More stories

  • in

    A multilevel carbon and water footprint dataset of food commodities

    With the aim of obtaining a useful tool for stakeholders to explore, assess and use the information related to CF and WF of food commodities, we implemented a multi-step methodological framework to create an easy to use CF and WF repository of food items, which can be expanded or modified for tailored requirements using a science based approach for each step of its creation (Fig. 1).The overall methodological procedure is made of 3 steps. Step 1 is related to CF and WF data collection from literature, eligibility check and harmonization, to create the base level of the database (level 1). Step 2 is about the creation of other three informative layers with higher level of data aggregation. These might be the data of direct interests for stakeholders of the food systems. A rigorous statistical approach is proposed to evaluate the quality of analysed data and criteria for the correct use of data, based on statistical evidence, are set and applied to the data. In Step 3 the complex set of statistical evaluations, done for each informative level, is summarized into an easy to use dataset reporting values of CF and WF of food items. Thanks to its multilevel approach, the database provides a flexible tool for different purposes and levels of expertise. Each step is based on transparent procedures that allow users to replicate, to implement and to modify each level of the database.The three steps are described in details in the following paragraphs.Step 1 – CF and WF data collection, harmonization and compilation of level 1 of SEL databaseThe first step was to review the published data of CF and WF of food commodities. We revised literature data published till January 2020 including peer-reviewed papers, conference proceedings, public reports or studies where methods of data collection and handling were described, and Environmental Product Declarations (EPDs).For the collection of CF data, a significant input came from the systematic review of Clune et al.11, who reviewed 369 published studies, covering the period 2000–2015, proving 168 varieties of fresh food products based on 1718 data entries. An additional source of studies reporting both CF and WF was the Double Pyramid database 2016 built on the previous version 201414 (BCFN2016 https://www.barillacfn.com/en/publications/double-pyramid-2016/), which reports 1202 CF values from 468 sources covering 240 food items and 309 WF values from 136 data sources covering 152 food items (reference period 1998–2016). Part of CF data of this latter dataset, up to year 2014, were already revised and included in the Clune et al.11 study. To avoid double counting from these two sources, data from both sources were checked for authorship, plus the CF reported data were compared and if in disagreement the original data were checked in the paper. Data reported in the Double Pyramid database 2016 but not present in Clune et al.11, mostly referring to processed food, were checked for eligibility applying the exclusion criteria reported in Table 2 and if considered eligible they were included in the present database.Table 2 Exclusion criteria to be applied to CF and WF data collected from literature to create SEL database level 1.Full size tableA new literature search was done to integrate data not covered by the previous reviews using three online bibliographic sources SCOPUS (https://www.scopus.com/home.uri), Google Scholar (https://scholar.google.com/) and the Google search engine (https://www.google.com/), which was concluded in January 2020. To search the bibliographic sources, we used the combinations of two sets of words. The first set referred to “impacts” and included the following words: carbon footprint, water footprint, virtual water, greenhouse gases, environmental impact, life cycle, LCA, LCI, EPD. The second set referred to “products” and included words like food, beverages, fish, shellfish, crops, vegetables, fruit, meat, eggs, dairy. EPDs were updated based on data reported on the International EPD’s System database (www.environdec.com). Added studies were evaluated for exclusion criteria (Table 2).The final list of data from single studies reported in the SEL database was distributed as follow: 3349 CF data, including 1397 data of fresh food commodities already reported in Clune et al.11, 803 CF data originally reported in Double Pyramid 2016 database, which were checked for eligibility and harmonized, and 701 CF data added with this study; 938 WF data, including 288 WF data originally reported in double pyramid 2016 and 650 WF data added with this study.All the CF and WF values extracted from the collected studies were assigned a group, a typology, a sub-typology when this applied, and an item name (Table 1) and were recorded on an excel sheet including the following additional information: type of bibliographic source, full reference, publication year, system boundary at distribution, country of production, region of production, relevant notes, presence of the same value in other data collections (i.e. Clune et al.11 or Double Pyramid 2016).After data collection, CF data where further analysed and handled for the harmonization of the system boundary following the approach as reported in Clune et al.11. The system boundary considered in the SEL database is the distribution centre to consumers located in the country of origin. It hence excludes post market phase like for example cooking. The system boundaries at distribution have a wide range of specifications in the published papers. We accepted regional distribution centre (RDC), international distribution centre (IDC), European distribution centre (EDC), country ports of final destination, warehouses, wholesalers, city markets, up to retailers. For the specific case of international transport, which includes also the emissions for shipping to regional distribution centres of the hosting country, rather than excluding the studies we have created a dedicated typology “imported”, which however includes very few studies. The imported commodity is indicated in the SEL database by a capital letter “I”.If CF values collected from literature referred to the system boundary “farm gate” or “slaughterhouse”, additional post farm gate GHG emissions were added as proposed by Clune et al.11. These additional emissions also included packaging if not reported in the publication. We adopted the median value for distribution to RDC (0,09 kg CO2/kg or kg CO2/L) and packaging (0,05 kg CO2/kg or kg CO2/L) used by Clune et al.11. Data referring to slaughterhouse emissions were also taken from the same publication.To address the share of WF for packaging and transportation to the market we analysed 256 EPD’s. No significant increase of WF in downstream stages associated to packaging and distribution was found. Thus we included in the analysis all system boundaries with the exception of ‘cooking’, human excretion and waste disposal.To transform CF values from carcass or live weight to bone free meat, ratios reported in in Clune et al.11 were used, while the ratio carcass weight to bone free meat for buffalo meat (1:0.684) was estimated from the studies of Gerber et al.15, Gurunathan et al.16, Li et al.17.The final version of CF and WF data, after data handling was recorded in a sheet where, in addition to the information mentioned above for each study, we also reported additional post farm gate emissions (transport T, slaughtering S, packaging P) or meat conversion factors (cf) when applying. This complete dataset represents the level 1 information sheet of the SEL database (Fig. 1).A change in 100-year global warming potential (GWP) factors provided by the International Panel on Climate Change reports AR3 (2001), AR4 (2007) and AR5 (2013) might have introduced additional variability in the studies of LCA on which CF data of level 1 are based. The extent of such variability is difficult to quantify as it depends on the relative weight of each GHG on the total CF of the item. However, the analysis of some item groups (tomato, rice, beef meat, chicken meat), used as sample test, did not show any clear trend of CF average reduction or increase over the years (1998–2020), suggesting that differences among production processes and conditions were the dominant source of CF variability.Step 2 – Creation of derived CF and WF datasets with higher aggregation level (2, 3 and 4)This step provides footprints of food commodities with a higher level of aggregation corresponding to food items, typologies and sub-typologies (Table 1), which might be of particular interest for different kinds of stakeholders. The item represents the higher detail of aggregated footprint data of a food commodity and it is often the most desirable information for food impact analysis and dietary assessments. We propose here a methodological framework to evaluate the uncertainty associated to data used to represent food items. The methodological framework will support the users in their choice of the optimal value to represent the food item on the basis of the available data present in the database. It also would easily allow for expansion and implementation of food item values.Level 2, SEL CF ITEM & SEL WF ITEM datasetsThese two datasets (CF and WF) report a comprehensive set of descriptive statistics for the list of food items present in the database. The population of data used to attribute a value and uncertainty to a food item is made of all the CF or WF values classified with that “item entry name” in the dataset of level 1 of SEL database.The item data population is described in level 2 by the following set of information.Size: number of studies used for the analysis of item population (n).Location and central-tendency measures: in terms of mean, median, first quartile (Q1) and third quartile (Q3), including also the minimum (Min) and maximum (Max) observed values.Variability measures: Standard Deviation (SD) Coefficient of Variation (CV) as absolute and relative dispersion indexes, the Interquartile Range (IQR) and the Median Absolute Deviation (MAD) as more robust indexes of variability.Shape measures: Skewness (SK), kurtosis (KU) indexes and Shapiro-Wilk normality test (SW test).The median of the item data population was chosen to assign a value of central tendency which represents the item. The median offers the advantage of not being influenced by the presence of outliers which misrepresent the value of the mean, making it a less meaningful measure. As such, the median represents the location estimator with the highest breakdown point (equal to 0.5) and with “the maximum proportion of observations that can be contaminated (i.e., set to infinity) without forcing the estimator to result in a “false” and not-representative value18,19. With these properties, the median also represents the most appropriate measure of central tendency to describe both positively and negatively skewed distributions20.To describe the uncertainty associated to the position value (median) we used descriptive statistic data relative to dispersion and shape of item data distribution. In particular, we used skewness and kurtosis indexes, which gave us information on the existence of symmetric or skewed distributions, as well as on their ‘peakedness’ measured as relative to the weights of the tails21, thus enabling us to evaluate (for each distribution) the importance of extreme values over the entire set of data and the related level of dispersion (platykurtic versus leptokurtic distributions). We completed the shape analysis by carrying out the Shapiro-Wilk test22,23 (4 ≤ n ≤ 2000).To define the uncertainty of the item value we created an assignment method based on a combination of the three quality flags (Fig. 2).Fig. 2Method for attribution of CF (or WF) value to a food item based on data quality flags. The scheme shows the procedure applied to evaluate the level of uncertainty associated to CF or WF value of a food item and how this information is used to decide the best value that should be used to represent the item. Three quality flags related to a statistical aspect of the data population are calculated to attribute the level of uncertainty. Each flag has different level of quality, red being the worst, green the best. Flags are then combined and expert judgement is used to associate a suggestion for data use to each flag combination. If the item median value is characterized by high uncertainty it poorly represents the item and caution is needed to use this data to represent the food commodity, the users is therefore redirected to a higher level of aggregation such as the sub-typology or the typology which includes the analysed item.Full size imageFlag 1, evaluation of the ‘size’ (n) of the “item data population”

    Red if n  More

  • in

    Evaluation of the performance and gas emissions of a tractor diesel engine using blended fuel diesel and biodiesel to determine the best loading stages

