)

    with

    $$E({epsilon }_{ijk}) =0,\ E({y}_{ijk}) ={d}_{jk}+{mu }_{ij},\ Var({y}_{ijk}) =Var({epsilon }_{ijk}):= {sigma }_{ijk}^{2}.$$
    (5)

    Note that with a slight abuse of notation for simplicity of exposition, the above log-transformation of data is inspired by the Box–Cox family of transformations23 which are routinely used in data analysis. Note that d in the above equation is not exactly log(c) due to Jensenʼs inequality, it simply reflects the effect of c
    An important distinction from standard ANOVA: Before we describe the details of the proposed methodology, we like to draw attention to a fundamental difference between the current formulation of the problem and the standard one-way ANOVA model. For simplicity, let us suppose we have two groups, say a treatment and a control group. Let us also suppose that there is only one taxon in our microbiome study and n subjects are assigned to the treatment group and n are assigned to the control group. Suppose the researcher is interested in comparing the mean absolute abundance of the taxon in the ecosystems of the two groups. Then under the above assumptions, the model describing the study is given by:

    $${y}_{jk}={d}_{jk}+{mu }_{j}+{epsilon }_{jk},j=1,2,k=1,2,ldots ,n.$$

    Then trivially the sample mean absolute abundance of jth group is given by ({bar{y}}_{j.}=frac{1}{n}mathop{sum }nolimits_{k = 1}^{n}{y}_{jk}) and (E({bar{y}}_{j.})=frac{1}{n}mathop{sum }nolimits_{k = 1}^{n}{d}_{jk}+{mu }_{j}={bar{d}}_{j.}+{mu }_{j}). The difference in the sample means between the two groups is ({bar{y}}_{1.}-{bar{y}}_{2.}) and its expectation is (E({bar{y}}_{1.}-{bar{y}}_{2.})=({bar{d}}_{1.}-{bar{d}}_{2.})+({mu }_{1}-{mu }_{2})). Under the null hypothesis μ1 = μ2, (E({bar{y}}_{1.}-{bar{y}}_{2.})={bar{d}}_{1.}-{bar{d}}_{2.}ne ,0), unless ({bar{d}}_{1.}={bar{d}}_{2.}). Thus because of the differential sampling fractions, which are sample specific, the numerator of the standard t-test under the null hypothesis for these microbiome data is non-zero. This introduces bias and hence inflates the Type I error. On the other hand, the standard one-way ANOVA model for two groups, which is not applicable for the microbiome data described in this paper, is of the form:

    $${y}_{jk}=d+{mu }_{j}+{epsilon }_{jk},j=1,2,k=1,2,ldots ,n.$$

    Hence under the null hypothesis μ1 = μ2, (E({bar{y}}_{1.}-{bar{y}}_{2.})=0). Thus, in this case the standard t-test is appropriate. Hence in this paper we develop methodology to eliminate the bias introduced by the differential sampling fraction by each sample. To do so, we exploit the fact that we have a large number of taxa on each subject and we borrow information across taxa to estimate this bias, which is the essence of the following methodology.
    Bias and variance of bias estimation under the null hypothesis: From the above model (equation (4)), for each j, note that (E({bar{y}}_{ijcdot })={bar{d}}_{jcdot }+{mu }_{ij}) and (E({bar{y}}_{cdot jk})={d}_{jk}+{bar{mu }}_{cdot j}), where (bar{w}) represents the arithmetic mean over the suitable index. Using the least squares framework, we therefore estimate μij and djk as follows:

    $${hat{d}}_{jk} ={overline{y}}_{cdot jk}-{overline{y}}_{cdot jcdot },,k=1,,ldots ,,{n}_{j},j=1,2,ldots g,\ {hat{mu }}_{ij} ={overline{y}}_{ijcdot }-{overline{hat{d}}}_{jcdot }={overline{y}}_{ijcdot },,i=1,,ldots ,,m.$$
    (6)