    Performance evaluation of tractor engineThe performance of the direct-injection turbocharger diesel engine for the Kubota M-90 tractor was evaluated at different engine loads with the use of different biodiesel blends with mineral diesel to maximize the engine efficiencies of PTO torque, BP, BMEP, and BTE, while also minimizing specific fuel consumption, gas emissions, and, finally, fossil fuel consumption. The results in Table 1 showed a significant effect of engine load percentage and fuel blend percentage and their interaction on all the studied characters.Table 1 Effects of engine load percentage and fuel blends percentage on power take-off speed, power take-off power, power take-off torque, engine speed, brake power, brake specific fuel consumption, brake thermal efficiency, fuel consumption, brake mean effective pressure, O2 percentage, CO2 percentage, CO, NO, and SO2.Full size tableEngine speedFor the effects of engine load percentage on engine speed, the results in Table 1 indicated the relationship between engine load percentage and engine speed in rpm was inversely proportional. The maximum engine speed was recorded at a loading of 0%, and the lowest speed was at a loading of 100% (Table 1). Using 100% diesel fuel (B0) gave the highest engine speed among all treatments, and the lowest speed was recorded with 100% biodiesel fuel (B100). The significant interaction between engine load, percentage, and engine speed in rpm was inversely proportional, as shown in Fig. 2a. The maximum engine speed was 2854 rpm at the loading stage of 0% using 100% diesel fuel (B0), while the minimum speed was 276 rpm at the loading stage of 100% using 100% biodiesel fuel (B100), as shown in Table 2. At all loadings, stages with increased biodiesel percentages in the blended fuel samples resulted in decreased engine speed because the heating value of biodiesel is lower than that of mineral diesel32,33,34,35.Figure 2Effects of engine load on (a) engine speed, (b) PTO torque, (c) PTO speed on PTO torque, (d) engine load on brake power, (e) engine speed on brake power, (f) engine load on fuel consumption, (g) engine speed on fuel consumption, (h) engine load on (BSFC). (i) engine speed on (BSFC), (j) engine load on BMEP, (k) engine speed on BMEP, (l) engine speed on BTE and (m) engine load on BTE.Full size imageTable 2 Interaction effects between engine load percentage and fuel blends percentage on power take-off speed, power take-off power, power take-off torque, engine speed, brake power, brake specific fuel consumption, brake thermal efficiency, fuel consumption, brake mean effective pressure, O2 percentage, CO2 percentage, CO, NO, and SO2.Full size tablePTO torqueThe results presented in Table 1 showed the significant effect of load percentage on PTO torque, where a loading stage of 75% achieved the highest PTO torque among all loading stage percentages, and the lowest value for PTO torque was obtained with a loading stage of 0%. Regarding the effects of fuel blend percentage on PTO torque, the results in Table 1 indicated that the fuel blends significantly affected PTO torque, and the highest value of this trait was achieved with B0 blend (100% diesel fuel) in comparison to the other blend percentages, while the lowest PTO torque was given with 100% biodiesel. The relationship between the torque of PTO shaft, Nm, and PTO load in percentage, and speed in rpm are shown in Fig. 2b,c, respectively. Increased PTO load resulted in decreased PTO speed and increased PTO torque until maximum torque values were reached for all blended fuel samples at a loading stage of 75% and a speed between 316 and 332 rpm, and then the torque decreased incrementally until the maximum loading stage was reached at a minimum PTO speed. Table 2 presents the results of the interactions between engine load percentage and fuel blend percentage, indicating that the maximum PTO torque was 663 Nm at a loading stage of 75% and PTO speed of 332 rpm, using 100% diesel fuel (B0), and the minimum PTO torque was 98.51 Nm at loading stage of 0% and PTO speed of 699.19, rpm using 100% diesel fuel (B0). At all loading stages, increasing biodiesel percentage in the blended fuel samples resulted in decreased PTO torque, which, due to the heating value of biodiesel, was lower than that of diesel fuel34,35,36. The values for PTO torque were close at different biodiesel percentages at the loading stage 0%, but engine performance cannot be judged at the no load stage with minimum torque, so the PTO load should be increased to see the difference between fuel types.Engine brake powerData in Table 1 showed that engine load percentage significantly affected BP, kW, such that engine load of 50% achieved the highest BP, and the lowest value for BP was obtained with 100% load. The results given in Table 1 show that fuel blend percentage was significantly affected BP, whereas the highest value for this trait was achieved with the 0% blend (100% diesel fuel) in comparison to the other blend percentage, while the lowest BP was given with 100% biodiesel. The interactions among BP, engine load, and engine speed were significant and were as presented in Fig. 2d, e. Moreover, increased engine load resulted in decreased engine speed and increasing BP until the highest value was reached at the loading stage of (50%) at engine speeds of 2034–2137 rpm for all fuel types shown in Table 2, which was due to the increased mass of burning fuel. The BP decreased until engine stop at a maximum loading stage of 100%, which was due to the effects of higher frictional force at the maximum loading stage33,34,35,37. The maximum BP was 46.2 kW at a loading stage of 50% and a speed of 2137 rpm at 100% diesel fuel (B0), while the minimum BP was 5.82 kW at a maximum loading stage of 100% and a speed of 276 rpm using 100% biodiesel (B100). At all loading stages, increased biodiesel percentages resulted in decreased BP because the calorific value of biodiesel was lower than that of diesel, as noted.Fuel consumptionData in Table 1 showed that engine load percentage affected significantly fuel consumption; 50% load achieved the highest fuel consumption, and the lowest value for fuel consumption was obtained for 0% load. The results in Table 1 showed that fuel blends percentage significantly affected fuel consumption, and the highest value of fuel consumption was recorded with the B100 blend (100% biodiesel fuel), and the lowest was given with the B0 blend of 100% diesel fuel. The significant interaction between fuel consumption, kg/h (Kilogram per hour) and each of engine load and speed are shown in Fig. 2f,g and the interaction between engine load percentage and fuel blend percentage are shown in Table 2, such that increased engine load resulted in decreased engine speed and increased fuel consumption until reaching the maximum value at a loading stage of 50% at maximum BP, which was because of the increased mass of burning fuel at this stage, and then the fuel consumption decreasing until reaching maximum loading33,34,35. The maximum fuel consumption was 18.24 kg/h at an engine speed of 2034.35 rpm using 100% biodiesel B100 at a loading stage of 50%. The minimum fuel consumption was 9.76 kg/h at an engine speed of 2692.9 rpm using 100% biodiesel B100 at a no-load stage. At loading stages between 0 and 100%, increasing biodiesel percentage resulted in increased fuel consumption, which is because the density of biodiesel was higher than that of diesel fuel.Brake specific fuel consumptionThe results in Table 1 indicated that engine load percentage significantly affected BSFC, such that the highest BSFC was achieved with an engine load of 100%, while the lowest value was obtained with an engine load of 50%. Other results shown in Table 1 indicated that increased biodiesel percentage in fuel blends produced significantly increased BSFC, and the maximum value of BSFC was given with B100 (100% biodiesel fuel); the lowest was seen with B0 percentage (100% diesel fuel). The relationship of interaction between (BSFC), (Kilogram per kilowatt hour) kg/kWh, engine load, and engine speed are shown in Fig. 2h,i, indicating that increased engine load resulted in decreased engine speed and BSFC until the minimum value was reached at a loading stage of 50% at maximum BP and fuel consumption. Then, the BSFC increased until it reached maximum value at a maximum loading stage of 100%, which was due to the highest frictional force and the lowest BP occurring at this loading stage33,34,35. The maximum (BSFC) was 1.95 kg/kWh at a loading stage of 100% and an engine speed of 276 rpm using 100% biodiesel fuel (B100); the minimum BSFC was 0.32 kg/kWh at an engine speed of 2137 rpm and a loading stage of 50% using 100% diesel fuel (B0), as shown in Table 2. At all loading stages, increased biodiesel percentages resulted in increased BSFC, except at the no loading stage. This is because the fuel consumption for biodiesel was higher than that for mineral diesel. Additionally, the calorific value of biodiesel was lower than that for diesel fuel, and the viscosity of the biodiesel was higher than that for mineral diesel, which leads to unfavorable pumping and spray characteristics36,38.Brake mean effective pressureThe results in Table 1 indicated a significant effect of engine load percentage on BMEP, such that the highest BMEP was given by an engine load of 75%, and the other side the lowest value for BMEP was obtained for an engine load of 0%. The results given in the same table indicated that increased biodiesel percentage in fuel blends significantly decreased BMEP. The maximum value of BMEP was given with the 0 blend (100% diesel fuel), and the lowest BMEP was given with 100% biodiesel fuel. The interaction between BMEP, kPa, engine load, and engine speed are shown in Fig. 2j,k. The data in Table 2 show the interaction between engine load percentage and fuel blend percentage. It can be clearly seen that increased engine load resulted in decreased engine speed and increased BMEP until the maximum value was reached at a loading stage of 75% at engine speeds between 1293 and 1355 rpm. The BMEP decreased with slight values until reaching the maximum loading stage at minimum engine speeds between 276 and 288 rpm. The maximum BMEP was 625 kPa at an engine speed of 1355 rpm, using 100% diesel fuel (B0) at a loading stage of 75%. The minimum BMEP was 92 kPa at an engine speed of 2692 rpm, using 100% biodiesel (B100) at no loading stage. At all loading stages, increased biodiesel percentage resulted in decreased BMEP, except that there was no loading stage at which the BSFC did not change with different biodiesel percentages. This is because the effect of increased engine speed resulted in a decreased time remaining for combustion and resulted in an insufficient motion of air in the cylinder. Both effects decreased the combustion efficiency and the BMEP values, as shown in Fig. 2j according to33,34,35,39.Brake thermal efficiencyThe results shown in Table 1 cleared that engine load percentage significantly affected BTE; the highest BTE was recorded with a 50% load, and the lowest one was given with a 0% load percentage. Table 1 also indicated that fuel blend percentage significantly affected BTE, and the maximum value for BTE was given with 0 blend (100% diesel fuel). The lowest value was obtained with 100% biodiesel (B100). The relationship between BTE and engine load and engine speed are shown in Figs. 2l,m. Increased engine load caused decreased engine speed and increased BTE until the maximum value was reached at a loading stage of 50%; BTE decreased until a minimum value was reached at a maximum loading stage of 100% and minimum engine speeds between 276 and 288 rpm. The maximum BTE was 26% at a speed of 2137.17 rpm using 100% diesel fuel (B0) at loading stage of 50%. The minimum BTE was 4.4% at speed of 276 rpm, using 100% biodiesel (B100) at the maximum loading stage of 100%, as shown in Table 2. For all loadings stages increased biodiesel percentage resulted in decreased BTE, except at the no loading and maximum loading stages, where the BTE did not change with different biodiesel percentages. This is because the density of waste frying oil biodiesel was higher than that of diesel fuel, while its calorific value and volatility was lower, such that the combustion characteristics of biodiesel were lower than those of diesel fuel34,35,36,40.Gas emissions qualityThe results in Table 1 showed that an engine load of 0% significantly increased O2 emissions, and fuel blends of 100% biodiesel also increased O2 emissions relative to the other treatments. The relationships between O2 emissions, biodiesel percentage, engine load, and engine speed are shown in Fig. 3a,b. Increased engine load resulted in decreased O2 emissions because of the increased engine consumption of O2 to optimize fuel combustion, while increased engine speed resulted in increased O2 emissions. The maximum O2 emissions were 15.3% at the minimum loading stage for all fuel blends, while the minimum O2 emissions were 4.3% at maximum loading stage for 100% diesel fuel, as presented in Table 2. At all loading stages, increased biodiesel percentage in the blended fuel samples resulted in increased O2 emissions, except at the no loading stage, where the oxygen content in the biodiesel was about 10 to 12% higher than that of diesel fuel34,35,41,42.Figure 3Effects of engine load on (a) engine load on O2 emissions, (b) engine speed on O2 emissions, (c) engine load on CO2 emissions, (d) engine speed on CO2 emissions, (e) engine load on CO emissions, (f) engine speed on CO emissions, (g) engine load on NO emissions, (h) engine speed on NO emissions, (i) engine load on SO2 emissions and (j) engine speed on SO2 emissions.Full size imageThe results in Table 1 showed that engine loading of 100% significantly increased CO2 and CO emissions, and the fuel blend of 100% diesel fuel (B0) increased CO2 and CO emissions relative to other treatments. The relationship between CO2 emissions, engine load, and engine speed are presented in Fig. 3c,d and Table 2. Increased engine load resulted in increased CO2 emissions until a maximum loading stage of 100% was reached, while increased engine speed resulted in decreased CO2 emissions. The maximum value for CO2 emissions was 12.3% at the maximum loading stage using 100% diesel (B0), and the minimum CO2 emissions was 4.2% at the no loading stage for all fuel blends. At loading stages of 50, 75, and 100%, increased biodiesel percentage in the blended fuel samples resulted in decreased CO2 emissions, which due to the oxygen content in the biodiesel was about 10–12%. A higher oxygen content contributes to increasing ignition quality and decrease CO2 emissions35,36,41.The relationship between CO emissions, biodiesel percentage, engine load, and engine speed are shown in Fig. 3e,f. For all tested fuel samples, increased engine load resulted in a greater increase in CO emissions, until a maximum load was reached except at 100% biodiesel (B100), which increased slightly. Increased engine speed resulted in a sharp decrease in CO emissions until the maximum speed was reached, except at B100, which decreased slightly43,44,45. The maximum CO emissions value was 369 ppm at the maximum loading stage using 100% diesel fuel (B0), while the minimum CO emissions was 69 ppm at the minimum loading stage using 100% biodiesel fuel (B100). At all loading stages, increased biodiesel percentage resulted in decreased CO emissions except that at loading stages of 25% and 50%, for which the values of CO emissions were close. This was because high oxygen content in biodiesel increases ignition quality and decreases CO emissions, so increased biodiesel percentages reduce environmental pollution36,43,44,45,46. The results in Table 2 showed that an engine load of 75% significantly increased NO emissions, and 100% biodiesel fuel (B100) increased NO emissions relative to the other treatments.The relationship between NO emissions, engine load, and engine speed are shown in Fig. 3g,h. Increased engine load resulted in decreased engine speed and increased NO emissions until the maximum value was reached at a loading stage of 75%. NO emissions decreased until reach a loading stage of 100% was reached with a minimum engine speed. The maximum NO emissions were 593 ppm at a loading stage of 75% using 100% biodiesel fuel (B100), while the minimum NO emissions were 266 ppm at the minimum loading stage using (B100) as showed in Table 1. At all loading stages, increased biodiesel percentages in the blended fuel samples resulted in increased NO emissions, except at the no loading stage, which was due to the increased burned fuel, which resulted in increased cylinder temperature. This was responsible for thermal NOx formation. Higher flame and cylinder temperatures with high oxygen content in the biodiesel led to higher NOx36,43,44,45,46. Table 2 shows that the engine load of 100% significantly increased SO2 emissions, and 100% diesel fuel increased SO2 emissions, relative to the other treatments.The relationship between SO2 emissions, diesel percentage, engine load, and engine speed are shown in Fig. 3I,j and Table 1. Increased engine load resulted in increased SO2 emissions, and increased engine speed resulted in decreased SO2 emissions. There were no SO2 emissions by using 100% biodiesel (B100). The maximum SO2 emissions was 21 ppm at maximum loading stage using 100% diesel (B0). At all loading stages increasing biodiesel percentage in the blended fuel resulted in decreasing SO2 emissions43,44,45,46. More

  • in

    Whole genome sequencing reveals high differentiation, low levels of genetic diversity and short runs of homozygosity among Swedish wels catfish

    Allendorf FW (2017) Genetics and the conservation of natural populations: allozymes to genomes. Mol Ecol 26(2):420–430CAS 
    PubMed 
    Article 

    Google Scholar 
    Allendorf FW, Hohenlohe PA, Luikart G (2010) Genomics and the future of conservation genetics. Nat Rev Genet 11(10):697–709CAS 
    PubMed 
    Article 
    PubMed Central 

    Google Scholar 
    Allendorf FW, Luikart G (2007) Conservation and the genetics of populations. Blackwell Publishing, Oxford, UK
    Google Scholar 
    Allendorf FW, Luikart G, Aitken SN (2013) Conservation and the genetics of populations, 2nd ed. Blackwell Publishing, Oxford, UK
    Google Scholar 
    Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ (1990) Basic Local Alignment Searsh Tool. J Mol Biol 215(3):403–410CAS 
    PubMed 
    PubMed Central 
    Article 

    Google Scholar 
    Andrews S (2010) FastQC: a quality control tool for high throughput sequence data. http://www.bioinformatics.babraham.ac.uk/projects/fastqc/ArtDatabanken (2020) Mal Silurus glanis. https://artfakta.se/naturvard/taxon/100131Begun DJ, Holloway AK, Stevens K, Hillier LW, Poh YP, Hahn MW et al. (2007) Population genomics: Whole-genome analysis of polymorphism and divergence in Drosophila simulans. PLOS Biol 5(11):2534–2559CAS 
    Article 

    Google Scholar 
    Borger T, Kjellberg A (2006) Malprovfiske i Emån 2006 [Fish survey for wels catfish in Emån 2006; in Swedish]. Länsstyrelsen i Kalmar län informerar. Meddelande 2006:16. Länsstyrelsen i Kalmar Län
    Google Scholar 
    Brandies P, Peel E, Hogg CJ, Belov K (2019) The value of reference genomes in the conservation of threatened species. Genes 10(11):846CAS 
    PubMed Central 
    Article 
    PubMed 

    Google Scholar 
    Bylak A, Kukuła K (2018) Importance of peripheral basins: implications for the conservation of fish assemblages. Aquat Conserv Mar Freshw Ecosyst 28:1055–1066Article 

    Google Scholar 
    Bylak A, Kukuła K (2020) Conservation of fish communities: Extending the ‘research life cycle’ by achieving practical effects. Aquat Conserv Mar Freshw Ecosyst 30:1741–1746Article 

    Google Scholar 
    Calles EO, Greenberg LA (2005) Evaluation of nature-like fishways for re-establishing connectivity in fragmented salmonid populations in the River Emån. River Res Appl 21:951–960Article 

    Google Scholar 
    Carol J, Zamora L, García-Berthou E (2007) Preliminary telemetry data on the movement patterns and habitat use of European catfish (Silurus glanis) in a reservoir of the River Ebro, Spain. Ecol Freshw Fish 16:450–456Article 

    Google Scholar 
    Ceballos FC, Joshi PK, Clark DW, Ramsay M, Wilson JF (2018) Runs of homozygosity: windows into population history and trait architecture. Nat Rev Genet 19(4):220–235CAS 
    PubMed 
    Article 

    Google Scholar 
    Channell R (2004) The conservation value of peripheral populations: The supporting science. In: Hooper TD (ed.) Proceedings of the species at risk. Pathways to Recovery Conference. Conference Organizing Committee, Victoria, BCChannell R, Lomolino MV (2000) Dynamic biogeography and conservation of endangered species. Nature 403:84–86CAS 
    PubMed 
    Article 

    Google Scholar 
    Copp GH, Britton JR, Cucherousset J, Garcia-Berthou E, Kirk R, Peeler E et al. (2009) Voracious invader or benign feline? A review of the environmental biology of European catfish Silurus glanis in its native and introduced ranges. Fish Fish 10(3):252–282Article 

    Google Scholar 
    Cucherousset J, Horky P, Slavik O, Ovidio M, Arlinghaus R, Bouletreau S et al. (2018) Ecology, behaviour and management of the European catfish. Rev Fish Biol Fish 28(1):177–190Article 

    Google Scholar 
    Danecek P, Auton A, Abecasis G, Albers CA, Banks E, DePristo MA et al. (2011) The variant call format and VCFtools. Bioinformatics 27(15):2156–2158CAS 
    PubMed 
    PubMed Central 
    Article 

    Google Scholar 
    DePristo MA, Banks E, Poplin R, Garimella KV, Maguire JR, Hartl C et al. (2011) A framework for variation discovery and genotyping using next-generation DNA sequencing data. Nat Genet 43(5):491–498CAS 
    PubMed 
    PubMed Central 
    Article 

    Google Scholar 
    Eckert CG, Samis KE, Lougheed SC (2008) Genetic variation across species’ geographical ranges: the central-marginal hypothesis and beyond. Mol Ecol 17(5):1170–1188CAS 
    PubMed 
    Article 
    PubMed Central 

    Google Scholar 
    Falush D, Stephens M, Pritchard JK (2003) Inference of population structure using multilocus genotype data: linked loci and correlated allele frequencies. Genetics 164(4):1567–1587CAS 
    PubMed 
    PubMed Central 
    Article 

    Google Scholar 
    Frankham R, Ballou JD, Briscoe DA (2010) Introduction to conservation genetics, 2 edn. Cambridge University Press, CambridgeBook 

    Google Scholar 
    Frankham R, Ballou JD, Eldridge MDB, Lacy RC, Ralls K, Dudash MR et al. (2011) Predicting the probability of outbreeding depression. Conserv Biol 25(3):465–475PubMed 
    Article 
    PubMed Central 

    Google Scholar 
    Fraser DJ, Bernatchez L (2001) Adaptive evolutionary conservation: towards a unified concept for defining conservation units. Mol Ecol 10(12):2741–2752CAS 
    PubMed 
    Article 
    PubMed Central 

    Google Scholar 
    Freyhof J (2010). Silurus glanis (errata version published in 2018). The IUCN red list of threatened species. https://www.iucnredlist.org/species/40713/136595620#errataGarcía-Alcalde F, Okonechnikov K, Carbonell J, Cruz LM, Götz S, Tarazona S et al. (2012) Qualimap: evaluating next-generation sequencing alignment data. Bioinformatics 28:2678–2679PubMed 
    Article 
    CAS 
    PubMed Central 

    Google Scholar 
    Garner BA, Hand BK, Amish SJ, Bernatchez L, Foster JT, Miller KM et al. (2016) Genomics in conservation: case studies and bridging the gap between data and application. Trends Ecol Evol 31(2):81–83PubMed 
    Article 
    PubMed Central 

    Google Scholar 
    Gibson J, Newton ME, Collins A (2006) Extended tracts of homozygosity in outbred human populations. Hum Mol Genet 15(5):789–795CAS 
    PubMed 
    Article 
    PubMed Central 

    Google Scholar 
    Guillerault N, Delmotte S, Bouletreau S, Lauzeral C, Poulet N, Santoul F (2015) Does the non-native European catfish Silurus glanis threaten French river fish populations? Freshw Biol 60(5):922–928Article 

    Google Scholar 
    Havs-och-vattenmyndighetens. (2017) Åtgärdsprogram för mal (Silurus glanis). [Swedish Agency for Marine and Water Management. Action plan for wels catfish in Sweden; in Swedish]. Havs- och Vattenmyndighetens Rapp 2017:33
    Google Scholar 
    Helyar SJ, Hemmer-Hansen J, Bekkevold D, Taylor MI, Ogden R, Limborg MT et al. (2011) Application of SNPs for population genetics of nonmodel organisms: new opportunities and challenges. Mol Ecol Resour 11:123–136PubMed 
    Article 
    PubMed Central 

    Google Scholar 
    Hendricks S, Anderson EC, Antao T, Bernatchez L, Forester BR, Garner B et al. (2018) Recent advances in conservation and population genomics data analysis. Evol Appl 11(8):1197–1211PubMed Central 
    Article 

    Google Scholar 
    Hohenlohe PA, Funk WC, Rajora OP (2020) Population genomics for wildlife conservation and management. Mol Ecol 30:62–82PubMed 
    PubMed Central 
    Article 

    Google Scholar 
    Hohenlohe PA, Rajora OP (eds) (2020) Population genomics: wildlife. Population Genomics. Springer, ChamHöglund J (2009) Evolutionary Conservation Genetics. Oxford University Press, OxfordBook 

    Google Scholar 
    Katoh K, Rozewicki J, Yamada KD (2019) MAFFT online service: multiple sequence alignment, interactive sequence choice and visualization. Brief Bioinform 20:1160–1166CAS 
    PubMed 
    Article 
    PubMed Central 

    Google Scholar 
    Kimura M (1983) The neutral theory of molecular evolution. Cambridge University Press, CambridgeBook 

    Google Scholar 
    Krieg F, Triantafyllidis A, Guyomard R (2000) Mitochondrial DNA variation in European populations of Silurus glanis. J Fish Biol 56(3):713–724CAS 
    Article 

    Google Scholar 
    Lamichhaney S, Fuentes-Pardo AP, Rafati N, Ryman N, McCracken GR, Bourne C et al. (2017) Parallel adaptive evolution of geographically distant herring populations on both sides of the North Atlantic Ocean. Proc Natl Acad Sci USA 114(17):E3452–E3461CAS 
    PubMed 
    Article 

    Google Scholar 
    Leigh JW, Bryant D (2015) popart: full-feature software for haplotype network construction (S Nakagawa, Ed.). Methods Ecol Evol 6:1110–1116Article 

    Google Scholar 
    Lesica P, Allendorf FW (1995) When are peripheral-populations valuable for conservation. Conserv Biol 9(4):753–760Article 