    Note that (E({hat{mu }}_{ij})=E({overline{y}}_{ijcdot })={mu }_{ij}+{overline{d}}_{jcdot }). Thus, for each j = 1, 2, …g, ({hat{mu }}_{ij}) is a biased estimator and (E({hat{mu }}_{i1}-{hat{mu }}_{i2})=({mu }_{i1}-{mu }_{i2})+{overline{d}}_{1cdot }-{overline{d}}_{2cdot }). Denote (delta ={overline{d}}_{1cdot }-{overline{d}}_{2cdot }.) To begin with, in the following we shall assume there are two experimental groups with balanced design, i.e., g = 2 and n1 = n2 = n. Later the methodology is easily extended to unbalanced design and multigroup settings. Suppose we have two ecosystems and for each taxon i, i = 1, 2, …m, we wish to test the hypothesis

    $${H}_{0} :{mu }_{i1}={mu }_{i2}\ {H}_{1} :{mu }_{i1}ne {mu }_{i2}.$$
    (7)

    Under the null hypothesis, (E({hat{mu }}_{i1}-{hat{mu }}_{i2})=delta , ne , 0), and hence biased. The goal of ANCOM-BC is to estimate this bias and accordingly modify the estimator ({hat{mu }}_{i1}-{hat{mu }}_{i2}) so that the resulting estimator is asymptotically centered at zero under the null hypothesis and hence the test statistic is asymptotically centered at zero. First, we make the following observations. Since (E({overline{y}}_{ijcdot })={overline{d}}_{jcdot }+{mu }_{ij}) and ({hat{mu }}_{ij}={overline{y}}_{ijcdot }), therefore ({hat{mu }}_{ij}) is an unbiased estimator of ({overline{d}}_{jcdot }+{mu }_{ij}). From (5) and Lyapunov central limit theorem, we have:

    $$frac{{hat{mu }}_{ij}-({mu }_{ij}+{overline{d}}_{jcdot })}{{sigma }_{i}}{to }_{d}N(0,1),,,{rm{as}} nto infty ,\ {rm{where}} {sigma }_{ij}^{2}=Var({hat{mu }}_{ij})=Var({overline{y}}_{ij.})=frac{1}{{n}^{2}}mathop{sum }limits_{k=1}^{n}{sigma }_{ijk}^{2}.$$
    (8)

    Let Σjk denote an m × m covariance matrix of ({epsilon }_{jk}={({epsilon }_{1jk},{epsilon }_{2jk},ldots ,{epsilon }_{mjk})}^{T}), where ({sigma }_{ii^{prime} jk}) is the ({(i,i^{prime} )}^{th}) element of Σjk and ({sigma }_{ijk}^{2}) is the ith diagonal element of Σjk. Furthermore, suppose
    Assumption 0.3.

    $${sigma }_{ijk}^{2} νi0. Thus, without loss of generality for κ1, κ2  > 0, let νi1 = νi0 + κ1 and νi2 = νi0 + κ2. While this assumption is not a requirement for our method, it is reasonable to assume that variability among differentially abundant taxa is larger than that among the null taxa. By making this assumption, we speed-up the computation time.
    Assuming samples are independent between experimental groups, we begin by first estimating ({nu }_{i0}^{2}={rm{V}}{rm{ar}}({hat{mu }}_{i1}-{hat{mu }}_{i2})={rm{V}}{rm{ar}}({hat{mu }}_{i1})+{rm{V}}{rm{ar}}({hat{mu }}_{i2})). Using the estimator stated in (14), we estimate ({nu }_{i0}^{2}) consistently as follows:

    $${hat{nu }}_{i0}^{2}=mathop{sum }limits_{j=1}^{2}{hat{sigma }}_{ij}^{2}=mathop{sum }limits_{j=1}^{2}frac{1}{{n}^{2}}mathop{sum }limits_{k=1}^{n}{({y}_{ijk}-{hat{d}}_{jk}-{hat{mu }}_{ij})}^{2}.$$
    (20)

    In all future calculations, we plug in ({hat{nu }}_{i0}^{2}) for ({nu }_{i0}^{2}). This is similar in spirit to many statistical procedures involving nuisance parameters. The following lemma is useful in the sequel.
    Lemma 0.1.
    (frac{partial }{partial theta }{mathrm{log}},f(x)={E}_{f(z| x)}[frac{partial }{partial theta }{mathrm{log}},f(z)+frac{partial }{partial theta }{mathrm{log}},f(x| z)]).25
    Let (Theta ={(delta ,{pi }_{1},{pi }_{2},{pi }_{3},{l}_{1},{l}_{2},{kappa }_{1},{kappa }_{2})}^{T}) denote the set of unknown parameters, then for each taxon the log-likelihood can be reformulated using Lemma 0.1, as follows:

    $$Theta leftarrow arg {max }_{Theta }mathop{sum }limits_{i=1}^{m}mathop{sum }limits_{r=0}^{2}{p}_{r,i}[{mathrm{log}},{rm{P}}{rm{r}}(iin {C}_{r})+{mathrm{log}},f({Delta }_{i}| iin {C}_{r})].$$
    (21)