    Google Scholar 
    Li H, Durbin R (2009) Fast and accurate short read alignment with Burrows-Wheeler transform. Bioinformatics 25(14):1754–1760CAS 
    PubMed 
    PubMed Central 
    Article 

    Google Scholar 
    Li H, Handsaker B, Wysoker A, Fennell T, Ruan J, Homer N et al. (2009) The sequence alignment/map format and SAMtools. Bioinformatics 25:2078–2079PubMed 
    PubMed Central 
    Article 
    CAS 

    Google Scholar 
    McKenna A, Hanna M, Banks E, Sivachenko A, Cibulskis K, Kernytsky A et al. (2010) The genome analysis toolkit: a MapReduce framework for analyzing next-generation DNA sequencing data. Genome Res 20(9):1297–1303CAS 
    PubMed 
    PubMed Central 
    Article 

    Google Scholar 
    McMahon BJ, Teeling EC, Hoglund J (2014) How and why should we implement genomics into conservation? Evol Appl 7(9):999–1007PubMed 
    PubMed Central 
    Article 

    Google Scholar 
    Meyermans R, Gorssen W, Buys N, Janssens S (2020) How to study runs of homozygosity using PLINK? A guide for analyzing medium density SNP data in livestock and pet species. BMC Genomics 21:94CAS 
    PubMed 
    PubMed Central 
    Article 

    Google Scholar 
    Nathanson JE (1987). Malens utbredning i Sverige. English summary: Distribution of the sheatfish (Silurus glanis) in Sweden. Information från Sötvattenslaboratoriet (Institute of Freshwater Research), DrottningholmPalm S, Prestegaard T, Dannewitz J, Petersson E, Nathanson JE (2008). Genetisk kartläggning av svenska malbestånd [Genetic survey of swedish populations of wels catfish]. Fiskeriverkets Sötvattenslaboratorium, Drottningholm & Uppsala UniversitetPalm S, Vinterstare J, Nathanson JE, Triantafyllidis A, Petersson E (2019) Reduced genetic diversity and low effective size in peripheral northern European catfish Silurus glanis populations. J Fish Biol 95(6):1407–1421PubMed 
    Article 
    PubMed Central 

    Google Scholar 
    R Core Team (2017). R: A language and environment for statistical computing. R Foundation for Statistical Computing, Vienna, Austria. http://www.R-project.org/Savolainen O, Lascoux M, Merilä J (2013) Ecological genomics of local adaptation. Nat Rev Genet 14(11):807–820CAS 
    PubMed 
    Article 

    Google Scholar 
    Schiffels S, Durbin R (2014) Inferring human population size and separation history from multiple genome sequences. Nat Genet 46(8):919–925CAS 
    PubMed 
    PubMed Central 
    Article 

    Google Scholar 
    Shafer ABA, Wolf JBW, Alves PC, Bergström L, Bruford MW, Brannstrom I et al. (2015) Genomics and the challenging translation into conservation practice. Trends Ecol Evol 30(2):78–87PubMed 
    Article 

    Google Scholar 
    Shafer ABA, Wolf JBW, Alves PC, Bergström L, Colling G, Dalen L et al. (2016) Genomics in conservation: case studies and bridging the gap between data and application reply. Trends Ecol Evol 31(2):83–84PubMed 
    Article 

    Google Scholar 
    Shendure J, Ji HL (2008) Next-generation DNA sequencing. Nat Biotech 26(10):1135–1145CAS 
    Article 

    Google Scholar 
    Svensson M, Kjellberg A, Lessmark O, Nathanson JE, Almer B, Wagnström J (2013). Beskrivning av förväntade effekter av återintroduktion av mal i nedre delen av Skräbeåns vattensystem [Description of expected effects of reintroduction of wels catfish in the lower parts of Skräbeåns watersystem]. Ivösjöns FiskevårdsföreningTallmon DA, Luikart G, Waples RS (2004) The alluring simplicity and complex reality of genetic rescue. Trends Ecol Evol 19(9):489–496PubMed 
    Article 

    Google Scholar 
    Taylor HR, Dussex N, van Heezik Y (2017) Bridging the conservation genetics gap by identifying barriers to implementation for conservation practitioners. Global Ecol Conserv 10:231–242Article 

    Google Scholar 
    Triantafyllidis A, Abatzopoulos TJ, Economidis PS (1999a) Genetic differentiation and phylogenetic relationships among Greek Silurus glanis and Silurus aristotelis (Pisces, Siluridae) populations, assessed by PCR-RFLP analysis of mitochondrial DNA segments. Heredity 82:503–509CAS 
    PubMed 
    Article 

    Google Scholar 
    Triantafyllidis A, Krieg F, Cottin C, Abatzopoulos TJ, Triantaphyllidis C, Guyomard R (2002) Genetic structure and phylogeography of European catfish (Silurus glanis) populations. Mol Ecol 11(6):1039–1055CAS 
    PubMed 
    Article 

    Google Scholar 
    Triantafyllidis A, Ozouf-Costaz C, Rab P, Suciu R, Karakousis Y (1999b) Allozyme variation in European silurid catfishes, Silurus glanis and Silurus aristotelis. Biochem Syst Ecol 27(5):487–498CAS 
    Article 

    Google Scholar 
    Vittas S, Drosopoulou E, Kappas I, Pantzartzi CN, Scouras ZG (2011) The mitochondrial genome of the European catfish Silurus glanis (Siluriformes, Siluridae). J Biol Res 15:25–35CAS 

    Google Scholar 
    Weisenfeld NI, Kumar V, Shah P, Church DM, Jaffe DB (2017) Direct determination of diploid genome sequences. Genome Res 27(5):757–767CAS 
    PubMed 
    PubMed Central 
    Article 

    Google Scholar 
    Zoonomia Consortium (2020) A comparative genomics multitool for scientific discovery and conservation. Nature 597:240–245Article 
    CAS 

    Google Scholar  More

  • in

    Multiple social network influences can generate unexpected environmental outcomes

    1.Amel, E., Manning, C., Scott, B. & Koger, S. Beyond the roots of human inaction: Fostering collective effort toward ecosystem conservation. Science 356, 275–279 (2017).
    Google Scholar 
    2.Bodin, Ö. Collaborative environmental governance: Achieving collective action in social-ecological systems. Science 357, eaan1114 (2017).
    Google Scholar 
    3.Cinner, J. E. How behavioral science can help conservation. Science 362, 889–891 (2018).
    Google Scholar 
    4.Abrahamse, W. & Steg, L. Social influence approaches to encourage resource conservation: A meta-analysis. Glob. Environ. Chang. 23, 1773–1785 (2013).
    Google Scholar 
    5.Christoff, Z., Hansen, J. U. & Proietti, C. Reflecting on social influence in networks. J. Logic Lang. Inf. 25, 299–333 (2016).
    Google Scholar 
    6.Fowler, J. H. & Christakis, N. A. Cooperative behavior cascades in human social networks. Proc. Natl. Acad. Sci. USA. 107, 5334–5338 (2010).
    Google Scholar 
    7.Friedkin, N. E. & Johnsen, E. C. Social positions in influence networks. Soc. Netw. 19, 209–222 (1997).
    Google Scholar 
    8.Christakis, N. A. & Fowler, J. H. The collective dynamics of smoking in a large social network. N. Engl. J. Med. 358, 2249–2258 (2008).
    Google Scholar 
    9.Barnes, M. L., Lynham, J., Kalberg, K. & Leung, P. Social networks and environmental outcomes. Proc. Natl. Acad. Sci. 113, 6466–6471 (2016).
    Google Scholar 
    10.McPherson, M., Smith-lovin, L. & Cook, J. M. Homophily in social networks. Annu. Rev. Sociol. 27, 415–444 (2001).
    Google Scholar 
    11.Bodin, Ö., Mancilla García, M. & Robins, G. Reconciling conflict and cooperation in environmental governance: A social network perspective. Annu. Rev. Environ. Resour. 45, 471–495 (2020).
    Google Scholar 
    12.Bodin, Ö. & Prell, C. Social Networks and Natural Resource. Management Uncovering the Social Fabric of Environmental Governance (Cambridge University Press, 2011).
    Google Scholar 
    13.Small, B., Brown, P. & Montes de Oca Munguia, O. Values, trust, and management in New Zealand agriculture. Int. J. Agric. Sustain. 14, 282–306 (2016).
    Google Scholar 
    14.Friedman, R. S. et al. Beyond the community in participatory forest management: A governance network perspective. Land Use Policy 97, 104738 (2020).
    Google Scholar 
    15.Schill, C. et al. A more dynamic understanding of human behaviour for the Anthropocene. Nat. Sustain. 2, 1075–1082 (2019).
    Google Scholar 
    16.Yletyinen, J., Hentati-Sundberg, J., Blenckner, T. & Bodin, O. Fishing strategy diversification and fishers’ ecological dependency. Ecol. Soc. 23, 28 (2018).
    Google Scholar 
    17.Grêt-Regamey, A., Huber, S. H. & Huber, R. Actors’ diversity and the resilience of social-ecological systems to global change. Nat. Sustain. 2, 290–297 (2019).
    Google Scholar 
    18.Kremen, C. & Merenlender, A. M. Landscapes that work for biodiversity and people. Science 362, eaau6020 (2018).
    Google Scholar 
    19.de Lange, E., Milner-Gulland, E. J. & Keane, A. Improving environmental interventions by understanding information flows. Trends Ecol. Evol. 34, 1034–1047 (2019).
    Google Scholar 
    20.Vainio, A., Paloniemi, R. & Hujala, T. How are forest owners’ objectives and social networks related to successful conservation?. J. Rural Stud. 62, 21–28 (2018).
    Google Scholar 
    21.de Snoo, G. R. et al. Toward effective nature conservation on farmland: Making farmers matter. Conserv. Lett. 6, 66–72 (2013).
    Google Scholar 
    22.Hanski, I. Habitat loss, the dynamics of biodiversity, and a perspective on conservation. Ambio 40, 248–255 (2011).
    Google Scholar 
    23.Wintle, B. A. et al. Global synthesis of conservation studies reveals the importance of small habitat patches for biodiversity. Proc. Natl. Acad. Sci. 116, 909–914 (2018).
    Google Scholar 
    24.Hill, R. et al. A social-ecological systems analysis of impediments to delivery of the Aichi 2020 Targets and potentially more effective pathways to the conservation of biodiversity. Glob. Environ. Chang. 34, 22–34 (2015).
    Google Scholar 
    25.Bengtsson, J. et al. Reserves, resilience and dynamic landscapes. AMBIO J. Hum. Environ. 32, 389–396 (2016).
    Google Scholar 
    26.Johnson, C. N. et al. Biodiversity losses and conservation responses in the Anthropocene. Science 356, 270–275 (2017).
    Google Scholar 
    27.Miller, B. W., Caplow, S. C. & Leslie, P. W. Feedbacks between conservation and social-ecological systems. Conserv. Biol. 26, 218–227 (2012).
    Google Scholar 
    28.Larrosa, C., Carrasco, L. R. & Milner-Gulland, E. J. Unintended feedbacks: Challenges and opportunities for improving conservation effectiveness. Conserv. Lett. 9, 316–326 (2016).
    Google Scholar 
    29.Reyers, B. & Selig, E. R. Global targets that reveal the social–ecological interdependencies of sustainable development. Nat. Ecol. Evol. 4, 1011–1019 (2020).
    Google Scholar 
    30.Brehony, P., Tyrrell, P., Kamanga, J., Waruingi, L. & Kaelo, D. Incorporating social-ecological complexities into conservation policy. Biol. Conserv. 248, 108697 (2020).
    Google Scholar 
    31.Jacob, U. et al. Marine conservation: Towards a multi-layered network approach. Philos. Trans. R. Soc. B. Biol. Sci. 375, 20190459 (2020).
    Google Scholar 
    32.Hoole, A. & Berkes, F. Breaking down fences: Recoupling social-ecological systems for biodiversity conservation in Namibia. Geoforum 41, 304–317 (2010).
    Google Scholar 
    33.Dajka, J. et al. Red and green loops help uncover missing feedbacks in a coral reef social–ecological system. People Nat. 2, 608–618 (2020).
    Google Scholar 
    34.Yletyinen, J. et al. Understanding and managing social-ecological tipping points in primary industries. Bioscience 69, 335–347 (2019).
    Google Scholar 
    35.Mason, W. A., Conrey, F. R. & Smith, E. R. Situating social influence processes: Dynamic, multidirectional flows of influence within social networks. Personal. Soc. Psychol. Rev. 11, 279–300 (2007).
    Google Scholar 
    36.Niemiec, R. M., Willer, R., Ardoin, N. M. & Brewer, F. K. Motivating landowners to recruit neighbors for private land conservation. Conserv. Biol. 33, 930–941 (2019). 
    Google Scholar 
    37.Brown, P. Survey of rural decision makers. Manaaki Whenua Landcare Res. https://doi.org/10.7931/J2736P2D (2015).
    Google Scholar 
    38.Burt, R. S. & Doreian, P. Testing a structural model of perception: Conformity and deviance with respect to Journal norms in elite sociological methodology. Qual. Quant. 16, 109–150 (1982).
    Google Scholar 
    39.Zhang, B., Pavlou, P. A. & Krishnan, R. On direct vs. indirect peer influence in large social networks. Inf. Syst. Res. 29, 292–314 (2018).
    Google Scholar 
    40.Pinheiro, F. L., Santos, M. D., Santos, F. C. & Pacheco, J. M. Origin of peer influence in social networks. Phys. Rev. Lett. 112, 1–5 (2014).
    Google Scholar 
    41.Lewis, K., Gonzalez, M. & Kaufman, J. Social selection and peer influence in an online social network. Proc. Natl. Acad. Sci. 109, 68–72 (2012).
    Google Scholar 
    42.Stein, C., Barron, J. & Ernstson, H. A social network approach to analyze multi-stakeholders governance arrangement in water resources management: Three case studies from catchments in Burkina Faso, Tanzania and Zambia. In Proceedings of the XIVth World Water Congress, 25–29 September, at Porto de Galinhas, Pernambuco, Brazil. (2011).43.Autant-bernard, C., Mairesse, J. & Massard, N. Spatial knowledge diffusion through collaborative networks. Pap. Reg. Sci. 86, 341–350 (2007).
    Google Scholar 
    44.Ward, P. S. & Pede, V. O. Capturing social network effects in technology adoption: The spatial diffusion of hybrid rice in Bangladesh. Aust. J. Agric. Resour. Econ. 59, 225–241 (2015).
    Google Scholar 
    45.Kuhfuss, L. et al. Nudges, social norms, and permanence in agri-environmental schemes. Land Econ. 92, 641–655 (2016).
    Google Scholar 
    46.Fehr, E. & Schurtenberger, I. Normative foundations of human cooperation. Nat. Hum. Behav. 2, 458–468 (2018).
    Google Scholar 
    47.Delaroche, M. Adoption of conservation practices: What have we learned from two decades of social-psychological approaches?. Curr. Opin. Environ. Sustain. 45, 25–35 (2020).
    Google Scholar 
    48.Knowler, D. & Bradshaw, B. Farmers’ adoption of conservation agriculture: A review and synthesis of recent research. Food Policy 32, 25–48 (2007).
    Google Scholar 
    49.O’Sullivan, D. & Perry, G. L. W. Spatial Simulation. Exploring Pattern and Process (Wiley, 2013).
    Google Scholar 
    50.Will, M., Groeneveld, J., Frank, K. & Müller, B. Combining social network analysis and agent-based modelling to explore dynamics of human interaction: A review. Socio-Environ. Syst. Model. 2, 16325 (2020).
    Google Scholar 
    51.Bodin, Ö. & Crona, B. I. The role of social networks in natural resource governance: What relational patterns make a difference?. Glob. Environ. Chang. 19, 366–374 (2009).
    Google Scholar 
    52.Erdős, P. & Rényi, A. On random graphs. Publ. Math. 6, 290–297 (1959).
    Google Scholar 
    53.Hanski, I. Dynamics of regional distribution: The core and satellite species hypothesis. Oikos 38, 210–221 (1982).
    Google Scholar 
    54.Groce, J. E., Farrelly, M. A., Jorgensen, B. S. & Cook, C. N. Using social-network research to improve outcomes in natural resource management. Conserv. Biol. 33, 53-65 (2018).
    Google Scholar 
    55.Schill, C., Wijermans, N., Schlüter, M. & Lindahl, T. Cooperation is not enough – Exploring social-ecological micro-foundations for sustainable common-pool resource use. PLoS ONE 11, e0165009 (2016).
    Google Scholar 
    56.Valente, T. W. Network interventions. Science 337, 49–53 (2012).
    Google Scholar 
    57.Valente, T. W. Putting the network in network interventions. Proc. Natl. Acad. Sci. USA. 114, 9500–9501 (2017).
    Google Scholar 
    58.Kossinets, G. & Watts, D. J. Empirical analysis of an evolving social network. Science 311, 88–90 (2006).
    Google Scholar 
    59.De Domenico, M., Solé-Ribalta, A., Omodei, E., Gómez, S. & Arenas, A. Ranking in interconnected multilayer networks reveals versatile nodes. Nat. Commun. 6, 6868 (2015).
    Google Scholar 
    60.Prell, C. Social Network Analysis (SAGE publications Ltd, 2012).
    Google Scholar 
    61.Thampi, V. A., Anand, M. & Bauch, C. T. Socio-ecological dynamics of Caribbean coral reef ecosystems and conservation opinion propagation. Sci. Rep. 8, 2597 (2018).
    Google Scholar 
    62.Dannenberg, A. & Barrett, S. Cooperating to avoid catastrophe. Nat. Hum. Behav. 2, 435–437 (2018).
    Google Scholar 
    63.Rasoulkhani, K., Logasa, B., Reyes, M. P. & Mostafavi, A. Understanding fundamental phenomena affecting the water conservation technology adoption of residential consumers using agent-based modeling. Water 10, 993 (2018).
    Google Scholar 
    64.Wang, P., Robins, G., Pattison, P. & Lazega, E. Exponential random graph models for multilevel networks. Soc. Netw. 35, 96–115 (2013).
    Google Scholar 
    65.Kivelä, M. et al. Multilayer networks. J. Complex Networks 2, 203–271 (2014).
    Google Scholar 
    66.Gao, J., Buldyrev, S. V., Stanley, H. E. & Havlin, S. Networks formed from interdependent networks. Nat. Phys. 8, 40–48 (2011).
    Google Scholar 
    67.May, R. M., Levin, S. A. & Sugihara, G. Complex systems: Ecology for bankers. Nature 451, 893–895 (2008).
    Google Scholar 
    68.Grimm, V. et al. The ODD protocol for describing agent-based models: a second update to improve clarity, replication and structural realism. J. Artif. Soc. Soc. Simul. 23(2), 7 (2020).
    Google Scholar 
    69.Alexander, S. M., Bodin, Ö. & Barnes, M. L. Untangling the drivers of community cohesion in small-scale fisheries. Int. J. Commons 12, 519–547 (2018).
    Google Scholar 
    70.QE II National Trust. QE II National Trust. Ngā Kiarauhi Papa|Forever protected. https://qeiinationaltrust.org.nz.71.Hanski, I. & Ovaskainen, O. The metapopulation capacity of a fragmented landscape. Nature 404, 755–758 (2000).
    Google Scholar 
    72.Gower, J. C. A general coefficient of similarity and some of its properties. Biometrics 27, 857–871 (1971).
    Google Scholar 
    73.Aral, S., Muchnik, L. & Sundararajan, A. Distinguishing influence-based contagion from homophily-driven diffusion in dynamic networks. Proc. Natl. Acad. Sci. US. A. 106, 21544–21549 (2009).
    Google Scholar 
    74.Stefano, A. D. et al. Quantifying the role of homophily in human cooperation using multiplex evolutionary game theory. PLoS ONE 10, e0140646 (2015).
    Google Scholar 
    75.Wilensky, U. NetLogo. http://ccl.northwestern.edu/netlogo/. (Center for Connected Learning and Computer-Based Modeling, Northwestern University, Evanston, IL, 1999).76.Thiele, J. C. R Marries NetLogo: Introduction to the RNetLogo Package. J. Stat. Softw. 58, 1–41 (2014).
    Google Scholar 
    77.R Core Team. R: A language and environment for statistical computing. https://www.R-project.org/. (R Foundation for Statistical Computing, Vienna, 2018).78.Kampstra, P. Beanplot: A boxplot alternative for visual comparison of distributions. J. Stat. Softw. Code Snippets 28, 1–9 (2008).
    Google Scholar 
    79.Warnes, G. R. et al. gplots: Various R Programming Tools for Plotting Data. R package version 3.0.1. (2016).80.Csardi, G. & Nepusz, T. The igraph software package for complex network research. Interjournal Complex Syst. 1695, 1–9 (2006).
    Google Scholar  More

  • in

    Dynamic global monitoring needed to use restoration of forest cover as a climate solution

    1.Griscom, B. W. et al. Proc. Natl Acad. Sci. USA 114, 11645–11650 (2017).CAS 
    Article 

    Google Scholar 
    2.Anderson, C. M. et al. Science 363, 933–934 (2019).CAS 
    Article 

    Google Scholar 
    3.Bastin, J.-F. et al. Science 365, 6–9 (2019).Article 

    Google Scholar 
    4.Cook-Patton, S. C. et al. Nature 585, 545–550 (2020).CAS 
    Article 

    Google Scholar 
    5.Holl, K. D. & Brancalion, P. S. Science 368, 580–582 (2020).CAS 
    Article 

    Google Scholar 
    6.Fargione, J. et al. Front. For. Glob. Change (in the press).7.West, T. A. P., Börner, J., Sills, E. O. & Kontoleon, A. Proc. Natl Acad. Sci. USA 117, 24188–24194 (2020).CAS 
    Article 

    Google Scholar 
    8.Brancalion, P. H. S. et al. L. Degrad. Dev. 32, 830–841 (2020).Article 

    Google Scholar 
    9.Sills, E. O. et al. PLoS ONE 10, e0132590 (2015).Article 

    Google Scholar 
    10.Ferraro, P. J. & Hanauer, M. M. Annu. Rev. Environ. Resour. 39, 495–517 (2014).Article 

    Google Scholar 
    11.Harris, N. L. et al. Nat. Clim. Change 11, 234–240 (2021).Article 

    Google Scholar 
    12.Reytar, K. et al. The challenge of tracking how a trillion trees grow. World Resources Institute https://www.wri.org/blog/2020/07/trillion-trees-tracking-challenges (2020).13.Shoch, D. et al. Methodology For Improved Forest Management (Family Forest Carbon Program, 2020).14.McDowell, N. G. et al. Science 368, eaaz9463 (2020).CAS 
    Article 

    Google Scholar 
    15.IPCC Special Report on Global Warming of 1.5 °C (eds Masson-Delmotte, V. et al.) (WMO, 2018). More

  • in

    Woody-biomass projections and drivers of change in sub-Saharan Africa

    1.Davis, S. J. & Caldeira, K. Consumption-based accounting of CO2 emissions. Proc. Natl Acad. Sci. USA 107, 5687–5692 (2010).CAS 
    Article 

    Google Scholar 
    2.Wiedmann, T. O. et al. The material footprint of nations. Proc. Natl Acad. Sci. USA 112, 6271–6276 (2015).CAS 
    Article 