    Then the E–M algorithm is described as follows:

    E-step: Compute conditional probabilities of the latent variable. Define ({p}_{r,i}={rm{P}}{rm{r}}(iin {C}_{r}| {Delta }_{i})=frac{{pi }_{r}phi (frac{{Delta }_{i}, -, (delta , +, {l}_{r})}{{nu }_{ir}})}{{sum }_{r}{pi }_{r}phi (frac{{Delta }_{i}, -, (delta , + , {l}_{r})}{{nu }_{ir}})},r=0,1,2;i=1,ldots ,m), which are conditional probabilities representing the probability that an observed value follows each distribution. Note that l0 = 0.

    M-step: Maximize the likelihood function with respect to the parameters, given the conditional probabilities.

    We shall denote the resulting estimator of δ by ({hat{delta }}_{{rm{EM}}}.)
    Next we estimate ({rm{V}}{rm{ar}}({hat{delta }}_{{rm{EM}}})). Since the likelihood function is not a regular likelihood and hence it is not feasible to derive the Fisher information. Consequently, we take a simpler and a pragmatic approach to derive an approximate estimator of ({rm{V}}{rm{ar}}({hat{delta }}_{{rm{EM}}})) using ({rm{V}}{rm{ar}}({hat{delta }}_{{rm{WLS}}})), which is defined below. Extensive simulation studies suggest that ({hat{delta }}_{{rm{EM}}}) and ({hat{delta }}_{{rm{WLS}}}) are highly correlated (Supplementary Fig. 9) and it appears to be reasonable to approximate ({rm{V}}{rm{ar}}({hat{delta }}_{{rm{EM}}})) by ({rm{V}}{rm{ar}}({hat{delta }}_{{rm{WLS}}})).
    Let {Cr} = mr, r = 0, 1, 2, then

    $${hat{delta }}_{{rm{WLS}}} =frac{{sum }_{iin {C}_{0}}frac{{Delta }_{i}}{{hat{nu }}_{i0}^{2}}+{sum }_{iin {C}_{1}}frac{{Delta }_{i}-{hat{l}}_{1}}{{hat{nu }}_{i1}^{2}}+{sum }_{iin {C}_{2}}frac{{Delta }_{i}-{hat{l}}_{2}}{{hat{nu }}_{i2}^{2}}}{{sum }_{iin {C}_{0}}frac{1}{{hat{nu }}_{i0}^{2}}+{sum }_{iin {C}_{1}}frac{1}{{hat{nu }}_{i1}^{2}}+{sum }_{iin {C}_{2}}frac{1}{{hat{nu }}_{i2}^{2}}}\ =frac{{sum }_{iin {C}_{0}}frac{{Delta }_{i}}{{nu }_{i0}^{2}}+{sum }_{iin {C}_{1}}frac{{Delta }_{i}-{l}_{1}}{{nu }_{i1}^{2}}+{sum }_{iin {C}_{2}}frac{{Delta }_{i}-{l}_{2}}{{nu }_{i2}^{2}}}{{sum }_{iin {C}_{0}}frac{1}{{nu }_{i0}^{2}}+{sum }_{iin {C}_{1}}frac{1}{{nu }_{i1}^{2}}+{sum }_{iin {C}_{2}}frac{1}{{nu }_{i2}^{2}}}+{o}_{p}(1).$$
    (22)

    The above expression is of the form

    $$frac{{a}_{1}^{T}{x}_{1}+{a}_{2}^{T}{x}_{2}+{a}_{3}^{T}{x}_{3}}{{a}_{1}^{T}{bf{1}}+{a}_{2}^{T}{bf{1}}+{a}_{3}^{T}{bf{1}}}equiv frac{{alpha }^{T}u}{{alpha }^{T}{bf{1}}},$$
    (23)

    where
    (1)
    1 = (1, …, 1)T,

    (2)
    ({a}_{r}={({a}_{r1},{a}_{r2},ldots ,{a}_{r{m}_{r}})}^{T}:= {(frac{1}{{nu }_{ir}^{2}})}^{T},,iin {C}_{r},,r=0,1,2),