    Google Scholar 
    3.Rogelj, J. et al. Paris Agreement climate proposals need a boost to keep warming well below 2 °C. Nature 534, 631–639 (2016).CAS 
    Article 

    Google Scholar 
    4.Brandt, M. et al. Satellite passive microwaves reveal recent climate-induced carbon losses in African drylands. Nat. Ecol. Evol. 2, 827–835 (2018).Article 

    Google Scholar 
    5.Sankaran, M. et al. Determinants of woody cover in African savannas. Nature 438, 846–849 (2005).CAS 
    Article 

    Google Scholar 
    6.Bond, W. J. & Keane, R. E. Fires, Ecological Effects of☆. In Reference Module in Life Sciences (Elsevier, 2017); https://doi.org/10.1016/B978-0-12-809633-8.02098-77.Valentini, R. et al. A full greenhouse gases budget of Africa: synthesis, uncertainties, and vulnerabilities. Biogeosciences 11, 381–407 (2014).Article 
    CAS 

    Google Scholar 
    8.Williams, C. A. et al. Africa and the global carbon cycle. Carbon Balance Manag. 2, 3 (2007).Article 
    CAS 

    Google Scholar 
    9.Hanan, N. P. Agroforestry in the Sahel. Nat. Geosci. 11, 296–297 (2018).Article 
    CAS 

    Google Scholar 
    10.Dai, A. Increasing drought under global warming in observations and models. Nat. Clim. Change 3, 52–58 (2013).Article 

    Google Scholar 
    11.Zhou, L. et al. Widespread decline of Congo rainforest greenness in the past decade. Nature 509, 86–90 (2014).CAS 
    Article 

    Google Scholar 
    12.Feng, S. & Fu, Q. Expansion of global drylands under a warming climate. Atmos. Chem. Phys. 13, 10081–10094 (2013).CAS 
    Article 

    Google Scholar 
    13.Anchang, J. Y. et al. Trends in woody and herbaceous vegetation in the savannas of West Africa. Remote Sens. 11, 576 (2019).Article 

    Google Scholar 
    14.Andela, N., Liu, Y. Y., van Dijk, A. I. J. M., de Jeu, R. A. M. & McVicar, T. R. Global changes in dryland vegetation dynamics (1988–2008) assessed by satellite remote sensing: comparing a new passive microwave vegetation density record with reflective greenness data. Biogeosciences 10, 6657–6676 (2013).Article 

    Google Scholar 
    15.Kaptué, A. T., Prihodko, L. & Hanan, N. P. On regreening and degradation in Sahelian watersheds. Proc. Natl Acad. Sci. USA 112, 12133–12138 (2015).Article 
    CAS 

    Google Scholar 
    16.Schneider, S. H. The greenhouse effect: science and policy. Science 243, 771–781 (1989).CAS 
    Article 

    Google Scholar 
    17.Walsh, J. et al. Climate Change Impacts in the United States: The Third National Climate Assessment Ch. 2 (US Global Change Research Program, 2014); https://doi.org/10.7930/J0KW5CXT18.Filatova, T., Polhill, J. G. & van Ewijk, S. Regime shifts in coupled socio-environmental systems: review of modelling challenges and approaches. Environ. Model. Softw. 75, 333–347 (2016).Article 

    Google Scholar 
    19.Loarie, S. R. et al. The velocity of climate change. Nature 462, 1052–1055 (2009).CAS 
    Article 

    Google Scholar 
    20.Brandt, M. et al. Reduction of tree cover in West African woodlands and promotion in semi-arid farmlands. Nat. Geosci. 11, 328–333 (2018).CAS 
    Article 

    Google Scholar 
    21.Keys, P. W. et al. Anthropocene risk. Nat. Sustain. 2, 667–673 (2019).Article 

    Google Scholar 
    22.Rockström, J. et al. A safe operating space for humanity. Nature 461, 472–475 (2009).Article 
    CAS 

    Google Scholar 
    23.Steffen, W. et al. Planetary boundaries: guiding human development on a changing planet. Science 347, 1259855 (2015).Article 
    CAS 

    Google Scholar 
    24.Hanan, N. P., Prihodko, L., Ross, C. W., Bucini, G. & Tredennick, A. T. Gridded Estimates of Woody Cover and Biomass across Sub-Saharan Africa, 2000-2004 (ORNL DAAC, 2020); https://doi.org/10.3334/ORNLDAAC/177725.Bouvet, A. et al. An above-ground biomass map of African savannahs and woodlands at 25 m resolution derived from ALOS PALSAR. Remote Sens. Environ. 206, 156–173 (2018).Article 

    Google Scholar 
    26.Avitabile, V. et al. An integrated pan-tropical biomass map using multiple reference datasets. Glob. Change Biol. 22, 1406–1420 (2016).Article 

    Google Scholar 
    27.Saatchi, S. S. et al. Benchmark map of forest carbon stocks in tropical regions across three continents. Proc. Natl Acad. Sci. USA 108, 9899–9904 (2011).CAS 
    Article 

    Google Scholar 
    28.Baccini, A. et al. Estimated carbon dioxide emissions from tropical deforestation improved by carbon-density maps. Nat. Clim. Change 2, 182–185 (2012).CAS 
    Article 

    Google Scholar 
    29.Anchang, J. Y. et al. Toward operational mapping of woody canopy cover in tropical savannas using Google Earth Engine. Front. Environ. Sci. https://doi.org/10.3389/fenvs.2020.00004 (2020).30.Kahiu, M. N. & Hanan, N. P. Fire in sub-Saharan Africa: the fuel, cure and connectivity hypothesis. Glob. Ecol. Biogeogr. 27, 946–957 (2018).Article 

    Google Scholar 
    31.Venter, O. et al. Global terrestrial Human Footprint maps for 1993 and 2009. Sci. Data 3, 160067 (2016).Article 

    Google Scholar 
    32.Ross, C. W. et al. HYSOGs250m, global gridded hydrologic soil groups for curve-number-based runoff modeling. Sci. Data 5, 180091 (2018).Article 

    Google Scholar 
    33.Lüdeke, M. K. B., Moldenhauer, O. & Petschel-Held, G. Rural poverty driven soil degradation under climate change: the sensitivity of the disposition towards the Sahel Syndrome with respect to climate. Environ. Model. Assess. 4, 315–326 (1999).Article 

    Google Scholar 
    34.Hansfort, S. L. & Mertz, O. Challenging the woodfuel crisis in West African woodlands. Hum. Ecol. 39, 583 (2011).Article 

    Google Scholar 
    35.Andela, N. et al. A human-driven decline in global burned area. Science 356, 1356–1362 (2017).CAS 
    Article 

    Google Scholar 
    36.Wei, F. et al. Nonlinear dynamics of fires in Africa over recent decades controlled by precipitation. Glob. Change Biol. 26, 4495–4505 (2020).Article 

    Google Scholar 
    37.Jones, B. & O’Neill, B. C. Spatially explicit global population scenarios consistent with the Shared Socioeconomic Pathways. Environ. Res. Lett. 11, 084003 (2016).Article 

    Google Scholar 
    38.Riahi, K. et al. The Shared Socioeconomic Pathways and their energy, land use, and greenhouse gas emissions implications: an overview. Glob. Environ. Change 42, 153–168 (2017).Article 

    Google Scholar 
    39.Potapov, P. et al. Mapping the World’s intact forest landscapes by remote sensing. Ecol. Soc. 13, 2 (2008).Article 

    Google Scholar 
    40.Herold, M., Mayaux, P., Woodcock, C. E., Baccini, A. & Schmullius, C. Some challenges in global land cover mapping: an assessment of agreement and accuracy in existing 1 km datasets. Remote Sens. Environ. 112, 2538–2556 (2008).Article 

    Google Scholar 
    41.Martens, C. et al. Large uncertainties in future biome changes in Africa call for flexible climate adaptation strategies. Glob. Change Biol. 27, 340–358 (2021).Article 

    Google Scholar 
    42.Smith, W. K. et al. Large divergence of satellite and Earth system model estimates of global terrestrial CO2 fertilization. Nat. Clim. Change 6, 306–310 (2016).Article 
    CAS 

    Google Scholar 
    43.Reich, P. B., Hobbie, S. E. & Lee, T. D. Plant growth enhancement by elevated CO2 eliminated by joint water and nitrogen limitation. Nat. Geosci. 7, 920–924 (2014).CAS 
    Article 

    Google Scholar 
    44.Wieder, W. R., Cleveland, C. C., Smith, W. K. & Todd-Brown, K. Future productivity and carbon storage limited by terrestrial nutrient availability. Nat. Geosci. 8, 441–444 (2015).CAS 
    Article 

    Google Scholar 
    45.Körner, C. A matter of tree longevity. Science 355, 130–131 (2017).Article 

    Google Scholar 
    46.Olson, D. M. & Dinerstein, E. The Global 200: priority ecoregions for global conservation. Ann. Mo. Bot. Gard. 89, 199–224 (2002).Article 

    Google Scholar 
    47.R Core Team. R: A Language and Environment for Statistical Computing (R Foundation for Statistical Computing, 2019).48.Liaw, A. & Wiener, M. Classification and regression by randomForest. R News 2, 18–22 (2002).
    Google Scholar 
    49.Breiman, L. Random forests. Mach. Learn. 45, 5–32 (2001).Article 

    Google Scholar 
    50.Massey, F. J. The Kolmogorov-Smirnov test for goodness of fit. J. Am. Stat. Assoc. 46, 68–78 (1951).Article 

    Google Scholar 
    51.Jarvis, A., Reuter, H. I., Nelson, A. & Guevara, E. Hole-filled SRTM for the globe: version 4: data grid (CGIAR Consortium for Spatial Information, 2008).52.Ross, C. W. et al. Global Hydrologic Soil Groups (HYSOGs250m) for Curve Number-Based Runoff Modeling (ORNL DAAC, 2018); https://doi.org/10.3334/ORNLDAAC/156653.Simard, M., Pinto, N., Fisher, J. B. & Baccini, A. Mapping forest canopy height globally with spaceborne lidar. J. Geophys. Res. https://doi.org/10.1029/2011JG001708 (2011).54.Jucker, T. et al. Allometric equations for integrating remote sensing imagery into forest monitoring programmes. Glob. Change Biol. 23, 177–190 (2017).Article 

    Google Scholar 
    55.Sanderson, E. W. et al. The human footprint and the last of the wild. BioScience 52, 891–904 (2002).Article 

    Google Scholar 
    56.Molnar, C., Bischl, B. & Casalicchio, G. iml: an R package for interpretable machine learning. J. Open Source Softw. 3, 786 (2018).Article 

    Google Scholar 
    57.Wickham, H. tidyverse: Easily Install and Load the ‘Tidyverse’ (CRAN, 2017).58.Hijmans, R. J. et al. raster: Geographic Data Analysis and Modeling (CRAN, 2016).59.Perpiñán, O. & Hijmans, R. rasterVis (CRAN, 2018).60.Wickham, H. ggplot2: Elegant Graphics for Data Analysis (Springer, 2016).61.Zeileis, A. et al. colorspace: A toolbox for manipulating and assessing colors and palettes. J. Stat. Soft. https://doi.org/10.18637/jss.v096.i01 (2020).62.Neuwirth, E. RColorBrewer: ColorBrewer Palettes (CRAN, 2014).63.Auguie, B. gridExtra: Miscellaneous Functions for ‘Grid’ Graphics (CRAN, 2017).64.Pebesma, E. Simple features for R: standardized support for spatial vector data. R J. 10, 439–446 (2018).Article 

    Google Scholar 
    65.Ross, C. W., Hanan, N. P. & Prihodko, L. Prediction Maps: Woody-Biomass Projections and Drivers of Change in Sub-Saharan Africa (Figshare, 2021); https://doi.org/10.6084/M9.FIGSHARE.14150210.V266.Ross, C. W. R Code for Woody-Biomass Projections and Drivers of Change in Sub-Saharan Africa (Figshare, 2021); https://doi.org/10.6084/M9.FIGSHARE.14143799.V1 More