    (3)
    ({x}_{r}={({x}_{r1},{x}_{r2},ldots ,{x}_{r{m}_{r}})}^{T}:= {({Delta }_{i}-{l}_{i})}^{T},,iin {C}_{r},,r=0,1,2). Note that l0 = 0,

    (4)
    (alpha ={({alpha }_{1},{alpha }_{2},ldots ,{alpha }_{m})}^{T}equiv {({a}_{1}^{T},{a}_{2}^{T},{a}_{3}^{T})}^{T}),

    (5)
    (u={({u}_{1},{u}_{2},ldots ,{u}_{m})}^{T}equiv {({x}_{1}^{T},{x}_{2}^{T},{x}_{3}^{T})}^{T}).

    For the simplicity of notation, we relabel a and x by α and u, respectively. Denote Cov(x) = Cov(u) by Ω, and let ({omega }_{ii^{prime} }) denotes the ((i,i^{prime} )) element of Ω. As in Assumption 0.3, we make the following assumption
    Assumption 0.4.

    $$frac{mathop{sum }nolimits_{ine i^{prime} }^{m}{omega }_{ii^{prime} }}{{m}^{2}}=o(1).$$
    (24)

    Using the above expressions, we compute the variance as follows:

    $${rm{V}}{rm{ar}}({hat{delta }}_{{rm{WLS}}})={rm{V}}{rm{ar}}(frac{{alpha }^{T}u}{{alpha }^{T}{bf{1}}})=frac{mathop{sum }nolimits_{i = 1}^{m}{alpha }_{i}^{2}{omega }_{ii}}{{(mathop{sum }nolimits_{i = 1}^{m}{alpha }_{i})}^{2}}+frac{mathop{sum }nolimits_{ine i^{prime} }^{m}{alpha }_{i}{alpha }_{i^{prime} }{omega }_{ii^{prime} }}{{(mathop{sum }nolimits_{i = 1}^{m}{alpha }_{i})}^{2}}.$$
    (25)

    Recall that (a) for i ∈ C0, ({omega }_{ii}={rm{V}}{rm{ar}}({Delta }_{i})={nu }_{i0}^{2}=O({n}^{-1})), (b) for i ∈ C1, ({omega }_{ii}={rm{V}}{rm{ar}}({Delta }_{i})={nu }_{i1}^{2}={nu }_{i0}^{2}+{kappa }_{1}=O(1)), and (c) for i ∈ C2, ({omega }_{ii}={rm{V}}{rm{ar}}({Delta }_{i})={nu }_{i2}^{2}={nu }_{i0}^{2}+{kappa }_{2}=O(1)). Note that ({alpha }_{i}=frac{1}{{rm{V}}{rm{ar}}({Delta }_{i})}=frac{1}{{omega }_{ii}}), thus we have:

    $${rm{V}}{rm{ar}}(frac{{alpha }^{T}u}{{alpha }^{T}{bf{1}}})=frac{mathop{sum }nolimits_{i = 1}^{m}{alpha }_{i}^{2}{omega }_{ii}}{{(mathop{sum }nolimits_{i = 1}^{m}{alpha }_{i})}^{2}}+frac{mathop{sum }nolimits_{ine i^{prime} }^{m}{alpha }_{i}{alpha }_{i^{prime} }{omega }_{ii^{prime} }}{{(mathop{sum }nolimits_{i = 1}^{m}{alpha }_{i})}^{2}}=frac{1}{mathop{sum }nolimits_{i = 1}^{m}{alpha }_{i}}+frac{mathop{sum }nolimits_{ine i^{prime} }^{m}{alpha }_{i}{alpha }_{i^{prime} }{omega }_{ii^{prime} }}{{(mathop{sum }nolimits_{i = 1}^{m}{alpha }_{i})}^{2}}.$$
    (26)