  • in

    Carbon tariffs

    Thank you for visiting nature.com. You are using a browser version with limited support for CSS. To obtain
    the best experience, we recommend you use a more up to date browser (or turn off compatibility mode in
    Internet Explorer). In the meantime, to ensure continued support, we are displaying the site without styles
    and JavaScript. More

  • in

    A biogeochemical–hydrological framework for the role of redox-active compounds in aquatic systems

    1.Gruber, N. & Galloway, J. N. An Earth-system perspective of the global nitrogen cycle. Nature 451, 293–296 (2008).Article 

    Google Scholar 
    2.Zimmerman, J. B., Mihelcic, J. R. & Smith, J. Global stressors on water quality and quantity. Environ. Sci. Technol. 42, 4247–4254 (2008).Article 

    Google Scholar 
    3.Banwart, S. A., Nikolaidis, N. P., Zhu, Y.-G., Peacock, C. L. & Sparks, D. L. Soil functions: connecting Earth’s critical zone. Annu. Rev. Earth Planet. Sci. Lett. 47, 333–359 (2019).Article 

    Google Scholar 
    4.Hartmann, D. L. et al. in Climate Change 2013: The Physical Science Basis (eds Stocker, T. F. et al.) Ch. 2 (Cambridge Univ. Press, 2013).5.Knorr, K. H., Lischeid, G. & Blodau, C. Dynamics of redox processes in a minerotrophic fen exposed to a water table manipulation. Geoderma 153, 379–392 (2009).Article 

    Google Scholar 
    6.McClain, M. E. et al. Biogeochemical hot spots and hot moments at the interface of terrestrial and aquatic ecosystems. Ecosystems 6, 301–312 (2003).Article 

    Google Scholar 
    7.Yabusaki, S. B. et al. Water table dynamics and biogeochemical cycling in a shallow, variably-saturated floodplain. Environ. Sci. Technol. 51, 3307–3317 (2017).Article 

    Google Scholar 
    8.Krause, S. et al. Ecohydrological interfaces as hot spots of ecosystem processes. Water Resour. Res. 53, 6359–6376 (2017).Article 

    Google Scholar 
    9.Stumm W. & Morgan J. J. Aquatic Chemistry, Chemical Equilibria and Rates in Natural Waters 3rd edn (John Wiley & Sons, 1996).10.Aeschbacher, M., Vergari, D., Schwarzenbach, R. P. & Sander, M. Electrochemical analysis of proton and electron transfer equilibria of the reducible moieties in humic acids. Environ. Sci. Technol. 45, 8385–8394 (2011).Article 

    Google Scholar 
    11.Thamdrup, B. Bacterial manganese and iron reduction in aquatic sediments. Adv. Microb. Ecol. 16, 41–84 (2000).Article 

    Google Scholar 
    12.Kostka, J. E. & Nealson, K. H. Dissolution and reduction of magnetite by bacteria. Environ. Sci. Technol. 29, 2535–2540 (1995).Article 

    Google Scholar 
    13.Piepenbrock, A., Dippon, U., Porsch, K., Appel, E. & Kappler, A. Dependence of microbial magnetite formation on humic substance and ferrihydrite concentrations. Geochim. Cosmochim. Acta 75, 6844–6858 (2011).Article 

    Google Scholar 
    14.Amstaetter, K., Borch, T., Larese-Casanova, P. & Kappler, A. Redox transformation of arsenic by Fe(II)-activated goethite (α-FeOOH). Environ. Sci. Technol. 44, 102–108 (2010).Article 

    Google Scholar 
    15.Ilgen, A. G., Foster, A. L. & Trainor, T. P. Role of structural Fe in nontronite NAu-1 and dissolved Fe(II) in redox transformations of arsenic and antimony. Geochim. Cosmochim. Acta 94, 128–145 (2012).Article 

    Google Scholar 
    16.Lan, S. et al. Efficient catalytic As(III) oxidation on the surface of ferrihydrite in the presence of aqueous Mn(II). Water Res. 128, 92–101 (2018).Article 

    Google Scholar 
    17.Lovley, D. R. et al. Humic substances as a mediator for microbially catalyzed metal reduction. Acta Hydroch. Hydrob. 26, 152–157 (1998).Article 

    Google Scholar 
    18.Lovley, D. R., Fraga, J. L., Coates, J. D. & Blunt-Harris, E. L. Humics as an electron donor for anaerobic respiration. Environ. Microbiol. 1, 89–98 (1999).Article 

    Google Scholar 
    19.Peretyazhko, T. & Sposito, G. Reducing capacity of terrestrial humic acids. Geoderma 137, 140–146 (2006).Article 

    Google Scholar 
    20.Heitmann, T. & Blodau, C. Oxidation and incorporation of hydrogen sulfide by dissolved organic matter. Chem. Geol. 235, 12–20 (2006).Article 

    Google Scholar 
    21.Yu, Z. G., Peiffer, S., Goettlicher, J. & Knorr, K. H. Electron transfer budgets and kinetics of abiotic oxidation and incorporation of aqueous sulfide by dissolved organic matter. Environ. Sci. Technol. 49, 5441–5449 (2015).Article 

    Google Scholar 
    22.Rose, A. L. & Waite, T. D. Kinetics of iron complexation by dissolved natural organic matter in coastal waters. Mar. Chem. 84, 85–103 (2003).Article 

    Google Scholar 
    23.Bauer, I. & Kappler, A. Rates and extent of reduction of Fe(III) compounds and O2 by humic substances. Environ. Sci. Technol. 43, 4902–4908 (2009).Article 

    Google Scholar 
    24.Uchimiya, M. & Stone, A. T. Reversible redox chemistry of quinones: impact on biogeochemical cycles. Chemosphere 77, 451–458 (2009).Article 

    Google Scholar 
    25.Borch, T. et al. Biogeochemical redox processes and their impact on contaminant dynamics. Environ. Sci. Technol. 44, 15–23 (2010).Article 

    Google Scholar 
    26.Ilgen, A. G., Kukkadapu, R. K., Leung, K. & Washington, R. E. ‘Switching on’ iron in clay minerals. Environ. Sci. Nano 6, 1704–1715 (2019).Article 

    Google Scholar 
    27.Peiffer, S., dos Santos Afonso, M., Wehrli, B. & Gaechter, R. Kinetics and mechanism of the reaction of hydrogen sulfide with lepidocrocite. Environ. Sci. Technol. 26, 2408–2413 (1992).Article 

    Google Scholar 
    28.Poulton, S. W., Krom, M. D. & Raiswell, R. A revised scheme for the reactivity of iron (oxyhydr)oxide minerals towards dissolved sulfide. Geochim. Cosmochim. Acta 68, 3703–3715 (2004).Article 

    Google Scholar 
    29.Hellige, K., Pollok, K., Larese-Casanova, P., Behrends, T. & Peiffer, S. Pathways of ferrous iron mineral formation upon sulfidation of lepidocrocite surfaces. Geochim. Cosmochim. Acta 81, 69–81 (2012).Article 

    Google Scholar 
    30.Wan, M., Shchukarev, A., Lohmayer, R., Planer-Friedrich, B. & Peiffer, S. Occurrence of surface polysulfides during the interaction between ferric (hydr)oxides and aqueous sulfide. Environ. Sci. Technol. 48, 5076–5084 (2014).Article 

    Google Scholar 
    31.Hedderich, R. et al. Anaerobic respiration with elemental sulfur and with disulfides. FEMS Microbiol. Rev. 22, 353–381 (1998).Article 

    Google Scholar 
    32.Milucka, J. et al. Zero-valent sulphur is a key intermediate in marine methane oxidation. Nature 491, 541–546 (2012).Article 

    Google Scholar 
    33.Poser, A. et al. Disproportionation of elemental sulfur by haloalkaliphilic bacteria from soda lakes. Extremophiles 17, 1003–1012 (2013).Article 

    Google Scholar 
    34.Aeppli, M. et al. Decreases in iron oxide reducibility during microbial reductive dissolution and transformation of ferrihydrite. Environ. Sci. Technol. 53, 8736–8746 (2019).Article 

    Google Scholar 
    35.Aeppli, M. et al. Electrochemical analysis of changes in iron oxide reducibility during abiotic ferrihydrite transformation into goethite and magnetite. Environ. Sci. Technol. 53, 3568–3578 (2019).Article 

    Google Scholar 
    36.Klüpfel, L., Piepenbrock, A., Kappler, A. & Sander, M. Humic substances as fully regenerable electron acceptors in recurrently anoxic environments. Nat. Geosci. 7, 195–200 (2014).Article 

    Google Scholar 
    37.Blodau, C. Carbon cycling in peatlands—a review of processes and controls. Environ. Rev. 10, 111–134 (2002).Article 

    Google Scholar 
    38.Gao, C., Sander, M., Agethen, S. & Knorr, K.-H. Electron accepting capacity of dissolved and particulate organic matter control CO2 and CH4 formation in peat soils. Geochim. Cosmochim. Acta 245, 266–277 (2019).Article 

    Google Scholar 
    39.Schaefer, M. V., Gorski, C. A. & Scherer, M. M. Spectroscopic evidence for interfacial Fe(II)–Fe(III) electron transfer in a clay mineral. Environ. Sci. Technol. 45, 540–545 (2011).Article 

    Google Scholar 
    40.Pentrakova, L., Su, K., Pentrak, M. & Stucko, J. W. A review of microbial redox interactions with structural Fe in clay minerals. Clay Miner. 48, 543–560 (2013).Article 

    Google Scholar 
    41.Kostka, J. E., Dalton, D. D., Skelton, H., Dollhopf, S. & Stucki, J. W. Growth of iron(III)-reducing bacteria on clay minerals as the sole electron acceptor and comparison of growth yields on a variety of oxidized iron forms. Appl. Environ. Microbiol. 68, 6256–6262 (2002).Article 

    Google Scholar 
    42.Li, Y. L. et al. Iron reduction and alteration of nontronite NAu-2 by a sulfate-reducing bacterium. Geochim. Cosmochim. Acta 68, 3251–3260 (2004).Article 

    Google Scholar 
    43.Liu, D. et al. Reduction of structural Fe(III) in nontronite by methanogen Methanosarcina barkeri. Geochim. Cosmochim. Acta 75, 1057–1071 (2011).Article 

    Google Scholar 
    44.Zhang, J., Dong, H., Liu, D. & Agrawal, A. Microbial reduction of Fe(III) in smectite minerals by thermophilicmethanogen Methanothermobacter thermautotrophicus. Geochim. Cosmochim. Acta 106, 203–215 (2013).Article 

    Google Scholar 
    45.Shelobolina, E. et al. Microbial lithotrophic oxidation of structural Fe(II) in biotite. Appl. Environ. Microbiol. 78, 5746–5752 (2012).Article 

    Google Scholar 
    46.Gorski, C. A. et al. Redox properties of structural Fe in clay minerals. 1. Electrochemical quantification of electron-donating and -accepting capacities of smectites. Environ. Sci. Technol. 46, 9360–9368 (2012).Article 

    Google Scholar 
    47.Blodau, C., Mayer, B., Peiffer, S. & Moore, T. R. Support for an anaerobic sulfur cycle in two Canadian peatland soils. J. Geophys. Res. 112, G000364 (2007).
    Google Scholar 
    48.Gauci, V., Dise, N. & Fowler, D. Controls on suppression of methane flux from a peat bog subjected to simulated acid rain sulfate deposition. Glob. Biogeochem. Cycles 16, GB001370 (2002).Article 