    Since ({nu }_{i0}^{2}=O({n}^{-1})), ({nu }_{i1}^{2}=O(1)), and ({nu }_{i2}^{2}=O(1)), consequently, a1i = O(n), a2i = a3i = O(1), and

    $$mathop{sum }limits_{i=1}^{m}{alpha }_{i} ={{bf{1}}}^{T}{a}_{1}+{{bf{1}}}^{T}{a}_{2}+{{bf{1}}}^{T}{a}_{3} = sum _{iin {C}_{0}}O(n)+sum _{iin {C}_{1}}O(1)+sum _{iin {C}_{2}}O(1)\ = O({m}_{0}n)+O({m}_{1})+O({m}_{2})\ =O({m}_{0}n),,,{rm{if}}{m}_{0}nge max {{m}_{1},{m}_{2}}.$$
    (27)

    Using these facts and Assumption 0.4 in (26), we get

    $${rm{V}}{rm{ar}}(frac{{alpha }^{T}u}{{alpha }^{T}{bf{1}}}) = O({m}_{0}^{-1}{n}^{-1})+frac{mathop{sum }nolimits_{ine i^{prime} }^{m}{{n}^{-1}{m}^{-1}{alpha }_{i}}{{n}^{-1}{m}^{-1}{alpha }_{i^{prime} }}{omega }_{ii^{prime} }}{{n}^{-2}{m}^{-2}{(mathop{sum }nolimits_{i = 1}^{m}{alpha }_{i})}^{2}}\ = O({m}_{0}^{-1}{n}^{-1})+frac{1}{{m}^{2}}frac{mathop{sum }nolimits_{ine i^{prime} }^{m}{{n}^{-1}{alpha }_{i}}{{n}^{-1}{alpha }_{i^{prime} }}{omega }_{ii^{prime} }}{{(mathop{sum }nolimits_{i = 1}^{m}{n}^{-1}{m}^{-1}{alpha }_{i})}^{2}}\ = O({m}_{0}^{-1}{n}^{-1})+frac{1}{{m}^{2}}frac{O(1)o({m}^{2})}{O(1)}\ = O({m}_{0}^{-1}{n}^{-1}).$$
    (28)

    Thus, under Assumption 0.4 regarding ({omega }_{ii^{prime} }), the contribution of the covariance terms in the above variance expression is negligible as long as m is very large compared with n, which is usually the case. Hence

    $${rm{V}}{rm{ar}}({hat{delta }}_{{rm{WLS}}})={rm{V}}{rm{ar}}(frac{{alpha }^{T}u}{{alpha }^{T}{bf{1}}})=O({m}_{0}^{-1}{n}^{-1}).$$
    (29)

    Furthermore, appealing to Cauchy–Schwartz inequality we get

    $${rm{Cov}}({hat{mu }}_{i1}-{hat{mu }}_{i2},{hat{delta }}_{{rm{WLS}}}) le sqrt{{rm{V}}{rm{ar}}({hat{mu }}_{i1}-{hat{mu }}_{i2}){rm{V}}{rm{ar}}({hat{delta }}_{{rm{WLS}}})}\ le O({n}^{-1/2})O({m}_{0}^{-1/2}{n}^{-1/2})=O({n}^{-1}{m}_{0}^{-1/2}).$$
    (30)

    Hence, as long as m0 is large, the contribution made by ({rm{V}}{rm{ar}}({hat{delta }}_{{rm{WLS}}})) and ({rm{Cov}}({hat{mu }}_{i1}-{hat{mu }}_{i2},{hat{delta }}_{{rm{WLS}}})) relative to ({rm{V}}{rm{ar}}({hat{mu }}_{i1}-{hat{mu }}_{i2})) is negligible.
    Neglect the covariance term in (26), let ({hat{C}}_{r}) denote the estimator of Cr, r = 0, 1, 2 from the E–M algorithm, define

    $$widehat{{rm{V}}{rm{ar}}}({hat{delta }}_{{rm{WLS}}})=frac{1}{{sum }_{iin {hat{C}}_{0}}frac{1}{{hat{nu }}_{i0}^{2}}+{sum }_{iin {hat{C}}_{1}}frac{1}{{hat{nu }}_{i1}^{2}}+{sum }_{iin {hat{C}}_{2}}frac{1}{{hat{nu }}_{i2}^{2}}},$$
    (31)