    Google Scholar 
    49.Pester, M., Knorr, K. H., Friedrich, M. W., Wagner, M. & Loy, A. Sulfate-reducing microorganisms in wetlands—fameless actors in carbon cycling and climate change. Front. Microbiol. 3, 72 (2012).Article 

    Google Scholar 
    50.Hansel, C. M., Ferdelman, T. G. & Tebo, B. M. Cryptic cross-linkages among biogeochemical cycles: novel insights from reactive intermediates. Elements 11, 409–414 (2015).Article 

    Google Scholar 
    51.Kappler, A. & Bryce, C. Cryptic biogeochemical cycles: unravelling hidden redox reactions. Environ. Microbiol. 19, 842–846 (2017).Article 

    Google Scholar 
    52.Holmkvist, L., Ferdelman, T. G. & Jørgensen, B. B. A cryptic sulfur cycle driven by iron in the methane zone of marine sediment (Aarhus Bay, Denmark). Geochim. Cosmochim. Acta 75, 3581–3599 (2011).Article 

    Google Scholar 
    53.Hansel, C. M. et al. Dominance of sulfur-fueled iron oxide reduction in low-sulfate freshwater sediments. ISME J. 9, 2400–2412 (2015b).Article 

    Google Scholar 
    54.Findlay, A. J. Microbial impact on polysulfide dynamics in the environment. FEMS Microbiol. Lett. https://doi.org/10.1093/femsle/fnw103(2016).55.Berg, J. S. et al. Intensive cryptic microbial iron cycling in the low iron water column of the meromictic Lake Cadagno. Environ. Microbiol. 18, 5288–5302 (2016).Article 

    Google Scholar 
    56.Peng, C., Bryce, C., Sundman, A. & Kappler, A.Cryptic cycling of complexes containing Fe(III) and organic matter by phototrophic Fe(II)-oxidizing bacteria. Appl. Environ. Microbiol. 85, e02826-18 (2019).Article 

    Google Scholar 
    57.Bethke, C. M., Sanford, R. A., Kirk, M. F., Jin, Q. & Flynn, T. M. The thermodynamic ladder in geomicrobiology. Am. J. Sci. 311, 183–210 (2011).Article 

    Google Scholar 
    58.Otte, J. M. et al. The distribution of active iron cycling bacteria in marine and freshwater sediments is decoupled from geochemical gradients. Environ. Microbiol. 20, 2483–2499 (2018).Article 

    Google Scholar 
    59.Steefel, C. I. & van Cappellen, P. A new kinetic approach to modeling water–rock interaction: the role of nucleation, precursors, and Ostwald ripening. Geochim. Cosmochim. Acta 54, 2657–2677 (1990).Article 

    Google Scholar 
    60.Vinson, D. S., Block, S. E., Crossey, L. J. & Dahm, C. N. Biogeochemistry at the zone of intermittent saturation: field-based study of the shallow alluvial aquifer, Rio Grande, New Mexico. Geosphere 3, 366–380 (2007).Article 

    Google Scholar 
    61.Frei, S., Knorr, K., Peiffer, S. & Fleckenstein, J. Surface micro-topography causes hot spots of biogeochemical activity in wetland systems: a virtual modeling experiment. J. Geophys. Res. Biogeosciences 117, G00N12 (2012).Article 

    Google Scholar 
    62.Briggs, M. A. et al. A physical explanation for the development of redox microzones in hyporheic flow. Geophys. Res. Lett. 42, 4402–4410 (2015).Article 

    Google Scholar 
    63.Stockdale, A., Davison, W. & Zhang, H. Micro-scale biogeochemical heterogeneity in sediments: a review of available technology and observed evidence. Earth Sci. Rev. 92, 81–97 (2009).Article 

    Google Scholar 
    64.Sawyer, A. H. Enhanced removal of groundwater-borne nitrate in heterogeneous aquatic sediments. Geophys. Res. Lett. 42, 403–410 (2015).Article 

    Google Scholar 
    65.Arora, B., Dwivedi, D., Hubbard, S. S., Steefel, C. I. & Williams, K. H. Identifying geochemical hot moments and their controls on a contaminated river floodplain system using wavelet and entropy approaches. Environ. Model. Softw. 85, 27–41 (2016).Article 

    Google Scholar 
    66.Sawyer, A. H., Kaplan, L. A., Lazareva, O. & Michael, H. A. Hydrologic dynamics and geochemical responses within a floodplain aquifer and hyporheic zone during Hurricane Sandy. Water Resour. Res. 50, 4877–4892 (2014).Article 

    Google Scholar 
    67.Posth, N., Canfield, D. E. & Kappler, A. Biogenic Fe(III) minerals: from formation to diagenesis and preservation in the rock record. Earth Sci. Rev. 135, 103–121 (2014).Article 

    Google Scholar 
    68.Tomaszewski, E. J., Cronk, S. S., Gorski, C. A. & Ginder-Vogel, M. The role of dissolved Fe(II) concentration in the mineralogical evolution of Fe (hydr)oxides during redox cycling. Chem. Geol. 438, 163–170 (2016).Article 

    Google Scholar 
    69.Bishop, M. E. et al. Reactivity of redox cycled Fe-bearing subsurface sediments towards hexavalent chromium reduction. Geochim. Cosmochim. Acta 252, 88–106 (2019).Article 

    Google Scholar 
    70.Bartsch, S. et al. River–aquifer exchange fluxes under monsoonal climate conditions. J. Hydrol. 509, 601–614 (2014).Article 

    Google Scholar 
    71.McAllister, S. M. et al. Dynamic hydrologic and biogeochemical processes drive microbially enhanced iron and sulfur cycling within the intertidal mixing zone of a beach aquifer. Limnol. Oceanogr. 60, 329–345 (2015).Article 

    Google Scholar 
    72.Goldberg, S. D., Knorr, K. ‐H., Blodau, C., Lischeid, G. & Gebauer, G. Impact of altering the water table height of an acidic fen on N2O and NO fluxes and soil concentrations. Glob. Change Biol. 16, 220–233 (2010).Article 

    Google Scholar 
    73.Moore, T. R. et al. A multi-year record of methane flux at the Mer Bleue bog, Southern Canada. Ecosystems 14, 646–657 (2011).Article 

    Google Scholar 
    74.Brown, M. G., Humphreys, E. R., Moore, T. R., Roulet, N. T. & Lafleur, P. M. Evidence for a nonmonotonic relationship between ecosystem-scale peatland methane emissions and water table depth. J. Geophys. Res. Biogeosciences 119, 826–835 (2014).Article 

    Google Scholar 
    75.Estop-Aragonés, C., Zając, K. & Blodau, C. Effects of extreme experimental drought and rewetting on CO2 and CH4 exchange in mesocosms of 14 European peatlands with different nitrogen and sulfur deposition. Glob. Change Biol. 22, 2285–2300 (2016).Article 

    Google Scholar 
    76.Chamberlain, S. D. et al. Soil properties and sediment accretion modulate methane fluxes from restored wetlands. Glob. Change Biol. 24, 4107–4121 (2018).Article 

    Google Scholar 
    77.Arora, B. et al. Influence of hydrological, biogeochemical and temperature transients on subsurface carbon fluxes in a flood plain environment. Biogeochemistry 127, 367–396 (2016).Article 

    Google Scholar 
    78.Frei, S. & Peiffer, S. Exposure times rather than residence times control redox transformation efficiencies in Riparian Wetlands. J. Hydrol. 543, 182–196 (2016).Article 

    Google Scholar 
    79.Dwivedi, D., Arora, B., Steefel, C. I., Dafflon, B. & Versteeg, R. Hot spots and hot moments of nitrogen in a riparian corridor. Water Resour. Res. 54, 205–222 (2018).Article 

    Google Scholar 
    80.Peiffer, S., Klemm, O., Pecher, K. & Hollerung, R. Redox measurements in aqueous solutions—a theoretical approach to data interpretation, based on electrode kinetics. J. Contam. Hydrol. 10, 1–18 (1992).Article 

    Google Scholar 
    81.Wainwright, H. M. et al. Hierarchical Bayesian method for mapping biogeochemical hot spots using induced polarization imaging. Water Resour. Res. 52, 533–551 (2016).Article 

    Google Scholar 
    82.Mellage, A. et al. Sensing coated iron-oxide nanoparticles with spectral induced polarization (SIP): experiments in natural sand packed flow-through columns. Environ. Sci. Technol. 52, 14256–14265 (2018).Article 

    Google Scholar 
    83.Revil, A., Florsch, N. & Mao, D. Induced polarization response of porous media with metallic particles—part 1: a theory for disseminated semiconductors. Geophysics 80, D525–D538 (2015).Article 

    Google Scholar 
    84.Revil, A., Abdel Aal, G. Z., Atekwana, E. A., Mao, D. & Florsch, N. Induced polarization response of porous media with metallic particles—part 2: comparison with a broad database of experimental data. Geophysics 80, D539–D552 (2015).Article 

    Google Scholar 
    85.Pausch, J. & Kuzyakov, Y. Carbon input by roots into the soil: quantification of rhizodeposition from root to ecosystem scale. Glob. Change Biol. 24, 1–12 (2018).Article 

    Google Scholar 
    86.Dwivedi, D. et al. Geochemical exports to river from the intrameander hyporheic zone under transient hydrologic conditions: East River mountainous watershed, Colorado. Water Resour. Res. 54, 8456–8477 (2018).Article 

    Google Scholar 
    87.Jin, Q. & Bethke, C. M. The thermodynamics and kinetics of microbial metabolism. Am. J. Sci. 307, 643–677 (2007).Article 

    Google Scholar 
    88.Nitzsche, K. S. et al. Arsenic removal from drinking water by a household sand filter in Vietnam—effect of filter usage practices on arsenic removal efficiency and microbiological water quality. Sci. Total Environ. 502, 526–536 (2015).Article 

    Google Scholar 
    89.Appelo, C. A. J. & Postma, D. Geochemistry, Groundwater and Pollution (CRC Press, 2004).90.Brazhkin, V. V. Metastable phases and ‘metastable’ phase diagrams. J. Phys. Condens. Matter 18, 9643–9650 (2006).Article 

    Google Scholar 
    91.Cornell, R. M. & Schwertmann, U. The Iron Oxides: Structure, Properties, Reactions, Occurrences and Uses (Wiley-VCH, 2006).92.Ahmed, I. A. M. & Maher, B. A. Identification and paleoclimatic significance of magnetite nanoparticles in soils. Proc. Natl Acad. Sci. USA 115, 1736–1741 (2018).Article 

    Google Scholar 
    93.Engel, M. H. & Macko, S. A. Organic Geochemistry. Principles and Applications (Springer, 1993).94.Lovley, D. R. & Phillips, E. J. P. Novel mode of microbial energy metabolism: organic carbon oxidation coupled to dissimilatory reduction of iron or manganese. Appl. Environ. Microbiol. 54, 1472–1480 (1988).Article 

    Google Scholar 
    95.Gorski, C. A. & Scherer, M. M. in Aquatic Redox Chemistry (eds Tratnyek, P. G. et al.) 315–343 (ACS, 2011).96.Orsetti, S., Laskov, C. & Haderlein, S. B. Electron transfer between iron minerals and quinones: estimating the reduction potential of the Fe(II)–goethite surface from AQDS speciation. Environ. Sci. Technol. 47, 14161–14168 (2013).Article 

    Google Scholar 
    97.Gorski, C. A., Edwards, R., Sander, M., Hofstetter, T. B. & Stewart, S. M. Thermodynamic characterization of iron oxide–aqueous Fe2+ redox couples. Environ. Sci. Technol. 50, 8538–8547 (2016).Article 

    Google Scholar 
    98.Byrne, J. M. et al. Redox cycling of Fe(II) and Fe(III) in magnetite by Fe-metabolizing bacteria. Science 347, 1473–1476 (2015).Article 

    Google Scholar  More