    an estimator of ({rm{V}}{rm{ar}}({hat{delta }}_{{rm{WLS}}})) under the Assumption 0.4. Then

    $$widehat{{rm{V}}{rm{ar}}}({hat{delta }}_{{rm{WLS}}}){to }_{p}frac{1}{mathop{sum }nolimits_{i = 1}^{m}{alpha }_{i}}=frac{1}{{sum }_{iin {C}_{0}}frac{1}{{nu }_{i0}^{2}}+{sum }_{iin {C}_{1}}frac{1}{{nu }_{i1}^{2}}+{sum }_{iin {C}_{2}}frac{1}{{nu }_{i2}^{2}}},{rm{as}},, m,nto infty .$$
    (32)

    We performed extensive simulations to evaluate the bias and variance of ({hat{delta }}_{{rm{EM}}}) and that of ({hat{delta }}_{{rm{WLS}}}). The scatter plot (Supplementary Fig. 9) of ({hat{delta }}_{{rm{EM}}}) and ({hat{delta }}_{{rm{WLS}}}) are almost perfectly linear with correlation coefficient nearly 1 in all cases. This suggests that ({hat{delta }}_{{rm{WLS}}}) is a very good approximation for ({hat{delta }}_{{rm{EM}}}). The variance of ({hat{delta }}_{{rm{EM}}}) as well as that of ({hat{delta }}_{{rm{WLS}}}) are roughly of the order ({n}^{-1}{m}_{0}^{-1}), as we expected. In addition, they are approximately unbiased (Supplementary Table 6).
    Hypothesis testing for two-group comparison
    For taxon i, we test the following hypothesis

    $${H}_{0} :{mu }_{i1}={mu }_{i2}\ {H}_{1} :{mu }_{i1},,ne ,,{mu }_{i2}$$

    using the following test statistic which is approximately centered at zero under the null hypothesis:

    $${W}_{i}=frac{{hat{mu }}_{i1}-{hat{mu }}_{i2}-{hat{delta }}_{{rm{EM}}}}{sqrt{{hat{sigma }}_{i1}^{2}+{hat{sigma }}_{i2}^{2}}}.$$
    (33)

    From Slutsky’s theorem, we have:

    $${W}_{i}{to }_{d}N(0,1),{rm{as}},, m,,n,to infty .$$
    (34)

    If the sample size is not very large and/or the number of non-null taxa are very large, then we modify the above test statistic as follows:

    $${W}_{i}^{* }=frac{{hat{mu }}_{i1}-{hat{mu }}_{i2}-{hat{delta }}_{{rm{WLS}}}}{sqrt{{hat{sigma }}_{i1}^{2}+{hat{sigma }}_{i2}^{2}+widehat{{rm{V}}{rm{ar}}}({hat{delta }}_{{rm{WLS}}})+2sqrt{({hat{sigma }}_{i1}^{2}+{hat{sigma }}_{i2}^{2})widehat{{rm{V}}{rm{ar}}}({hat{delta }}_{{rm{WLS}}})}}}.$$
    (35)

    To control the FDR due to multiple comparisons, we recommend applying the Holm–Bonferroni method26 or Bonferroni27,28 correction rather than the Benjamini–Hochberg (BH) procedure29 to adjust the raw p values as research has showed that it is more appropriate to control the FDR when p values were not accurate30, and the BH procedure controls the FDR provided you have either independence or some special correlation structures such as perhaps positive regression dependence among taxa29,31. In our simulation studies, since the absolute abundances for each taxon are generated independently, we compared the ANCOM-BC results adjusted either by Bonferroni correction (Fig. 4) or BH procedure (Supplementary Fig. 10), it is clearly that the FDR control by Bonferroni correction is more conservative while implementing BH procedure results in FDR around the nominal level (5%). Obviously, ANCOM-BC has larger power when using BH procedure.
    Hypothesis testing for multigroup comparison
    In some applications, for a given taxon, researchers are interested in drawing inferences regarding DA in more than two ecosystems. For example, for a given taxon, researchers may want to test whether there exists at least one experimental group that is significantly different from others, i.e., to test

    $${H}_{0,i} :{cap }_{jne j^{prime} in {1,ldots ,g}}{mu }_{ij}={mu }_{ij^{prime} }\ {H}_{1,i} :{cup }_{jne j^{prime} in {1,ldots ,g}}{mu }_{ij},, ne ,, {mu }_{ij^{prime} }.$$

    Similar to the two-group comparison, after getting the initial estimates of ({hat{mu }}_{ij}) and ({hat{d}}_{jk}), setting the reference group r (e.g., r = 1), and obtaining the estimator of the bias term ({hat{delta }}_{rj}) through E–M algorithm, the final estimator of mean absolute abundance of the ecosystem (in log scale) are obtained by transforming ({hat{mu }}_{ij}) of (6) into:

    $${hat{mu }}_{ij}^{* }:= left{begin{array}{l}{}hskip -42pt {hat{mu }}_{ir},,,, qquad j=r\ {hat{mu }}_{ij}+{hat{delta }}_{rj},,,,j ,, ne ,, rin 1,ldots ,gend{array}right..$$
    (36)

    Thus, based on (18) and the E–M estimator of δrj, as (m,min ({n}_{j},{n}_{j^{prime} })to infty)

    $${{hat{mu }}_{ij}^{* }-{hat{mu }}_{ij^{prime} }^{* }to }_{p}left{begin{array}{ll}hskip -30pt 0&{rm{if}} {rm{taxon}} i {rm{is}} {rm{not}} {rm{differentially}} {rm{abundant}} {rm{between}} {rm{group}} j {rm{and}} j^{prime} ,\ {mu }_{ij}-{mu }_{ij^{prime} }&hskip -219pt {rm{otherwise}}.end{array}right.$$
    (37)

    Similarly, the estimator of the sampling fraction is obtained by transforming ({hat{d}}_{jk}) of (6) into

    $${hat{d}}_{jk}^{* }:= left{begin{array}{l}hskip -45pt {hat{d}}_{rk},,,,, qquad j=r\ {hat{d}}_{jk}-{hat{delta }}_{rj},,,,j ,, ne ,, rin 1,ldots ,gend{array}right..$$
    (38)

    As by (13) and the E–M estimator of δrj

    $${hat{d}}_{jk}^{* }{to }_{p}{d}_{jk}-{overline{d}}_{rcdot }{rm{as}} m,,min ({n}_{j},{n}_{j^{prime} })to infty,$$
    (39)

    which indicates that we are only able to estimate sampling fractions up to an additive constant (({overline{d}}_{rcdot })).
    Define the test statistic for pairwise comparison as:

    $${W}_{i,jj^{prime} }=frac{{hat{mu }}_{ij}^{* }-{hat{mu }}_{ij^{prime} }^{* }}{sqrt{{hat{sigma }}_{ij}^{2}+{hat{sigma }}_{ij^{prime} }^{2}}},,,,i=1,,ldots ,,m,j ,, ne ,, j^{prime} in {1,,ldots ,,g}.$$
    (40)

    For computational simplicity, inspired by the William’s type of test32,33,34,35, we reformulate the global test with the following test statistic:

    $${W}_{i}=mathop{max }limits_{jne j^{prime} in {1,ldots ,g}}| {W}_{i,jj^{prime} }| ,,,,i=1,,ldots ,,m.$$
    (41)

    Under null, ({W}_{i,jj^{prime} }{to }_{d}N(0,1)), thus we can construct the null distribution of Wi by simulations, i.e., for each specific taxon i,
    (a)
    Generate ({W}_{i,jj^{prime} }^{(b)} sim N(0,1),j, ne , j^{prime} in {1,,ldots ,,g},b=1,ldots ,B.)

    (b)
    Compute ({W}_{i}^{(b)}=mathop{max }limits_{jne j^{prime} in {1,ldots ,g}}{W}_{i,jj^{prime} }^{(b)}.)

    (c)
    Repeat above steps B times (e.g., B = 1000), we then get the null distribution of Wi by ({({W}_{i}^{(1)},ldots ,{W}_{i}^{(B)})}^{T}.)

    Finally, p value is calculated as

    $${p}_{i}=frac{1}{B}mathop{sum }limits_{b=1}^{B}I({W}_{i}^{(b)} > {W}_{i}),,,,i=1,,ldots ,,m$$
    (42)

    and the Bonferroni correction is applied to control the FDR.
    Reporting summary
    Further information on research design is available in the Nature Research Reporting Summary linked to this article. More